Interdependence of Thyroid and Corticosteroid Signaling in Vertebrate Developmental Transitions

Abstract

Post-embryonic acute developmental processes mainly allow the transition from one life stage in a specific ecological niche to the next life stage in a different ecological niche. Metamorphosis, an emblematic type of these post-embryonic developmental processes, has occurred repeatedly and independently in various phylogenetic groups throughout metazoan evolution, such as in cnidarian, insects, molluscs, tunicates, or vertebrates. This review will focus on metamorphoses and developmental transitions in vertebrates, including typical larval metamorphosis in anuran amphibians, larval and secondary metamorphoses in teleost fishes, egg hatching in sauropsids and birth in mammals. Two neuroendocrine axes, the hypothalamic-pituitary-thyroid and the hypothalamic-pituitary-adrenal/interrenal axes, are central players in the regulation of these life transitions. The review will address the molecular and functional evolution of these axes and their interactions. Mechanisms of integration of internal and environmental cues, and activation of these neuroendocrine axes represent key questions in an “eco-evo-devo” perspective of metamorphosis. The roles played by developmental transitions in the innovation, adaptation, and plasticity of life cycles throughout vertebrates will be discussed. In the current context of global climate change and habitat destruction, the review will also address the impact of environmental factors, such as global warming and endocrine disruptors on hypothalamic-pituitary-thyroid and hypothalamic-pituitary-adrenal/interrenal axes, and regulation of developmental transitions.

Introduction

The hypothalamic-pituitary-thyroid (HPT) axis is the neuroendocrine thyrotropic axis, which literally acts (“trope”) on the thyroid gland (“thyro”). In a simplified way, it is composed of brain thyrotropin-releasing hormone (TRH) neurons, pituitary thyrotropin (TSH) cells, and peripheral thyroid hormones (TH), thyroxine (T₄) and triiodothyronine (T₃). TRH acts via its receptor (TRH-R) expressed by the pituitary thyrotropes, and stimulates the synthesis and release of pituitary TSH. TSH binds its receptor (TSH-R) expressed by the thyroid gland to induce the production and release of T₄. At target tissues, T₄ is transformed into T₃ by monodeiodinases, and both bind to TH nuclear receptor, TR. TH can act on various tissues and they negatively feedback on the brain (hypothalamic TRH)/pituitary (TSH) axis (Zoeller et al., 2007).

The hypothalamic-pituitary-adrenal axis (HPA), in mammals and sauropsids, and hypothalamic-pituitary-interrenal (HPI), in amphibians and teleosts, is the neuroendocrine corticotropic axis responsible for the response to stress in all vertebrates (Gorissen and Flik, 2016). The neurohormone, corticotropin-releasing hormone (CRH), controls the production and release of corticotropin (also named adrenocorticotropic hormone, ACTH), at the pituitary level. ACTH acts to control the production and release of corticosteroids (CS) from adrenal cortex cells in amniotes or interrenal cells in amphibians and teleosts. CS can act on various tissues and they negatively feedback on the brain (hypothalamic CRH) / pituitary (ACTH) corticotropic axis (Bernier et al., 2009; Faught et al., 2016; Gorissen and Flik, 2016) via specific receptors.

The molecular components of the HPT and HPA/HPI axes have been subject to whole genome duplication (WGD) events during evolution. Two events of WGD, referred to as 1R and 2R for first and second rounds of WGD, occurred in ancestral vertebrates (Dehal and Boore, 2005). An additional WGD event occurred in ancestral teleosts, referred to as 3R for third round of WGD or as teleost specific WGD (Meyer and Schartl, 1999). A further WGD occurred more recently in some teleost groups, such as salmonids (Lien et al., 2016) and some carps (Wang et al., 2012). This event is referred to as 4R (fourth round of WGD). The WGD were at the origin of the diversification of the functions of the HPT and HPA/HPI axis.

One of the actions controlled by the HPT and HPA/HPI axis in vertebrates is the developmental body change coming from a need to adapt to a remarkable change in habitat during birth, hatching or post-embryonic development events. Dramatic changes occur in various metazoa such as cnidaria, insects, crustacean, molluscs, tunicates, and vertebrates. These events have been collectively termed as metamorphosis from the Greek meta- (change) and morph (form). Metamorphosis has a major role in the structure of complex life cycles encompassing different ecophases. In vertebrates, different developmental modes are observed. Amniotes, namely mammals, and sauropsids (birds and reptiles), as well as some amphibians, go through direct development and present a more mature stage at birth/hatching, with an earlier ontogeny of the HPA axis. Non-amniotes, comprising various fish and amphibians, go through indirect development with metamorphosis and present a more immature stage at hatching with a later ontogeny of the HPT and HPA/HPI axis. All the post-embryonic developmental changes are hormonally controlled processes by TH (Paris and Laudet, 2008), but recent studies confer to CS an increasingly prominent role (Sachs and Buchholz, 2017). These TH and CS actions allow to distinguish this period from other major late developmental events such as puberty, which is under the control of sexual steroids.

The post-embryonic developmental transitions are also sensitive to diverse biotic and abiotic factors that can profoundly influence behavior, morphology, growth, development, and sometimes survival. Vertebrates respond to the exposome by modulating the production of CS and TH (Figure 1). The adaptive response allows to adjust the timing of the developmental program, but with a trade-off between risk and benefit.

FIGURE 1

Molecular and Functional Evolution of the Hypothalamic-Pituitary-Thyroid and the Hypothalamic-Pituitary-Adrenal/Interrenal Axes and Their Interactions

Hypothalamic-Pituitary-Thyroid Axis

Thyrotropin-Releasing Hormone and Its Receptors

The hypothalamic-pituitary-thyroid (HPT) axis is the neuroendocrine thyrotropic axis (Figure 2). After indirect evidence of the existence of a thyrotropin-releasing factor in dogs (Shibusawa et al., 1955), a fraction, purified from bovine or ovine hypothalamic extracts, was found to stimulate the release of TSH (Schreiber et al., 1961; Guillemin et al., 1962, 1963). The TRH gene encodes multiple identical repeats of the three amino-acid (pyroglutamic acid-histidine-proline) TRH sequence (Galas et al., 2009). This is an example of intragenic duplication which allows an amplification of the synthesis and production of this neurohormone.

FIGURE 2

TRH-R are members of membrane class A G-protein coupled receptors (GPCR). Two subtypes, TRH-R1 and TRH-R2, have been characterized in mammals. A third one, TRH-R3, has been identified in birds (Li et al., 2020), amphibians (Bidaud et al., 2002), reptiles (Li et al., 2020), and teleosts (Mekuchi et al., 2011; Saito et al., 2011; Li et al., 2020). In birds, only TRH-R1 and TRH-R3 have been identified so far (Li et al., 2020). Four subtypes have been cloned in sockeye salmon Oncorhynchus nerka (TRH-R1, TRH-R2a, TRH-R2b, and TRH-R3; Saito et al., 2011), and in medaka Oryzias latipes (TRH-R1a, TRH-R1b, TRH-R2, and TRH-R3; Mekuchi et al., 2011). As in medaka (Mekuchi et al., 2011), duplicated TRH-R1a and b are found in many teleosts including zebrafish Danio rerio, and might be the result of 3R, even if only one TRH-R1 is identified in sockeye salmon (Saito et al., 2011). The duplicated TRH-R2s present in sockeye salmon may be due to the 4R; TRH-R2b is truncated (Saito et al., 2011). According to the recent hypothesis of Li et al. (2020) on the evolutionary history of TRH-Rs, multiple gene loss events might have occurred during evolution, including TRH-R2 loss in birds, and many mammals, as well as TRH-R3 loss in mammals. Interestingly, pituitary TRH-R3 expression was recently shown to elevate as metamorphosis progressed in bullfrog tadpole (Nakano et al., 2018). It would be interesting to investigate whether the possible involvement of TRH-R3 in amphibian metamorphosis is also observed in other major life history transitions, such as teleost metamorphoses and sauropsid hatching.

Thyrotropin and Its Receptors

TSH is a glycoprotein hormone composed of two subunits, the alpha subunit (Gpα) common to gonadotropins, and the hormone-specific TSHβ subunit, which is paralogous to the luteinising hormone (LH) and follicle-stimulating hormone (FSH) β subunits. The genes encoding the β subunits of the two gonadotropins LH, FSH and of TSH are paralogous genes that likely arose from the two successive 1R/2R in ancestral vertebrates. A single TSHβ is present in mammals and other tetrapods, as well as in actinopterygians, and is considered as the “classical” TSH. Its β subunit is now named TSHβ1 since a second TSHβ, called TSHβ2, has been identified in some representative species of early vertebrates such as in chondrichthyans and basal sarcopterygians (Maugars et al., 2014). These data suggest that the gene coding for tshβ2 was lost twice independently during osteichthyan evolution, in a tetrapod ancestor and in an actinopterygian ancestor. Indeed tshβ2 could not be retrieved in the genome of an holostean (spotted gar Lepisosteus oculatus) nor any teleosts, supporting an early loss of tshβ2 in the actinopterygian lineage, leading to inheritance of only tshβ1 by the teleost lineage (Maugars et al., 2014). Two tshβ paralogs were found in teleosts, resulting from the 3R duplication of tshβ1 (Maugars et al., 2014; Fleming et al., 2019), and named tshβ1a and tshβ1b (Fleming et al., 2019). Recently, up to three tshβ1 paralogs were identified in Oncorhynchus species, due to the conservation of the duplicated 4R-paralogs of tshβ1a (tshβ1aα and tshβ1aβ) while only the two tshβ1 paralogs issued from 3R (tshβ1a and tshβ1b) are present in Atlantic salmon Salmo salar as in other teleosts (Fleming et al., 2019). Interestingly, the two tshβ paralogs identified in Atlantic salmon are expressed in different pituitary cells (Fleming et al., 2019): tshβ1a in the anterior adenohypophysis, and tshβ1b in cells near to the pituitary stalk, cells comparable to the pars tuberalis TSH cells involved in seasonal physiology and behavior in birds (Yoshimura, 2013) and mammals (Dardente et al., 2019).

TSH-R is present at the surface of the thyroid follicle cells in the thyroid gland. It belongs to the class A GPCR receptors and is paralogous to the receptors for gonadotropins. In teleosts, due to the 3R, duplicated receptors tshra and tshrb have been characterized (Maugars et al., 2014). TSH-R are not only expressed in the thyroid gland, but also in a variety of other tissues (Williams, 2011). Of particular interest is the presence of tshr in the brain and the gonads, where they mediate TSH retrograde action on brain deiodinase and direct regulatory effect on reproduction, in birds and mammals (Nakane and Yoshimura, 2019).

Thyroid Hormones and Their Receptors

Two main forms of TH are found in vertebrates, T₄ with four iodinated tyrosine residues (3,3′,5,5′), the hormonal precursor produced by the thyroid gland, and T₃ with three iodinated tyrosine residues (3,3′,5), the active hormone which binds to TR with a 10-fold higher affinity compared to T₄ (Holzer et al., 2017). T₄ is produced, by thyrocytes under TSH control, from thyroglobulin, a large dimeric protein containing many tyrosine residues.

TR belong to the nuclear receptor superfamily. Two homologous receptors, TRα and TRβ, are present in tetrapods (Sap et al., 1986; Weinberger et al., 1986; Thompson et al., 1987; Brooks et al., 1989; Helbing et al., 2006; Kanaho et al., 2006). The 3R led to two duplicated trα paralogs and two duplicated trβ paralogs in basal teleosts, such as conger and eel. So far, four tr cDNAs have been cloned in Japanese flounder: two α types and two β types (Yamano et al., 1994; Yamano and Inui, 1995). In some other teleosts, such as zebrafish, two trα genes but a single trβ gene have been retrieved, suggesting that one of the trβ duplicated paralog would have been lost in the course of teleost evolution (Lazcano and Orozco, 2018). Xenopus laevis possesses two distinctive genes for each tr likely due to its genome polyploidisation (Yaoita et al., 1990). In tetrapods, alternative splicing of TR leads to various protein isoforms with different binding activities and biological functions. In mammals, two TRα variants (α1 and α2) are thus generated from a single gene (Izumo and Mahdavi, 1988). Similarly, in addition to the 3R-duplicated genes, alternative splicing may lead to a large variety of TR isoforms in teleosts, with species-specific variations (Marchand et al., 2001).

Deiodinases

Deiodination of TH corresponds to the removal of iodine from their outer or inner rings, and is performed by iodothyronine deiodinase enzymes in the thyroid, peripheral or central target tissues. By regulating the bioavailability of T₄ and T₃, they thus control their action (Bianco et al., 2002; Orozco and Valverde-R, 2005; Darras and Van Herck, 2012; Orozco et al., 2012; Steegborn and Schweizer, 2020). The first deiodinase to be cloned was dio1 from rat (Berry et al., 1991), then dio3 was cloned from Xenopus laevis (St. Germain et al., 1994), and dio2 from Rana catesbeiana (Davey et al., 1995). So far, these three types of iodothyronine deiodinases, DIO1, DIO2, and DIO3, have been identified in most vertebrates (Bianco et al., 2002; Darras and Van Herck, 2012; Orozco et al., 2012). DIO1 is a low selectivity enzyme with both outer and inner ring deiodinase activity. DIO2 is an outer ring deiodinase, which removes an iodine residue from T₄ and gives active T₃. DIO3 is an inner ring deiodinase, which inactivates T₄ and T₃ in reverse T₃ (rT₃ or 3,3′,5′-T₃), and diiodothyronine (T₂ or 3,3′-T₂), respectively. Orozco et al. (2012) reviewed the evolutionary history of deiodinase family and point out that dio1 is the oldest vertebrate deiodinase gene and dio2 the most recent one. Some teleosts possess 3R-duplicated dio2 and dio3 genes (Orozco et al., 2012; Alves et al., 2017). The widespread and differential tissue distribution for the three types of deiodinase in vertebrates has been reviewed previously (Darras and Van Herck, 2012; Orozco et al., 2012). In the Atlantic salmon, up to six deiodinase paralogs have been characterized, one dio1, two dio2 (dio2a and dio2b) and three dio3 (dio3a1, dio3a2, and dio3b) (Lorgen et al., 2015). A single dio2 gene is present in Northern pike Esox lucius (Rondeau et al., 2014), which suggests that the two dio2 paralogs of the Atlantic salmon arose recently from the salmonid-specific WGD, 4R (Lorgen et al., 2015). Dio3a1/3a2 likely also resulted from 4R (Lorgen et al., 2015). Functional divergence of the two salmon dio2 paralogs is reported: while gill dio2a expression is induced by seawater exposure (Lorgen et al., 2015), dio2b expression in the brain is sensitive to photoperiod during smoltification (Lorgen et al., 2015; Irachi et al., 2021).

Hypothalamic-Pituitary-Adrenal/Interrenal

Corticotropin-Releasing Hormone and Its Receptors

The hypothalamic-pituitary-adrenal axis (HPA), in mammals and sauropsids, and hypothalamic-pituitary-interrenal (HPI), in amphibians and teleosts, is the neuroendocrine corticotropic axis (Figure 3). In 1955, a substance, present in extracts of mammalian hypothalamus and able to stimulate ACTH secretion in vitro, was named corticotropin-releasing factor (CRF) (Guillemin and Rosenberg, 1955; Saffran et al., 1955). CRF (or CRH) was first isolated from sheep hypothalamus (Vale et al., 1981) and identified in all vertebrates thereafter (Lovejoy et al., 2014; On et al., 2019). Together with urotensin I (UI) in teleosts, sauvagine (SVG) in amphibians, and urocortins (Ucn) in mammals, it forms a large family of peptides, the CRH/urocortin family. As CRH, urotensin I, sauvagine and urocortins have roles in the regulation of ACTH and MSH, as well as energy metabolism and reproduction (Lovejoy and Balment, 1999). It was first suggested that two ancestral crh/ucn1 and ucn2/ucn3 genes likely arose by specific gene duplication before vertebrate WGD events (Hwang et al., 2013), as a single crh-like gene is identified in amphioxus and tunicates (On et al., 2019). Both ancestral genes were duplicated twice in ancestral vertebrates via 1R and 2R, followed by some paralog losses, leading to up to 5 genes (crh1, crh2, ucn1 coming from ancestral crh/ucn1; ucn2, ucn3 issued from ancestral ucn2/ucn3) in extant representative species of some vertebrate lineages such as chondrichthyans, holosteans and actinistians (Cardoso et al., 2016; On et al., 2019). Teleost specific 3R resulted in the duplication of crh1 into two paralogs crh1a and crh1b conserved in many species (Grone and Maruska, 2015; Cardoso et al., 2016). Crh2 may have been lost in recent teleosts (Cardoso et al., 2016), while one 3R-crh2 paralog has been conserved in basal groups of teleosts such as European eel (Maugars et al., 2016).

FIGURE 3

In tetrapods, CRH has been shown to act via two GPCRs, corticotropin-releasing hormone receptors (CRHR), CRHR1, and CRHR2, which belong to the class 2 subfamily B1 of secretin-like GPCR superfamily (Lovejoy et al., 2014). Crhr1 was duplicated by 3R into two paralogs (crhr1a and crhr1b) which were conserved in many extant teleosts, while one of 3R-duplicated crhr2 paralogs would have been lost (Cardoso et al., 2016). A third CRHR, CRHR3, identified in the catfish, Ameiurus nebulosus (Arai et al., 2001), highly similar to catfish CRHR1, likely results from gene-specific duplication, that may also occurred in various teleosts (Lovejoy et al., 2014; Cardoso et al., 2016).

Proopiomelanocortin-Derived Peptides and Their Receptors

The main pituitary hormone involved in the HPA/HPI axis is ACTH. ACTH is derived from tissue-specific post-translational processing of its precursor, the proopiomelanocortin (POMC); POMC also gives rise to melanocyte stimulating hormone (MSH), and β-endorphin (β-END). POMC forms the opioid/orphanin gene family together with proenkephalin, prodynorphin and proorphanin (Dores et al., 2002; Sundström et al., 2010). ACTH and MSH, called melanocortins (MC), act via MC receptors (MCR), while β-END acts via opioid receptor. Teleost 3R gave rise to pomc gene duplicates: pomc-α (a or A) and pomc-β (b or B), with pomc-β having lost a functional β-endorphin (De Souza et al., 2005). Further independent gene-specific duplications during teleost evolution resulted in duplicates of pomc-α, such as in sea bream Sparus aurata (Cardoso et al., 2011) and Astatotilapia burtoni (Harris et al., 2014).

Melanocortin receptors (MCR) belong to the rhodopsin class A13 family of GPCRs. In tetrapods, five MCR genes have been identified: mc1r to mc5r (Cortés et al., 2014; Dores et al., 2014). In teleost fish, probably due to 3R, the number of receptors increases up to six in zebrafish, which has two MC5R paralogs (Västermark and Schiöth, 2011), while pufferfish Fugu rubripes has only four, with no mc3r and only one copy of mc5r (Logan et al., 2003). Concerning the ligand selectivity of MCRs, all of the paralogous MCRs can be activated by both ACTH and MSH in extant cartilaginous fishes, while in extant teleosts and tetrapods, only ACTH can activate MC2R (Cortés et al., 2014; Dores et al., 2014). In mammals, the MCRs have distinct tissue expression (Cone, 2006; Dores et al., 2014): mc1r is mainly expressed in melanocytes; mc2r in adrenal cortex; mc3r and mc4r in the brain; and mc5r in a variety of exocrine glands, such as sebaceous, lacrimal and preputial glands. In concordance with their expression sites, each MCR has its proper function: MC1R is involved in skin and hair pigmentation; MC2R in adrenal steroidogenesis and stress response; MC3R and MC4R in energy homeostasis; and MC5R in exocrine gland secretion. These features can also be observed in non-mammalian vertebrates, with some differences. Of particular interest, mc5r is co-expressed with mc2r in the interrenal of Xenopus tropicalis (Dores and Garcia, 2015) and several teleosts [rainbow trout Oncorhynchus mykiss (Haitina et al., 2004; Aluru and Vijayan, 2008); common carp Cyprinus carpio (Metz et al., 2005); barfin flounder Verasper moseri (Kobayashi et al., 2011)], as well as in the chicken adrenal (Takeuchi and Takahashi, 1998), suggesting a possible role of MC5R, in addition to MC2R, in the regulation of HPI axis in these non-mammalian vertebrates.

Corticosteroids and Their Receptors

Corticosteroids (CS) are steroid hormones, divided into glucocorticoids (GC), and mineralocorticoids (MC). In mammals and sauropsids, CS are synthetized by the adrenal gland. In amphibians and teleosts, CS are synthetized by the interrenal gland, a tissue embedded inside the anterior part of the kidney (head kidney) and homologous to the adrenal cortex of the adrenal gland in mammals (Chester-Jones, 1987). Cortisol is the primary GC in most mammals and teleosts, while it is corticosterone in birds, reptiles, amphibians and many rodents (Mommsen et al., 1999; Aerts, 2018). Both GC can co-exist in most vertebrates. Aldosterone, which is the principal MC in mammals (Gilmour, 2005), is lacking in all teleosts studied so far. In teleosts, it is generally accepted that cortisol plays both GC and MC roles (McCormick, 2001; McCormick et al., 2008).

GC and MC receptors (respectively, GR and MR) belong to the nuclear receptor superfamily. 2R resulted in the emergence of GR and MR, present in all extant vertebrates. In teleosts, 3R gave rise to duplicated gr and mr (Bury, 2017). Zebrafish is the only known teleost to have conserved only one of the two gr paralogs (Schaaf et al., 2008). The two mr paralogs are present in a basal teleost, the European eel Anguilla anguilla (Lafont et al., 2014), while only one mr paralog has been conserved in the other extant teleosts studied so far (Baker and Katsu, 2019).

Metamorphoses and Other Developmental Transitions in Vertebrates and Their Control by Thyroid Hormones and Corticosteroids

Larval Metamorphosis in Anuran Amphibians

Involvement of Thyroid Hormones

After hatching and a period of growth, the tadpole undergoes a rapid and irreversible physiological, anatomical and environmental transition marking the transition from the larval state to the adult state, the metamorphosis. Gudernatch observed that the administration of extracts of the thyroid gland (and only this organ) via the water induced tadpole premature metamorphosis (Gudernatch, 1912). Following TH measurements (Leloup and Buscaglia, 1977), the elucidation of the roles and mechanisms of action of TH in vertebrates has thus benefited enormously from amphibian model (Grimaldi et al., 2013; Buchholz, 2017; Sachs and Buchholz, 2017). The activity of TH is regulated locally by deiodinases (DIO) and cytosolic proteins (Shi et al., 1994). In particular, the expression of DIO2 (enzyme activating TH) is high in tissues undergoing metamorphosis, while the expression of inactivating deiodinase (DIO3) is high in tissues before and after metamorphosis (Leloup et al., 1981; Galton, 1989).

Another level of TH signaling control is linked to the expression profiles of thyroid hormone receptors (TR) (Yaoita and Brown, 1990). A dual role of thyroid signaling was proposed (Sachs et al., 2000; Grimaldi et al., 2013; Buchholz and Shi, 2018). Thus, before metamorphosis, the relative absence of TH and the expression of TRα contribute to repressing target genes allowing tadpole growth. During the climax of metamorphosis, the high concentration of TH concomitant with the expression of TRα and TRβ contributes to the activation of the transcriptional program leading to tadpole transformation. The two TR isoforms have also different roles during metamorphosis. TRα was shown to be more involved in cell proliferation while TRβ in cell differentiation and apoptosis (Furlow and Neff, 2006; Denver et al., 2009). TRα is required for TH-dependent neurogenesis (Wen et al., 2019). The autoinduction of TRβ is one of the earliest responses to the thyroid signal (Yaoita and Brown, 1990) because trβ is a direct TH-target gene (Ranjan et al., 1994; Bilesimo et al., 2011).

Transgenic studies in Xenopus laevis revealed that TR are necessary and sufficient for mediating the effects of T₃ during metamorphosis (Buchholz et al., 2003, 2004). However, recent gene knockout studies in Xenopus tropicalis showed that TR are not required for most metamorphic transformations, although tadpoles lacking TR die in the middle of metamorphosis (Shi, 2021). Removal of TR enables premature metamorphosis of several adult tissues (Buchholz and Shi, 2018), likely due to the absence of T₃-inducible gene repression. This result supports the role of unliganded TR to avoid precocious metamorphosis for proper tadpole growth. Finally, removal of TR prevents the disappearance of tadpole-specific tissues (Shibata et al., 2020, 2021).

Involvement of Corticosteroids

Glucocorticoids (GC) are also essential during anuran metamorphosis. In Xenopus laevis tadpoles, corticosterone concentration is high during pre-metamorphosis, decreases during pro-metamorphosis and increases again during metamorphic climax (Jaudet and Hatey, 1984; Jolivet-Jaudet and Leloup-Hâtey, 1986; Kloas et al., 1997; Glennemeier and Denver, 2002). However, the actions of GC on anuran development are difficult to dissect because of their involvement in many biological processes. Thus, GC inhibit growth, both in pre- and pro-metamorphic tadpoles and the administration of exogenous GC to pre-metamorphic tadpoles inhibits the emergence of lower limbs (Kobayashi, 1958). However, the use of drugs which antagonize the molecular action of GC or prevent the production of GC by the adrenals, inhibits metamorphosis (Kikuyama et al., 1982).

During metamorphosis, GC act through glucocorticoid receptors (GR) that have dynamic and tissue-specific expression profiles (Krain and Denver, 2004). In the tail, GR expression follows the concentration profile of GC, but in the gut and brain the number of transcripts were constant during pro-metamorphosis, and slightly decreased or increased, respectively, during climax. GR knockout in Xenopus leads to complete abrogation of the corticosterone-responsive gene induction by exogenous hormone (Sterner et al., 2020). In addition, tadpoles lacking GR developed faster than wild-type sibling until forelimb emergence. Then, they developed more slowly and died at the climax of metamorphosis, indicating that GR is required for metamorphosis and control the developmental rate. The essential requirement of the HPA axis was confirmed with the gene-editing disruption of the pomc gene (Sterner et al., 2020). Mutant tadpoles had a reduced level of plasma corticosterone at metamorphosis, as well as lower expression of the corticosterone-responsive genes. Last but not least, these tadpoles had reduced rates of growth and development that finally led to death, late during metamorphosis at the time of tail resorption.

Interactions Between Thyroid Hormones and Corticosteroids

Although TH are the trigger for metamorphosis and are required throughout this process (Sachs and Buchholz, 2017), their actions strongly intersect with those of CS (Sachs and Buchholz, 2019). Stressors such as predation or pond desiccation can be experienced by tadpoles and cause activation of the HPI axis (Glennemeier and Denver, 2002). In the tadpole, the synthesis and release of TSH by the anterior pituitary is under the control of CRH (Denver, 1993, 2021), as in other non-mammalian vertebrates (De Groef et al., 2006). When injected to prometamorphic Bufo arenarum larvae, CRH is able to accelerate metamorphosis, likely by direct action on both TSH and ACTH pituitary cells (Miranda et al., 2000). This dual role of CRH allows the tadpole to modulate the rate of metamorphosis in response to environmental stimuli (Denver, 1997). CS are closely linked to metamorphosis by delaying or accelerating its rate of progression. Elevation in circulating CS during the pre-metamorphic stage slows tadpole growth (Denver, 2017). However, during pro-metamorphosis, tadpoles increase the production of TH and CS in response to environmental stress, and are therefore able to accelerate metamorphosis, which can allow the animal to escape a deteriorating larval habitat by transitioning to the next life history stage (Denver, 1997, 2009; Denver et al., 2009; Kulkarni and Buchholz, 2014). Remarkably, CS are capable of triggering metamorphosis in Buffo boreas (Hayes et al., 1993). This action is probably due to the endogenous levels of TH with which GC are able to act synergistically, but insufficient, on their own, to induce the metamorphosis.

How does the crosstalk between TH and CS occur? CS are known to promote the expression of activating deiodinases and repress the expression of inactivating deiodinases, thus contributing to the accumulation of active T₃ in target tissues. This model has long been the basis for explaining the potentiating effect of GC on metamorphosis (Galton, 1990). Furthermore, GC can also act in synergy with TH via cross-regulation at the level of their respective nuclear receptors. GC are able to increase the binding capacity of T₃ in cell nucleus (Suzuki and Kikuyama, 1983) and the amount of trβ transcripts in the tail, brain and intestine (Bonett et al., 2010). Conversely, the expression of GR seems to be partly controlled by TH depending on the tissues observed: while in the brain and intestine, treatment with T₃ induces a decrease in the expression of GR, the opposite occurs in the tail (Krain and Denver, 2004). These results suggest that CS are able to increase the sensitivity to TH in some tissues, thus accelerating metamorphosis. These actions are synergistic with low concentrations of TH (Bonett et al., 2010). Brown et al. (2014) reported similar hormonal synergy during larval development in fish.

Other genes expressed during metamorphosis are synergistically regulated by TH and CS (Kulkarni and Buchholz, 2012; Bagamasbad et al., 2015), some through direct transcriptional regulation by liganded TR and GR. One of the best studied examples of this type of regulation is the transcription factor krüppel-like factor 9 (Klf9), which is directly and synergistically regulated by TH and CS via an ultra-conserved super enhancer located upstream of the transcription start site (Bonett et al., 2009; Bagamasbad et al., 2015). Klf9 strongly enhances TRβ autoinduction in tadpole tissues, among other roles modulating gene transcription and hormone action during metamorphosis (Hu et al., 2016). Other genes show synergistic regulation by TH and CS in tadpole tissues, but whether their protein products function to modulate the rate of metamorphosis requires further study (Kulkarni and Buchholz, 2012, 2014).

Finally, the recent results with tadpoles lacking pomc reinforce the inseparable link between TH and GC at metamorphosis (Sterner et al., 2020). Tadpoles lacking pomc had reduced expression levels of TH-responsive genes such as klf9 and trβ. Even more significant, mutant death at metamorphosis is rescued by exogenous TH, suggesting a strong entanglement of the signaling by both hormones.

First/Primary and Secondary Metamorphoses in Teleost Fishes

In fishes, two types of metamorphoses can be observed. Both types involve various morphological, physiological and behavioral modifications that preadapt the animal to life in a new environmental niche/habitat, but occur at different life-stages. First/primary metamorphosis typically occurs in elopomorphs and pleuronectiforms, during larval stage and is so-called larval metamorphosis. Secondary metamorphosis occurs in juveniles of some diadromic migratory teleosts and involves less drastic morphological changes. This is the case of smoltification in anadromous salmonids, which allows the transition from a juvenile ecophase in freshwater to the next ecophase in the ocean.

Larval Metamorphosis in Teleosts: The Example of Flatfish

Beside the striking larval metamorphosis in eels and flatfishes, studies also report developmental changes controlled by TH during larval to juvenile transition in various teleosts such as grouper Epinephelus coioides (de Jesus et al., 1998), seabream (Campinho et al., 2010), gobiid Sicyopterus lagocephalus (Taillebois et al., 2011), or clownfish Amphiprion percula (Salis et al., 2021). Our review will focus on the well-known pleuronectiform/flatfish metamorphosis. Larval metamorphosis with the migration of one eye to the opposite side of the head is unparalleled in vertebrate development (Inui and Miwa, 2012). Spectacular morphological changes are accompanied by behavioral (pelagic to benthic life and locomotion) and physiological (such as development of gastrointestinal tract to adapt to the novel food resources in a new habitat) changes.

Involvement of Thyroid Hormones

In the Japanese flounder Paralichthys olivaceus, larval tissue T₄ and T₃ concentration increases gradually during pro-metamorphosis, and rises sharply at the beginning of climax, reaching highest level at climax (Miwa et al., 1988; Tanangonan et al., 1989; Tagawa et al., 1990; de Jesus et al., 1991). A similar surge of tissue TH concentration at metamorphic climax is reported in spotted halibut, Verasper variegatus (Hotta et al., 2001a,b), Atlantic halibut Hippoglossus hippoglossus (Einarsdóttir et al., 2006), and summer flounder, Paralichthys dentatus (Schreiber and Specker, 1998).

Treatments of flatfish by TH or anti-thyroid drug have demonstrated the involvement of TH in many metamorphic changes (Inui and Miwa, 2012). One of the most striking examples concerns skeleton development (shortening of fin rays, eye migration and asymmetry). The elongated fin rays at the anterior end of the dorsal fin shorten to reach similar length to other fin rays. Manipulation of T₄ availability disrupts pre-metamorphic Japanese flounder larvae shortening of elongated fin rays (Inui and Miwa, 1985; Miwa and Inui, 1987; de Jesus et al., 1990). Administration of T₄ to pre-metamorphic larvae accelerates eye migration (Inui and Miwa, 1985; Miwa and Inui, 1987; Solbakken et al., 1999). In addition, Schreiber and Specker showed a stage-specific developmental response to TH, with a more pronounced effect in the induction of eye migration at earlier stages (Schreiber and Specker, 1998). Campinho et al. (2018) gave the first evidence of a TH-responsive asymmetric center located in the anterior head region that is correlated with asymmetric development during metamorphosis of flatfish.

In Japanese flounder, expression of trαA and trβs (trβ1 and trβ2) genes increase rapidly at metamorphic climax; while expression of trαA peaks at climax and decreases thereafter (like T₄ content), expression of trβs peak at post-climax and remains high in metamorphosed juveniles; in contrast, expression of trαB remains low throughout larval development (Yamano and Miwa, 1998). In the turbot, Scophthalmus maximus, trα, but not trβ, expression is up-regulated at metamorphic climax (Marchand et al., 2004). In contrast, studies in two other flatfishes, the halibut (Galay-Burgos et al., 2008) and the Senegalese sole Solea senegalensis (Isorna et al., 2009; Manchado et al., 2009), describe a situation similar to that in amphibian with only trβ expression showing a peak during metamorphosis.

DIO2 activity and dio2 expression increase during sole metamorphosis, while DIO3 activity and dio3 expression decline at mid-late metamorphic period (Isorna et al., 2009). These developmental profiles of deiodinases coincide with the rise of TH levels observed. In this species, there is an asymmetric expression of dio2 and TRβ in the head, which coincides with the head region where asymmetric development of bone and brain occurs (Campinho et al., 2018). In the Japanese flounder, dio1 is expressed in liver from pro-metamorphosis to early climax, while dio2 is expressed in limited regions of the eyes, tectum and skeletal muscle from pro-metamorphosis to post-climax, and dio3 in skeletal muscle and gastric gland blastemas at metamorphic climax (Itoh et al., 2010).

Involvement of Corticosteroids

Data support a role of CS in larval flatfish metamorphosis. Whole body cortisol concentration in Japanese flounder increases during pro-metamorphic stage, reaching a peak level at climax, and decreases thereafter to about half of the maximal level (de Jesus et al., 1991). In vitro cortisol treatment of cultured dorsal ray fins from Japanese flounder is not effective alone on inducing metamorphic-like changes such as resorption of the fin rays (de Jesus et al., 1990). In contrast, in vivo cortisol treatment via water of pro-metamorphic flounder larvae for 15 days is not able to trigger some of the changes observed during metamorphosis, like settling (benthic) behavior and eye migration, but does induce shortening of second fin ray (de Jesus et al., 1990). Administration of cortisol via water to spotted halibut increases the occurrence of ambicolored juveniles by inducing the development of adult type pigment cells on the blind side of fishes (Yamada et al., 2011). In cortisol-implanted juvenile Senegalese sole, hepatic and renal DIO2 activities are enhanced, suggesting that CS can be key regulator of extrathyroidal T₃ production in this species (Arjona et al., 2011). This regulation is likely to occur also during sole larval metamorphosis.

Interactions Between Thyroid Hormones and Corticosteroids

Few data are available concerning the interactions between TH and GC in the control of teleost larval metamorphosis. In the Japanese flounder, a permissive effect of cortisol on thyroid hormone action is observed during metamorphosis (de Jesus et al., 1990). Indeed, cortisol alone does not affect the shortening of fin rays in vitro, whereas when added together with T₄ or T₃, it enhances its rate compared to T₄ or T₃ alone. This permissive effect of cortisol on TH action was not reported in vivo (de Jesus et al., 1990). Combined T₄ and cortisol treatment does not induce either synergistic effects on settling behavior and eye migration, compared to T₄ treatment alone (de Jesus et al., 1990). The authors concluded that it may be due to sufficient production of endogenous cortisol by larval interrenal. Future studies should aim at investigating the mechanisms of CS/TH interactions in teleost metamorphoses as deciphered in amphibians.

Secondary Metamorphosis in Teleosts: Example of Smoltification in Salmonids

Smoltification is the transition of sedentary juvenile parr into downstream migratory smolt, which will pursue its growth phase in the ocean. Smoltification gathers many changes, morphological ones, such as body silvering and fin darkening, behavioral ones, with swimming activity in open space, formation of schools and downstream migration, and physiological ones related to adaptation to seawater and imprinting (Hoar, 1976, 1988; Boeuf, 1993; McCormick, 2012; Rousseau et al., 2012).

Involvement of Thyroid Hormones

Even if some authors do not consider salmonid smoltification as a metamorphosis (Bishop et al., 2006), this transformation from parr to smolt involves major changes and is necessary for the fish to reach its next habitat and survive in a new environment. Moreover, many parallel features exist between flatfish metamorphosis and salmonid smoltification, as reviewed by Björnsson et al. (2012). Lastly, control by TH is crucial in smoltification.

In salmonids, a rise of plasma T₄ and/or T₃ levels is observed at the time of smoltification (McCormick et al., 2009; Björnsson et al., 2012). Manipulation of TH levels by administration of T₄, T₃ or anti-thyroid drugs supports a major role of TH in many smoltification-related morphological, behavioral and physiological changes, such as metabolism, olfaction, change in visual pigments, swimming behavior and downstream migration (McBride et al., 1982; Rousseau et al., 2012). The examples of TH-induced changes, given here, are necessary for avoiding predation and for adaptation to a new environment, seawater (SW). A pioneer study showed that intramuscular injection of mammalian thyroid extract or TSH induces silvery smolt stage in rainbow trout (Robertson, 1949). Following studies confirmed that exogenous TH (Miwa and Inui, 1983, 1985; Ikuta et al., 1985; Coughlin et al., 2001) and TSH (rainbow trout: Premdas and Eales, 1976) induce body silvering. The silvering of the body is due to the deposition in the skin of purines, hypoxanthine and guanine, the level of which is increased by T₄ treatment in masu salmon O. masou (Ura et al., 1994). Early evidence reported the involvement of TH in salinity preference: TSH-treated coho salmon O. kisutch shows a change from freshwater (FW) to SW-preference, while the contrary is observed in pink salmon O. gorbuscha treated by an anti-thyroid drug (Baggerman, 1963). Similarly, T₄ treatment increases the salinity preference in coho salmon (Iwata et al., 1990). In Atlantic salmon, T₃ increases SW survival (Saunders et al., 1985).

Interestingly, a large peak of expression of tshβ1b during Atlantic salmon smoltification, at the time of the initiation of the downstream migration, has recently been demonstrated, with no change in the expression of the paralog tshβ1a, suggesting the involvement of tshβ1b at smoltification, possibly in the initiation of migration (Fleming et al., 2019). In addition, the expression of pituitary tshβ1b, and not tshβ1a, is induced by long day-photoperiod (16h of light and 8h of dark) in Atlantic salmon (Irachi et al., 2021).

Expression of TR has been detected in all the tissues involved in smoltification-related changes (Marchand et al., 2001; Jones et al., 2002; Raine et al., 2005; Harada et al., 2008). Expressions of trα and trβ show no drastic change between the different stages of smoltification in brain, liver, eyeball, and skin in coho salmon (Harada et al., 2008). In contrast, the olfactory epithelium of masu salmon presents more T3 binding sites at smolt than at parr and pre-smolt stages, suggesting that olfactory tissues may be particularly sensitive to TH, related to a possible role in imprinting of natal stream odors in order to migrate back there to reproduce (Kudo et al., 1994). DIO3 activities are enhanced at smoltification in liver (Eales et al., 1993; Sweeting et al., 1994; Specker et al., 2000) and gill (Sweeting et al., 1994). The expression of one of the 4R-paralog, dio2b, increases in the brain in zones of cell proliferation during smoltification in response to photoperiod (Lorgen et al., 2015; Irachi et al., 2021).

Involvement of Corticosteroids

The cells of interrenal tissue undergo hypertrophy during smoltification (for review: (Specker, 1982). Pituitary corticotropic cells are also activated during smoltification in Atlantic salmon (Olivereau, 1975). Plasma cortisol levels are low in winter, increase during spring at the time of smoltification and decline from July to September (Langhorne and Simpson, 1981, 1986; Specker and Schreck, 1982; Barton et al., 1985; Virtanen and Soivio, 1985; Young et al., 1989; Nagae et al., 1994; Sundell et al., 2003). Maximal in vitro responsiveness of interrenal tissue to ACTH is observed in April in coho salmon (Young, 1986).

As for TH, we will concentrate on the effects of HPI manipulation on pigmentation and osmoregulation. Injection of ACTH in Atlantic salmon can induce darkening of dorsal, pectoral and caudal fins, but neither ACTH nor cortisol have an effect on body silvering (Langdon et al., 1984). Prolonged cortisol treatment in pre-smolt salmons increase Na⁺/K⁺-ATPase activity in the gill (Richman et al., 1987; Madsen, 1990) and in gut (Madsen, 1990; Veillette and Young, 2005). In vitro, cortisol treatment maintains Na⁺/K⁺-ATPase activity, which declines in controls, in tissue culture of FW-adapted sockeye salmon intestine (Veillette and Young, 2005). Injections of FW-Atlantic salmon with cortisol increase the expression of claudins (tight-junction proteins) involved in the remodeling of the gill in response to salinity changes (Tipsmark et al., 2009). Using primary cultures of Atlantic salmon gill tissue, a stimulatory effect of cortisol is observed on the expression of claudins; an effect blocked by GR antagonist, mifepristone (or RU486), suggesting the involvement of a glucocorticoid type receptor (GR) (Tipsmark et al., 2009).

An increase in gill GR concentration and gr expression is reported during smoltification in all studied salmonid species (McLeese et al., 1994; Shrimpton and Randall, 1994; Shrimpton, 1996; Mazurais et al., 1998; Shrimpton and McCormick, 1998, 2003; Mizuno et al., 2001; Kiilerich et al., 2007). This increase occurs before the increase in plasma cortisol, which could explain the increased responsiveness of gill tissue to cortisol observed in early spring in coho and Atlantic salmon (McCormick et al., 1991) and also demonstrated in vitro in rainbow trout (Shrimpton and McCormick, 1999).

Interactions of Thyroid Hormones and Corticosteroids

Studies report interactions between HPT and HPI during smoltification. For example, TH can increase CRH neurogenesis during smoltification in Atlantic salmon (Ebbesson et al., 2011), suggesting a positive effect of TH on HPI. Cortisol treatment can lower plasma T₃ (but not plasma T₄) in coho salmon (Vijayan and Leatherland, 1989), during smoltification (Redding et al., 1991). The increases of tr mRNA and TR protein expressions and of plasma TH levels, observed during transfer from FW to SW, are lower in cortisol-injected smolt sockeye salmon compared to controls (Shin et al., 2014), suggesting some antagonistic/negative effects of cortisol on TH action.

Egg Hatching in Sauropsids

Thyroid hormones have an important role in fish egg hatching (tilapia: Reddy and Lam, 1991; Walpita et al., 2007; zebrafish: Heijlen et al., 2014; for review: Brown et al., 2014), but it will not be considered in this review, as egg hatching in fish implies less drastic changes of environmental conditions, as compared to sauropsids. In contrast, hatching in oviparous sauropsids, such as birds and reptiles, is characterized by a transition from a “protected” aqueous environment to a terrestrial environment exposed to desiccation and predation.

Egg Hatching in Birds

Involvement of Thyroid Hormones

Considering the implication of TH in egg hatching, one must differentiate precocial from altricial birds (McNabb, 2006; De Groef et al., 2013). Precocial species (e.g., chicken Gallus domesticus, Japanese quail Coturnix japonica, bobwhite quail Colinus virginianus, turkey Melleagris gallopavo, mallard Pekin duck Anas platyrhynchos, goose Anser anser) have youngs that are immediately mobile and independent after hatching. In contrast, youngs of altricial birds (e.g., European starling Sturnus vulgaris, Ring dove Streptopelia risorii, red-winged blackbird Agelaius phoeniceus, great tit Parus major) need to be fed and thermoregulated by their parents in the nest (Starck and Ricklefs, 1998).

A gradual increase in plasma TH concentrations of the embryos to a peak is observed in precocial birds during the peri-hatch period (for review McNabb, 2006). In contrast, in altricial birds, circulating concentrations of TH are low during embryonic life and at hatching, and only increase after hatching (McNabb et al., 1984; Silverin and Rudas, 1996; Výboh et al., 1996; Olson et al., 1999).

Manipulation of egg TH levels influences avian hatching time. Injection of antithyroid drugs in the yolk sac of chick embryos retards hatching, and T₄ fully neutralizes these effects (Grossowicz, 1946; Adams and Bull, 1949; Romanoff and Laufer, 1956; Sinha et al., 1959; Balaban and Hill, 1971; Haba et al., 2011). In turkey, T₄ or T₃ injected to fertile eggs at Day 0 of incubation depresses hatchability, while improving it when administered at Day 25 of incubation out of a 28-day incubation period (Christensen, 1985). In Pekin duck, injection of T₃ results in earlier hatching, while injection of antithyroid drug delays hatching (Sirsat and Dzialowski, 2020). In Japanese quail, injection of T₄ alone or with T₃ doubles hatching success (Sarraude et al., 2020). Similarly, in a type 2 semi-altricial development model, the rock pigeon Columba livia, injection of a mixture of both T₃ and T₄ early results in higher hatching success but unchanged hatching time (Hsu et al., 2017).

In chicken, a differential temporal expression pattern of the three TR is observed. TRα mRNAs are detected as early as gastrula stage and throughout development in many embryonic tissues (Forrest et al., 1990). TRβ0 mRNAs appear later in embryonic life and are restricted to brain, eye, lung, and yolk sac (Forrest et al., 1990). TRβ2, a N-terminal variant of TRβ0, is predominantly expressed in retina (Sjöberg et al., 1992). The minimal generation of T3 until just before hatching is primarily due to the presence of DIO3 in chicken embryo liver (Galton and Hiebert, 1987). Hepatic DIO1 activity increases up to hatching and decreases thereafter, while hepatic DIO3 activity increases during embryogenesis, then decreases before hatching to remain low at post-hatching (Darras et al., 1992; Reyns et al., 2003). Dynamics of expression in deiodinases in the choroid plexus of the developing chicken brain have been reported: dio1 and dio2 mRNA levels increase over time to reach a peak around hatching, while dio3 expression is high before hatching and decreases at hatching to re-increase up to 1 day post-hatching (Van Herck et al., 2015).

Involvement of Corticosteroids

An increase of avian embryonic GC is observed around the time of hatching in plasma (Wise and Frye, 1973; Kalliecharan and Hall, 1974; Siegel and Gould, 1976; Marie, 1981; Scott et al., 1981; Tanabe, 1982; Tanabe et al., 1983, 1986; Wentworth and Hussein, 1985; Porter et al., 2007), in adrenal glands (Tanabe et al., 1983, 1986), and in feces (Frigerio et al., 2001), and in adrenocortical cells in culture (Carsia et al., 1987).

Most studies investigating the effects of exogenous treatment of embryos with corticosterone in birds look at the postnatal growth and behavior linked to stress response (Rubolini et al., 2005; Saino et al., 2005; Freire et al., 2006; Hayward et al., 2006; Janczak et al., 2006; Henriksen et al., 2013; Zimmer et al., 2013; Weber et al., 2018). However, a few looked at the effects of GC treatment on hatching. Injection of corticosterone in the yolk sac 2 days prior to hatching shortens incubation time and increases hatchability in turkey (Wentworth and Hussein, 1985). In contrast, dipping fertile eggs in corticosterone prevents hatching in chicken (Mashaly, 1991). Elevation of plasma corticosterone levels by mean of synthetic GC (dexamethasone) injection during the final stages of incubation in chicken embryos increases or shortens incubation period when administered, on Day 16 and Day 18, respectively (Tona et al., 2007). In Japanese quail, incubation period is shortened in eggs laid by corticosterone-implanted hens (Schmidt et al., 2009). Chicken lung becomes sensitive to corticosterone prior hatching (Hylka and Doneen, 1983). Corticosterone treatment triggers prehatching stimulation of surfactant phospholipid synthesis (Hylka and Doneen, 1983). The first two studies reporting the cloning and developmental expression of pituitary GR in bird (chicken) gave different results: While Kwok et al. (2007) demonstrate constant expression of GR during embryonic period, other authors show an increase of GR mRNA levels (Porter et al., 2007).

Interactions Between Thyroid Hormones and Corticosteroids

Creating hypothyroidism in chick embryos induces a cortical atrophy and medulla hypertrophy in adrenal gland (Kingsbury et al., 1955). Injection of cortisol onto the allantoic membrane of 17 or 16-days old chicken embryos induces the same premature maturational changes in T₃ and T₄ metabolism observed naturally on 19–20-days old embryos, meaning a decrease of DIO3 preserving the T₃ formed, and an increase of DIO2 sparing T₄ (Borges et al., 1980). The administration of either dexamethasone or corticosterone, or ACTH to chicken embryos increase plasma T₃ concentrations and hepatic DIO2 activity (Decuypere et al., 1983) and increase plasma T₃ levels, decreased plasma T₄, decreased hepatic DIO3 activity and increased hepatic DIO1 activity (Darras et al., 1996).

Egg Hatching in Reptiles

Involvement of Thyroid Hormones

An increase in TH correlates with hatching in saltwater crocodile Crocodylus porosus (Shepherdley et al., 2002). In the grass snake Natrix natrix, the activity of the embryonic thyroid exhibits the features of a fully active gland at the time of hatching (Rupik, 2011). Injection of antithyroid drug into embryos of the snapping turtle Chelydra serpentina gives enlarged thyroid gland and delays hatching time (Dimond, 1954). Eggs of red-eared turtle, Trachemys scripta, treated with T₃, have shortened incubation duration (Sun et al., 2016). Embryos from Murray River short-necked turtle, Emydura macquarii, exposed to T₃, hatch earlier than untreated ones (McGlashan et al., 2017). Treatment of saltwater crocodile embryos with T₃ increases DIO1 activity in liver and DIO2 in kidney (Shepherdley et al., 2002). Treatment with T₃ stimulates the secretion of phosphatidylcholine (PC, the major component of pulmonary surfactant) in sea turtle, Chelonia mydas (Sullivan et al., 2001). In saltwater crocodile, pre-treatment with T₃ increases surfactant phospholipids in lung (Sullivan et al., 2002a).

Involvement of Corticosteroids

An increase of corticosterone is observed from the last third of incubation to hatching in American alligator Alligator mississippiensis (Medler and Lance, 1998; Jennings et al., 2000). In contrast, a decrease in corticosterone is observed at hatching in saltwater crocodile (Shepherdley et al., 2002). Yolk corticosterone concentrations peak near the time of hatching in the tree lizard, Urosaurus ornatus (Jennings et al., 2000) and in sea turtles (Owens and Morris, 1985). In the tree lizard, treatment with corticosterone accelerates egg hatching (Weiss et al., 2007). Treatment with dexamethasone of saltwater crocodile embryos decreases DIO1 activity in kidney, DIO2 activity in liver and in kidney and DIO3 activity in liver (Shepherdley et al., 2002). Dexamethasone alone increases phospholipids from pulmonary surfactant in sea turtle when administered in ovo during late incubation (Sullivan et al., 2001). It also stimulates the secretion of phosphatidylcholine in vitro in saltwater crocodile (Sullivan et al., 2002a) and in lizard bearded dragon Pogona vitticeps (Sullivan et al., 2002b). In Chinese alligator Alligator sinensis, variations of the mRNA levels for gr in kidney, liver, and heart during embryonic development suggest a potential role for GC in tissue maturation before hatching (Izaz et al., 2021).

Interactions Between Thyroid Hormones and Corticosteroids

Treatment with dexamethasone and T₃ of saltwater crocodile embryos has effects on deiodinase activities: decrease of DIO1 activity in kidney, decrease of DIO2, and DIO3 activities in liver (Shepherdley et al., 2002). In the sea turtle Chelonia mydas, the secretion of phosphatidylcholine is stimulated by a combination of T₃ and dexamethasone before hatching (Sullivan et al., 2001). Similar results were obtained in the saltwater crocodile (Sullivan et al., 2002a) and in the lizard Pogona vitticeps (Sullivan et al., 2002b). All these data demonstrate the involvement of both TH and GC in the regulation of surfactant maturation in reptiles (Sullivan et al., 2003). Sullivan et al. (2003) reviewed the control of pulmonary surfactant and stated that dexamethasone and T₃ are crucial stimulators of surfactant production during embryonic development throughout evolution.

Birth in Mammals

Involvement of Thyroid Hormones

During most of the gestation in human, T₄ is converted in rT₃, while toward term, developmental changes in tissue deiodinase activity occur, leading to preferential deiodination of T4 to T3 (instead of rT₃) and rise in plasma T₃ concentration near term (Forhead and Fowden, 2014). In contrast, in the rat, circulating T₃ concentrations do not increase before birth (Dubois and Dussault, 1977; Harris et al., 1978; Lamers et al., 1986). Comparison of hormonal profiles during the perinatal period in two closely related murine species with distinct modes of development (altricial vs. precocial), the rat (altricial), and the spiny mouse Acomys cahirinus (precocial) allowed to show a correlation between perinatal increase in T₃ levels and precocial timing of birth (Lamers et al., 1986).

TH have a major regulatory role on fetal growth (Forhead and Fowden, 2014), and maturation of the central nervous system (Patel et al., 2011; Stenzel and Huttner, 2013). Furthermore, maternal hypothyroidism is associated with increased rates of respiratory distress syndrome in new-born (Casey et al., 2005; Männistö et al., 2013) and cardiorespiratory disorder (Rousseau et al., 2019). In various mammalian species, TH change the synthesis of the components of surfactant (Ballard et al., 1984; Das et al., 1984; Warburton et al., 1988; Gilbert et al., 2001; Van Tuyl et al., 2004). TH are also involved in the intestinal structural development (Trahair and Sangild, 1997; Sirakov and Plateroti, 2011; Sirakov et al., 2014). Specific TRα1 loss-of-function leads to low development and impaired activity of murine intestinal stem cells in culture (Godart et al., 2021). In addition, in vivo treatment confirms the positive action of T₃ on intestinal crypt cell proliferation and demonstrates its key action in modulating the number of stem cells, the expression of their specific markers and the commitment of progenitors into lineage-specific differentiation (Godart et al., 2021).

Involvement of Corticosteroids

An increase of plasma fetal GC is detected near parturition in many mammals (Alexander et al., 1968; Mulay et al., 1973; Lamers et al., 1986; Silver and Fowden, 1989; Yoon et al., 1998). The involvement of HPA axis in the timing of birth is first evidenced in ovines (Van Rensburg, 1967; Barnes et al., 1977). Furthermore, premature delivery is induced by injection of ACTH or corticosteroids into the ovine fetus (Van Rensburg, 1967; Halliday and Buttle, 1968; Liggins, 1968, 1969) as well as in fetal piglet (Bosc, 1973). More recently, the use of antalarmin, a CRH-R type I antagonist, can delay the onset of parturition in sheep, which suggests that CRH is involved in the induction of parturition in this species (Chan et al., 1998).

The many roles of GC on organ maturation have been the subjects of recent reviews (Fowden and Forhead, 2015; Fowden et al., 2016; Jellyman et al., 2020). As for TH, we will concentrate on GC involvement in lung and gastro-intestinal tract (GIT) maturations, which are crucial to cope with the change of environment (from aquatic to terrestrial) and of nutrition (from parenteral to enteral), respectively. In lambs born prematurely by infusion of dexamethasone, partial aeration of the lungs is noted, suggesting an accelerated appearance of surfactant activity (Liggins, 1969). Infusion of ACTH into one of twin pairs of lamb fetuses accelerates the morphological changes, that would normally occur in the lung, before birth (Sundell et al., 1979). GC treatment changes the synthesis of the phospholipid and protein components of surfactant (Warburton et al., 1988; Gilbert et al., 2001). At birth, there is a shift from mainly parenteral nutrition in the fetus (via the placenta) to enteral nutrition in the neonate, and the GIT has to prepare during gestation for coping with this change. This prenatal development of GIT is regulated by GC (Trahair and Sangild, 1997; Sangild et al., 2000). After bilateral adrenalectomy of fetal sheep, growth of mucosal structures and villus height are reduced in the small intestine (Trahair et al., 1987a). After infusion of cortisol, no change in enterocyte morphology is detected, but the proportion of crypt cells and the migration of enterocytes are increased (Trahair et al., 1987b). In addition, cortisol influences the prenatal development of gastric acid and gastrin secretion, and of GIT hydrolase activities in both the fetal pig and sheep (Trahair and Sangild, 1997; Sangild et al., 2000).

Interactions Between Thyroid Hormones and Corticosteroids

Before birth, TH and GC synergize for the maturation of various organs, especially the lung, the liver and the brain. This synergism is partly linked to the fact that GC induce local deiodinase expression and activities resulting in the increase of circulating T₃ and thus T₃ bioavailability (Forhead et al., 2006; Fowden and Forhead, 2009). A synergism of TRH/T₃ and cortisol has been reported on lung maturation in fetal sheep, as infusion of cortisol and TRH (Liggins et al., 1988) or T₃ (Schellenberg et al., 1988; Warburton et al., 1988) increase the distensibility and the stability of the lung. In explant culture of human fetal lung, a supra-additive response in the synthesis of surfactant is observed in the presence of both dexamethasone and T₃ (Gonzalez et al., 1986).

T₄ injection to rats induces a precocious appearance of pepsinogen in the oxyntic gland mucosa and increases acid secretion, while in propylthiouracil-induced hypothyroid pups, pepsinogen content and basal acid secretion are low (Tseng and Johnson, 1986). However, T₄ has no such effects in adrenalectomized rats, while corticosterone is able to increase pepsinogen content and basal acid secretion in the absence of normal levels of TH (Tseng and Johnson, 1986).

Comparison of the Involvement and the Interdependence Between Thyroid and Corticosteroid Signaling in Vertebrate Developmental Transitions

In all the major developmental transitions described here, a common synergistic activation of thyrotropic and corticotropic axes is observed, leading to synchronized increase of TH and CS production and release (Figure 4). Besides this hormonal activation, increased expression of receptors allows tissues to become more responsive to TH and CS in time (Figure 4) to induce morphological, behavioral and physiological changes when needed, meaning just before the animal has to adapt to its new environment and its new way of life. As in all the mechanisms underlying major biological processes, they are conserved along evolution. Thus, the involvement of both TH and CS signaling is encountered in fish and amphibian metamorphic processes, as well as in egg hatching in sauropsids and birth in mammals (Table 1).

FIGURE 4

In non-mammalian vertebrates, the neurohormone, corticotropin-releasing hormone (CRH), appears to be potentially a coordinator of activation of both thyrotropic and corticotropic axes, as it is able to simulate thyrotropin production and release as much as corticotropin ones. CRH may thus be involved in the simultaneous activation of these neuroendocrine axes at the time of developmental transitions in non-mammalian vertebrates, such as fish and amphibian metamorphoses or sauropsid egg hatching (Table 1). It is not the case in mammals, in which the thyrotropic and corticotropic axes are controlled centrally by different hormones, respectively, TRH and CRH. Another difference among vertebrate developmental transitions described in this review may lay in the degree of involvement (triggering vs. permissive) of the two signaling systems and their interdependence. Except perhaps during birth for mammals, corticosteroid signaling seems to be more permissive than crucial, in the way it allows the thyroid signaling to be even more efficient, by elevating the activating deiodinase expression and activities, as well as the expression of TH receptors. Another difference may be likely due to neofunctionalization of gene paralogs observed after WGD. Duplication of some genes, notably in teleosts, may lead to redistribution of function. For example, the involvement of tshβ1b at smoltification in Atlantic salmon, instead of the classical tshβ in other vertebrate developmental transitions, or also the relative importance and differential role of the various thyroid hormone receptors between flatfish and amphibian larval metamorphoses.

Impact of Environmental Factors on Post-Embryonic Transitions

Climate Change

Water Warming for Population Strictly Dependent on an Aquatic Habitat

Teleost fish as ectothermic vertebrates show complex responses to temperature variation (Pinsky et al., 2019). Temperature has in teleost fishes a direct effect on oxygen delivery, cardiovascular function, muscle function, food conversion, mitochondria efficiency, and biochemical reaction rates (Little et al., 2020). Fish physiology is thus likely to be affected by increases in average temperature and temperature variability leading to energy metabolism changes with impact on growth and locomotion. All these physiological processes have been associated with thyroid function.

T₃ regulates thermal acclimation in zebrafish (Little et al., 2013) with the decrease of metabolism, skeletal muscle function and swimming performance in hypothyroid cold-acclimated (18°C) but not hypothyroid warm-acclimated (28°C) animals. The interactions between temperature levels, thyroid conditions and swimming performance are also linked to performance of the heart and oxygen transport (Little and Seebacher, 2014). In the context of global warming, the low sensitivity to TH at warm temperature is a concern because it may reduce the capacity of zebrafish to match this environmental change. Furthermore, in medaka, exposure until hatching to warm temperatures (32°C) increases the activation of TH biosynthesis, via TSH (Castañeda-Cortés et al., 2020), as well as the activation of the stress axis, via CRH (Castañeda-Cortés et al., 2019).

Rainbow trout is a typical cold-water fish species for which seasonally warmer water correlates with a decrease in fry survival and an increase of T₃ and T₄ concentrations (Giroux and Schlenk, 2021). Transcriptome analysis of liver tissues from adult rainbow trout under heat stress (24°C) and control conditions (18°C) identifies the differential expression of 428 long non coding RNA some of which can be involved in maintenance of homeostasis or adaptation to stress (Quan et al., 2020). In Atlantic salmon, elevated temperature increases T₄ nocturnal levels (Nisenbaum et al., 2020). Thus, future climate changes can induce lower salinity tolerance and accordingly result in poor survival in seawater after smoltification.

To show the wide diversity of the links between global warming and TH, we will give three more examples. First, in the mosquitofish Gambusia holbrooki the thermal acclimation is mediated by TH and leads to decreased mitochondrial efficiency, metabolic rates, and swimming performance (Le Roy and Seebacher, 2020). Second, in the desert fish Amargosa pupfish Cyprinodon nevadensis amargosae, temperature contributes to altered TH levels and morphological development (Lema et al., 2016). We can thus expect that many desert fishes will be vulnerable to rising temperatures because they occupy habitats with already high temperatures. Finally, increased temperature induces a decrease of TH levels in convict surgeonfish Acanthurus triostegus (Besson et al., 2020). The effect on TH levels correlates with affected sensory development leading to higher predation.

Chronic temperature increases (persisting for a long time) are also known to induce acute stress responses in fishes (Alfonso et al., 2020). Global warming can cause water freshening from increased freshwater inputs. In Antarctic spiny plunderfish Harpagifer antarcticus, salinities decrease leads to high plasma cortisol levels compare to normal salinity (Vargas-Chacoff et al., 2021). This has implications for fish species that have evolved in stable environmental conditions like in the Antarctic. In a totally different environment, climate-induced bleaching of coral reefs alters anemonefish hormonal stress, resulting in decreased reproductive hormones and severely impacted reproduction (Beldade et al., 2017). Finally, in juvenile brown trout, Salmo trutta, water temperature affects cortisol and GR mRNA levels (Filipsson et al., 2020).

Aquatic and Terrestrial Life Cycle: Warming Leads to Double Penalty

Amphibians are another ectodermic taxon with complex interactions between costs and benefits of life in the aquatic and terrestrial environments. They are undergoing a precipitous decline linked with environmental pressures including climate change. Many amphibian species exploit temporary or even ephemeral aquatic habitats for reproduction. Survival from desiccation of pond drying is reached by maximizing larval growth and acceleration of development, including precocious metamorphosis.

The western spadefoot toad tadpoles, Pelobates cultripes, usually have long larval period, but it can shorten it in response to pond drying (Gomez-Mestre et al., 2013). Developmental acceleration correlates with increased corticosterone and TH levels as well as increased TRβ levels to increase metamorphic process. Anuran tadpole shows thus phenotypic plasticity in age and size at metamorphosis as a response to temperature variation (Ruthsatz et al., 2020). In Arizona tiger salamander Ambystoma tigrinum, the small increase in temperature tends also to decrease the time to metamorphosis and results in a worse body condition (Park et al., 2016). Plasticity in rates of growth and development is beneficial to allow a more rapid transition into the juvenile stage where rates of mortality are lower. However, early metamorphosis leads to juveniles with smaller size correlated with low survival and locomotor performance (Székely et al., 2020). Pond drying may also lead to the loss of the capacity to respond to desiccation following decreased food availability (Enriquez-Urzelai et al., 2013), liver damage with upregulation of DIO2 and TRα transcript levels while there is a decrease of TRβ (Chen et al., 2021), or increased oxidative damage during metamorphosis (Petrović et al., 2021).

TH and GC level variations underlie differences in the timing of metamorphosis. In response to pond drying, western spadefoot toad and New Mexico spadefoot toad Spea multiplicata that have long larval periods and large size at metamorphosis, accelerate metamorphosis and elevate whole-body content of TH and corticosterone (Kulkarni et al., 2017). In contrast, in Couch’s spadefoot toad Scaphiopus couchii that has a short larval period, whole-body TH and corticosterone content are high during metamorphosis and weakly affected by pond drying. Thus, species exhibiting less plasticity will be more sensitive to environmental changes. The TH and CS level variations to accelerate metamorphosis during habitat desiccation may originate from elevated CRH (Denver, 1997). CRH can be a transducer of environmental stimuli to modulate the rate of metamorphosis via the endocrine response. Interestingly, CRH has also been shown to control the term of pregnancy in mammals. Maternal plasma CRH concentrations are elevated early in pregnancy in those patients destined to deliver preterm, and are lower in patients destined to deliver post-dates (Challis and Hooper, 1989; McLean et al., 1995).

Climate Changes and Terrestrial Biodiversity

Temperature increase alters avian phenotypes such as advanced reproduction, migration schedules and individual appearance. Bird ability to maintain a stable body temperature in a wide range of thermal environments is regulated via endocrine pathways including TH and with a lesser extent CS (Ruuskanen et al., 2021). The knowledge on endocrine regulation of thermogenesis concerns mainly poultry, but poorly describe for environmental temperature variation. Offspring development are dependent of females via hormones deposited in eggs. Ambient temperature changes affect the hormone levels in the yolk including TH and CS. More specifically, T₄ levels were negatively correlated with ambient temperature in great tits Parus major (Ruuskanen et al., 2016). However, in wild pied flycatchers Ficedula hypoleuca, there is no evidence for context-dependent effects of prenatal TH related to postnatal temperature on growth, survival, and plasma TH levels (Hsu et al., 2020), suggesting species differences or unknown confounding effects.

In reptiles and turtles, temperature effect on TH and GC plasma levels is controversial being either absent, positive or negative. Highlighting only a few examples, in the alligator lizards Elgaria coerulea and Elgaria multicarinata, corticosterone levels increase with temperature (Telemeco and Addis, 2014) and in the South-American tegu lizard Salvator merianae, T₃, T₄, and corticosterone levels show a positive relationship with body temperature (Zena et al., 2020). Similar correlation between body temperature and plasma corticosterone is observed in the eastern fence lizards Sceloporus undulatus, under laboratory conditions, but not in the field (Racic et al., 2020). In contrast, in the common lizard Zootoca vivipara, baseline corticosterone levels decrease with increasing thermal conditions (Dupoué et al., 2018).

In mammals, we will only highlight two of the numerous examples. First, the transition between late gestation and early lactation is a developmental window sensitive to warming. Dairy cows experience stress due to the high energy and nutrient requirements of the fetus and the mammary gland. In early lactation, the decline of TH levels is more pronounced in cow maintained at 28°C compared to the one maintained at 15°C (Weitzel et al., 2017). The second example is an Artic mammal, which has highly evolved to these extreme environments and its capacity to adapt to this change may be limited. The polar bear is emblematic to this environment. It was shown that CS binding capacity of plasma CS binding globulin increases in polar bears as a consequence of climate warming (Boonstra et al., 2020). Evidence is still lacking to have a complete view of the interactions between GC and TH in response to global warming.

Endocrine Disruptors

Thyroid Function Disruption

As previously mentioned, TH orchestrates metamorphosis, brain development, and metabolism representing a potential target for endocrine disruptor chemicals/compounds (EDC). Although the molecular mechanisms for TH disruption is still unknown for most of the EDC, several affect TH synthesis, transport or metabolism and downstream effects (Thambirajah et al., 2019). One of the main concerns is disruption during early neurogenesis, which may affect several TH actions such as proliferation, differentiation, migration, synaptogenesis and myelination in the developing nervous system (Préau et al., 2015).

Because anuran metamorphosis is strictly dependent on TH, amphibians represent sensitive models for the detection and mechanistic elucidation of TH disrupting activities (thyroid histology, metamorphosis progression). EDC impact wild anurans and contribute to population declines. Some pesticides and biocides may interfere with TH signaling during nervous system development (Leemans et al., 2019; Trudeau et al., 2020) or metamorphosis timing (Orton and Tyler, 2015). Last but not least, exposition of Xenopus tadpoles to the benzo[a]pyrene leads to delayed metamorphosis and sexual maturity with transgenerational disruption of metabolism and population decline (Usal et al., 2021).

In zebrafish, exposure during the 7 first days of development to 25 known TH disrupting compounds leads to morphological defects and variations of transcripts involved in the HPT axis (Spaan et al., 2019). In another teleost fish, the metamorphosing convict surgeonfish Acanthurus triostegus, high doses of the pesticide chlorpyrifos induce defects by decreasing TH levels impacting olfactory, visual and mechano-sensory structure development (Besson et al., 2020). Interestingly, similar phenotypes were observed following temperature increase, highlighting the profound threat anthropogenic stressors pose to fish communities. To highlight the EDC mode of action, liver transcriptomic responses in yellow perch Perca flavescens population show variation of genes transcripts related to reproduction, retinol, iron, TH, oxidative stress, lipid metabolism, and immune functions between strongly impacted population vs. less impacted groups (Defo et al., 2018).

In birds as in teleost fishes and amphibians, because GC regulate metabolism, ability to modulate corticosterone in response to stressor is essential to face a wide array of environmental challenges. EDC contamination was shown to impair this GC role. Methylmercury exposure reduces stress-induced GC response in zebra finches, Taeniogypia guttata (Moore et al., 2014). TH function is also EDC target. The rural nestling peregrine falcon Falco peregrinus has significantly lower circulating concentrations of TH compared to urban nestlings where flame retardants are environmental contaminants that accumulate in predatory birds (Fernie et al., 2017).

EDC also affect TH signaling in mammals. Considering the large amount of recent data available, only a few examples will be given here. In mice, exposure to the flame-retardant, tetrabromo bisphenol A, modulates hypothalamic set-points controlling metabolic responses by targeting TR regulation of trh and mc4r (Decherf et al., 2010). In the polar bear Ursus maritimus, an heavily polluted organism for which some EDC are banned for decades (Routti et al., 2019), some EDC, such as organochlorine and perfluoroalkyl, are negatively correlated with plasma TH levels (Bourgeon et al., 2017). In wild chimpanzees, contamination by polluted drinking waters containing pesticides (Krief et al., 2017) and bisphenols (Krief et al., 2020) has been reported, and the water samples exhibit TH disrupting activities (Spirhanzlova et al., 2019). Experimental exposure of Xenopus laevis tadpoles to a mixture of 15 chemicals at concentrations reported in human amniotic fluid induces variation of behavior, of TH-responsive gene expression and of nervous system development (Fini et al., 2017). Considering the conservation of TH function across vertebrates, one may speculate on such impacts of amniotic fluid chemicals on human fetal brain development.

Environmental and health concerns remain particularly challenging when addressing thyroid hormone axis disruption. Only few chemicals have been tested, the number of test methods is limited and the thyroid system is complex. The development of specific chemical safety testing is required (Browne et al., 2020) with special attention to neurological development (Gilbert et al., 2020; Kortenkamp et al., 2020; O’Shaughnessy and Gilbert, 2020). Attention is also paid to break down the wall between mammalian and non-mammalian vertebrate regulatory testing (Couderq et al., 2020; Holbech et al., 2020). In addition to phenotypic or histological end-points, the use of molecular assays (transcripts, proteins or metabolites) will be more sensitive and most of all will allow detection before adverse effects occur (Fini et al., 2007; Kulkarni and Buchholz, 2013). Development of non-destructive (without euthanasia) biomarkers that provide causal link between the presence of a chemical and an ecological effect are also needed to allow the study of vulnerable populations.

Corticosteroid Function Disruption

The adrenal has been neglected in endocrine disruption regulatory testing strategy while the negative consequences of adrenocortical dysfunction during development have been recognized (Hinson and Raven, 2006; Harvey, 2016). Upstream of the biological effect, an activity mimicking that of GC was measured in surface waters (Schriks et al., 2013). Hydrocortisone was detected but could not explain a significant fraction of the observed GR activity.

GC synthesis pathway is also a target. Different environmental toxicants, including phthalate esters together with bisphenols and their analogs pose deleterious effects on the biosynthesis of GC in vitro (Ahmad et al., 2017; Verma et al., 2018). These observations were confirmed in vivo using nitrate, a major anthropogenic contaminant in the FW environment. In three-spined stickleback Gasterosteus aculeatus L., dissolved inorganic N directly exerts a disruptive influence on the function of the stress axis and GC levels, supporting concerns that nitrate is an EDC (Pottinger, 2017). GC disruption was linked to adverse effect in zebrafish exposed to methylparaben, widely used as antimicrobial preservative. In addition to increase in cortisol levels, animals show alteration of heart rate and hatching percentage as well as signs of anxiety-like behavior (Luzeena Raja et al., 2019).

Finally, because persistent organic pollutants can interact with GR, EDC mixtures were screened for GR translocation and GR transactivation in an in vitro assay (Wilson et al., 2016). EDC mixtures did not induce GR translocation in nucleus nor produce an agonist response in the GR transcriptional assay. However, in the presence of cortisol, some chemicals were found to decrease GR transcriptional activity.

Endocrine Disruptor Chemicals/Compounds and Climate Change: A Worst Combination

Climate change and exposure to EDCs are currently two of the most serious anthropogenic threats to biodiversity and ecosystems. Moreover, the ecological threats posed by EDC are further exacerbated by changing environmental conditions such as temperature, pond drying, food restriction, pH and ultraviolet radiation.

In aquatic environment, global warming may lead to temperature increase associated with either salinity increase due to evaporation or salinity decrease due to ice melting. One study addresses the combinatorial effect of temperature, salinity and diuron, an herbicide and antifouling agent with EDC property (Moreira et al., 2018). Combinatorial treatment of juveniles of the estuarine fish, the inland silverside Menidia beryllina, affects growth and hormonal levels. T₃ increases in all of them, while T₄ increases at low temperature and low salinity and decreases at low temperature and high salinity, in agreement with DIO2 expression. EDC, acidification and other contaminants can also perturb smolt development, resulting in poor survival after salinity increase (Björnsson et al., 2011). In the San Francisco Bay, the rainbow trout experiences warmer waters and saltwater intrusion (Giroux and Schlenk, 2021) leading to fry decrease in survival associated with TH increase. Our last example in teleost fishes highlights the interaction between temperature and perchlorate, a well-known thyroid disruptor (Lee et al., 2014). Overall, the results suggest that perchlorate affects thyroid function and reproduction, and these adverse effects are worsened under high temperature.

As previously described in amphibians, a rapid transition into the juvenile stage is beneficial in stress conditions. Pond desiccation is associated to a decrease in dissolved oxygen and an increase in nitrogen levels for which anthropogenic sources such as chemical fertilizers can be heavily suspected. Ammonium nitrate or hypoxic conditions leads to survival decrease of the Natterjack toad Bufo calamita tadpoles (Ortiz-Santaliestra and Marco, 2015). When both stressors were combined, the lethal effects were additive and include malformations. Global warming lead also to predator-prey relationship modifications decreasing survival rates of tadpoles (Jara et al., 2019). In addition, the Bullfrog sensitivity to temperature leads to corticosterone hormonal changes that correlate with immunosuppression (Lima et al., 2020) and increases sensitivity to emerging infectious diseases in the concept of OneHealth. Urodela amphibians are also affected. Compared to a single exposure, Arizona tiger salamander larvae subjected to both temperature increase and perchlorate treatment further decrease their rate of development. These cotreated salamander larvae also present a significant smaller body mass and worse body condition.

Finally, Artic biodiversity is concerned by this double threat. EDC were measured in Arctic marine mammals and seabirds. The most pronounced relationships with endocrine function have been reported with the thyroid hormone system, the sex steroid hormones and cortisol (Jenssen, 2006). Because these endocrine systems are essential for completing life cycles and enabling animals to respond adequately to environmental stress, EDC may interfere with adaptations to increased stress situations.

Conclusion

We have highlighted the roles of TH- and CS-regulated developmental transitions in the innovation, adaptation and plasticity of life cycles in vertebrates. In one of his review, Buchholz discusses the similarities between birth in mammals and metamorphosis in frog with a focus on their regulation by TH and GC (Buchholz, 2015). He reminds us that “both frogs and mammals undergo a life history transition from aquatic (water and amniotic fluid) to terrestrial habitat,” involving for the most striking examples, air-breathing thanks to lung maturation and maturation of the intestine to cope with the transition to a new food source. Similar TH and CS concentration profiles are observed in certain birds and reptiles at hatching and during molting, as well as in certain teleost fishes at hatching and during larval metamorphosis and smoltification (Wada, 2008). The multiple cross-talks between HPT and HPA/HPI axes represent critical mechanisms by which vertebrates modulate their perinatal/post-embryonic development as well as their responses to a changing environment (Figure 4).

The exposome includes stressors with, for some, potential mortality risk by their long-term effects. Vertebrate respond to the risk/benefit trade-off by modulating the production of hormones by the stress and thyroid neuroendocrine axes. In this context, global warming leads to increases in average temperature and temperature variability. Considered as a threat for biodiversity (Radchuk et al., 2019), global warming is a well-known reprotoxicity risk (Parisi and Guerriero, 2019). However, the properties of TH and CS suggest their fundamental roles in thermal acclimation (de Bruijn and Romero, 2018), and evolution of ectothermy/endothermy (Little, 2021). Changes in hormone sensitivity at warm temperatures could mean that increasing temperatures will reduce the capacity of animals to regulate their physiologies to match demands. Aquatic and terrestrial environments are also increasingly contaminated by anthropogenic sources. The contaminants include pharmaceuticals, personal care products, and industrial and agricultural chemicals. Many of these chemicals have the potential to disrupt endocrine function that may lead to disease or foundations to disease later in life as well as disease transmission to descendants (Gore et al., 2015). The adverse effects including metabolic diseases, decreased capacity of reproduction, hormone-sensitive cancers, thyroid disorders, and neurological defects may contribute to population decline. The difficulties tie in the circumstances EDC act, including non-monotonic dose-responses, low-dose effects, and developmental vulnerability. Possible roles for the neuroendocrine stress axis in mediating these developmental responses requires further investigation.

Publisher’s Note

All claims expressed in this article are solely those of the authors and do not necessarily represent those of their affiliated organizations, or those of the publisher, the editors and the reviewers. Any product that may be evaluated in this article, or claim that may be made by its manufacturer, is not guaranteed or endorsed by the publisher.

References

• 1

  AdamsA.BullA. (1949). The effects of antithyroid drugs of chick embryos.Anat. Rec.104421–443.

  • Google Scholar

• 2

  AertsJ. (2018). Quantification of a glucocorticoid profile in non-pooled samples is pivotal in stress research across vertebrates.Front. Endocrinol. (Lausanne)9:635. 10.3389/fendo.2018.00635

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 3

  AhmadS.KhanM. F.ParvezS.AkhtarM.RaisuddinS. (2017). Molecular docking reveals the potential of phthalate esters to inhibit the enzymes of the glucocorticoid biosynthesis pathway.J. Appl. Toxicol.37265–277. 10.1002/jat.3355

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 4

  AlexanderD. P.BrittonH. G.JamesV. H.NixonD. A.ParkerR. A.WintourE. M.et al (1968). Steroid secretion by the adrenal gland of foetal and neonatal sheep.J. Endocrinol.401–13. 10.1677/joe.0.0400001

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 5

  AlfonsoS.GestoM.SadoulB. (2020). Temperature increase and its effects on fish stress physiology in the context of global warming.J. Fish. Biol.981496–1508.

  • Google Scholar

• 6

  AluruN.VijayanM. M. (2008). Molecular characterization, tissue-specific expression, and regulation of melanocortin 2 receptor in rainbow trout.Endocrinology1494577–4588. 10.1210/en.2008-0435

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 7

  AlvesR. N.CardosoJ. C. R.HarboeT.MartinsR. S. T.ManchadoM.NorbergB.et al (2017). Duplication of Dio3 genes in teleost fish and their divergent expression in skin during flatfish metamorphosis.Gen. Comp. Endocrinol.246279–293. 10.1016/j.ygcen.2017.01.002

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 8

  AraiM.AssilI.Abou-SamraA. (2001). Characterization of three corticotropin-releasing factor receptors in catfish: a novel third receptor is predominantly expressed in pituitary and urophysis.Endocrinology142446–454. 10.1210/en.142.1.446

  • CrossRef
  • Google Scholar

• 9

  ArjonaF. J.Vargas-ChacoffL.Martin del RioM. P.FlikG.ManceraJ. M.KlarenP. H. M. (2011). Effects of cortisol and thyroid hormone on periphearl outer ring deiodination and osmoregulatory parameters in the Senegalese sole (Solea senegalensis).J. Endocrinol.208323–330.

  • Google Scholar

• 10

  BagamasbadP. D.BonettR. M.SachsL.BuisineN.RajS.KnoedlerJ. R.et al (2015). Deciphering the regulatory logic of an ancient, ultraconserved nuclear receptor enhancer module.Mol. Endocrinol.29856–872. 10.1210/me.2014-1349

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 11

  BaggermanB. (1963). The effect of TSH and antithyroid substances on salinity preference and thyroid activity in juvenile pacific salmon.Can. J. Zool.41307–319.

  • Google Scholar

• 12

  BakerM. E.KatsuY. (2019). Evolution of the mineralocorticoid receptor.Vitam. Horm.10917–36. 10.1016/bs.vh.2018.10.009

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 13

  BalabanM.HillJ. (1971). Effects of thyroxine level and temperature manipulations upon the hatching of chick embryos (Gallus domesticus).Dev. Psychobiol.417–35. 10.1002/dev.420040103

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 14

  BallardP. L.HoveyM. L.GonzalesL. K. (1984). Thyroid hormone stimulation of phosphatidylcholine synthesis in cultured fetal rabbit lung lung. since glucocorticoids stimulate surfactant synthesis drome in premature infants, we also examined the choline was determined in organ cultures of rabbit lun.J. Clin. Invest.74898–905.

  • Google Scholar

• 15

  BarnesR. J.ComlineR. S.SilverM. (1977). The effects of bilateral adrenalectomy or hypophysectomy of the foetal lamb in utero.J. Physiol.264429–447. 10.1113/jphysiol.1977.sp011676

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 16

  BartonB. A.SchreckC. B.EwingR. D.HemmingsenA. R.PatiñoR. (1985). Changes in plasma cortisol during stress and smoltification in Coho Salmon, Oncorhynchus kisutch.Gen. Comp. Endocrinol.59468–471. 10.1016/0016-6480(85)90406-X

  • CrossRef
  • Google Scholar

• 17

  BeldadeR.BlandinA.O’DonnellR.MillsS. (2017). Cascading effects of thermally-induced anemone bleaching on associated anemonefish hormonal stress response and reproduction.Nat. Commun.8:716. 10.1038/s41467-017-00565-w

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 18

  BernierN. J.FlikG.KlarenP. H. M. (2009). Regulation and contribution of corticotropic, melanotropic and thyrotropic axes to the stress response in fishes.Fish Physiol.28235–311. 10.1016/S1546-5098(09)28006-X

  • CrossRef
  • Google Scholar

• 19

  BerryX.BanuX.LarsenX. (1991). Type I iodothyronine deiodinase is a selenocysteine-containing enzyme.Nature349438–440.

  • Google Scholar

• 20

  BessonM.FeeneyW.MonizI.FRançoisL.BrookerR.HolzerG.et al (2020). Anthropogenic stressors impact fish sensory development and survival via thyroid disruption.Nat. Commun.11:3614. 10.1038/s41467-020-17450-8

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 21

  BiancoA. C.SalvatoreD.GerebenB.BerryM. J.LarsenP. R. (2002). Biochemistry, cellular and molecular biology, and physiological roles of the iodothyronine selenodeiodinases.Endocr. Rev.2338–89. 10.1210/edrv.23.1.0455

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 22

  BidaudI.LoryP.NicolasP.BulantM.LadramA. (2002). Characterization and functional expression of cDNAs encoding thyrotropin-releasing hormone receptor from Xenopus laevis: Identification of a novel subtype of thyrotropin-releasing hormone receptor.Eur. J. Biochem.2694566–4576. 10.1046/j.1432-1033.2002.03152.x

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 23

  BilesimoP.JolivetP.AlfamaG.BuisineN.Le MevelS.HavisE.et al (2011). Specific histone lysine 4 methylation patterns define TR-binding capacity and differentiate direct T3 responses.Mol. Endocrinol.25225–237. 10.1210/me.2010-0269

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 24

  BishopC. D.ErezyilmazD. F.FlattT.GeorgiouC. D.HadfieldM. G.HeylandA.et al (2006). What is metamorphosis?Integr. Comp. Biol.46655–661. 10.1093/icb/icl004

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 25

  BjörnssonB. T.EinarsdottirI. E.PowerD. (2012). Is salmon smoltification an example of vertebrate metamorphosis? Lessons learnt from work on flatfish larval development.Aquaculture362–363264–272. 10.1016/j.aquaculture.2011.03.002

  • CrossRef
  • Google Scholar

• 26

  BjörnssonB. T.StefanssonS. O.McCormickS. D. (2011). Environmental endocrinology of salmon smoltification.Gen. Comp. Endocrinol.170290–298. 10.1016/j.ygcen.2010.07.003

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 27

  BoeufG. (1993). “Salmonid smolting: a pre-adaptation to the oceanic environment,” in Fish Ecophysiology, edsRankinJ.JensenF. (London: Chapman Press), 105–135.

  • Google Scholar

• 28

  BonettR. M.HuF.BagamasbadP.DenverR. J. (2009). Stressor and glucocorticoid-dependent induction of the immediate early gene krüppel-like factor 9: implications for neural development and plasticity.Endocrinology1501757–1765. 10.1210/en.2008-1441

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 29

  BonettR.HoopferE.DenverR. (2010). Molecular mechanisms of corticosteroid synergy with thyroid hormone during tadpole metamorphosis.Gen. Comp. Endocrinol.168209–219.

  • Google Scholar

• 30

  BoonstraR.BodnerK.BossonC.ElehantyB.RichardsonE.LunnN.et al (2020). The stress of arctic warming on polar bears.Golb. Chang. Biol.264197–4214.

  • Google Scholar

• 31

  BorgesM.LaboureneJ.IngbarS. H. (1980). Changes in hepatic iodothyronine metabolism during ontogeny of the chick embryo.Endocrinology1071751–1761. 10.1210/endo-107-6-1751

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 32

  BoscM. (1973). Modification de la durée de gestation de la truie après administration d’ACTH aux foestus.Comptes Rendus Hebd. Des Seances L Acad. Des Sci. Ser. D2763183–3186.

  • Google Scholar

• 33

  BourgeonS.RiemerA. K.TartuS.AarsJ.PolderA.JenssenB. M.et al (2017). Potentiation of ecological factors on the disruption of thyroid hormones by organo-halogenated contaminants in female polar bears (Ursus maritimus) from the Barents Sea.Environ. Res.15894–104. 10.1016/j.envres.2017.05.034

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 34

  BrooksA.SweeneyG.OldR. (1989). Structure and functional expression of a cloned Xenopus thyroid hormone receptor.Nucleic Recept. Res179395–9405.

  • Google Scholar

• 35

  BrownC.UrbinatiE.ZhangW.BrownS.McComb-KobzaM. (2014). Maternal thyroid and glucocorticoid hormone interactions in larval fish development, and their applications in aquaculture.Rev. Fish. Sci. Aquac.22207–220.

  • Google Scholar

• 36

  BrowneP.Van Der WalL.GourmelonA. (2020). OECD approaches and considerations for regulatory evaluation of endocrine disruptors.Mol. Cell. Endocrinol.504:110675. 10.1016/j.mce.2019.110675

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 37

  BuchholzD. R. (2015). More similar than you think: frog metamorphosis as a model of human perinatal endocrinology.Dev. Biol.408188–195. 10.1016/j.ydbio.2015.02.018

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 38

  BuchholzD. R. (2017). Xenopus metamorphosis as a model to study thyroid hormone receptor function during vertebrate developmental transitions.Mol. Cell. Endocrinol.45964–70. 10.1016/j.mce.2017.03.020

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 39

  BuchholzD. R.ShiY. B. (2018). Dual function model revised by thyroid hormone receptor alpha knockout frogs.Gen. Comp. Endocrinol.265214–218. 10.1016/j.ygcen.2018.04.020

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 40

  BuchholzD. R.HsiaS.-C. V.FuL.ShiY.-B. (2003). A dominant-negative thyroid hormone receptor blocks amphibian metamorphosis by retaining corepressors at target genes.Mol. Cell. Biol.236750–6758. 10.1128/mcb.23.19.6750-6758.2003

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 41

  BuchholzD. R.TomitaA.FuL.PaulB. D.ShiY.-B. (2004). Transgenic analysis reveals that thyroid hormone receptor is sufficient to mediate the thyroid hormone signal in frog metamorphosis.Mol. Cell. Biol.249026–9037. 10.1128/mcb.24.20.9026-9037.2004

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 42

  BuryN. R. (2017). The evolution, structure and function of the ray finned fish (Actinopterygii) glucocorticoid receptors.Gen. Comp. Endocrinol.2514–11. 10.1016/j.ygcen.2016.06.030

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 43

  CampinhoM. A.Galay-BurgosM.SweeneyG. E.PowerD. M. (2010). Coordination of deiodinase and thyroid hormone receptor expression during the larval to juvenile transition in sea bream (Sparus aurata, Linnaeus).Gen. Comp. Endocrinol.165181–194. 10.1016/j.ygcen.2009.06.020

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 44

  CampinhoM. A.SilvaN.MartinsG. G.AnjosL.FlorindoC.Roman-PadillaJ.et al (2018). A thyroid hormone regulated asymmetric responsive centre is correlated with eye migration during flatfish metamorphosis.Sci. Rep.81–12. 10.1038/s41598-018-29957-8

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 45

  CardosoJ. C. R.BergqvistC. A.FélixR. C.LarhammarD. (2016). Corticotropin-releasing hormone family evolution: five ancestral genes remain in some lineages.J. Mol. Endocrinol.5773–86. 10.1530/JME-16-0051

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 46

  CardosoJ. C. R.Laiz-CarrionR.LouroB.SilvaN.CanarioA. V. M.ManceraJ. M.et al (2011). Divergence of duplicate POMC genes in gilthead sea bream Sparus auratus.Gen. Comp. Endocrinol.173396–404. 10.1016/j.ygcen.2010.12.001

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 47

  CarsiaR. V.MorinM. E.RosenH.WeberH. (1987). Ontogenic corticosteroidogenesis of the domestic fowl: response of isolated adrenocortical cells.Proc. Soc. Exp. Biol. Med.184436–445.

  • Google Scholar

• 48

  CaseyB. M.DasheJ. S.WellsC. E.McIntireD. D.ByrdW.LevenoK. J.et al (2005). Subclinical hypothyroidism and pregnancy outcomes.Obstet. Gynecol.105239–245. 10.1097/01.AOG.0000152345.99421.22

  • CrossRef
  • Google Scholar

• 49

  Castañeda-CortésD. C.Arias PadillaL. F.LangloisV. S.SomozaG. M.FernandinoJ. I. (2019). The central nervous system acts as a transducer of stress-induced masculinization through corticotropin-releasing hormone B.Development (Cambridge)146:dev172866.

  • Google Scholar

• 50

  Castañeda-CortésD. C.ZhangJ.BoanA. F.LangloisV. S.FernandinoJ. I. (2020). High temperature stress response is not sexually dimorphic at the whole-body level and is dependent on androgens to induce sex reversal.Gen. Comp. Endocrinol.299:113605.

  • Google Scholar

• 51

  ChallisJ. R. G.HooperS. (1989). Birth: outcome of a positive cascade.Baillieres Clin. Endocrinol. Metab.3781–793. 10.1016/S0950-351X(89)80053-9

  • CrossRef
  • Google Scholar

• 52

  ChanE.FalconerJ.MadsenG.RiceK.WebsterE.ChrousosG.et al (1998). A corticotropin-releasing hromone type I receptor antagonist delays parturition in sheep.Endocrinology1393357–3360.

  • Google Scholar

• 53

  ChenX.RenC.TengY.ShenY.WuM.XiaoH.et al (2021). Effects of temperature on growth, development and the leptin signaling pathway of Bufo gargarizans.J. Therm. Biol.96:102822. 10.1016/j.jtherbio.2020.102822

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 54

  Chester-JonesI. (1987). “Structure of the adrenal and interrenal glands,” in Fundamentals of Comparative Vertebrate Endocrinology, edsChester-JonesI.IngletonP. M.PhillipsJ. G. (Boston, MA: Springer), 95–121. 10.1007/978-1-4899-3617-2_3

  • CrossRef
  • Google Scholar

• 55

  ChristensenV. L. (1985). Supplemental thyroid hormones and hatchability of turkey eggs.Poult. Sci.642202–2210. 10.3382/ps.0642202

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 56

  ConeR. D. (2006). Studies on the physiological functions of the melanocortin system.Endocr. Rev.27736–749. 10.1210/er.2006-0034

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 57

  CortésR.NavarroS.AgulleiroM. J.GuillotR.García-HerranzV.SánchezE.et al (2014). Evolution of the melanocortin system.Gen. Comp. Endocrinol.2093–10. 10.1016/j.ygcen.2014.04.005

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 58

  CouderqS.LeemansM.FiniJ. B. (2020). Testing for thyroid hormone disruptors, a review of non-mammalian in vivo models.Mol. Cell. Endocrinol.508:110779. 10.1016/j.mce.2020.110779

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 59

  CoughlinD. J.ForryJ. A.McGlincheyS. M.MitchellJ.SaporettiK. A.StaufferK. A. (2001). Thyroxine induces transitions in red muscle kinetics and steady swimming kinematics in rainbow trout (Oncorhynchus mykiss).J. Exp. Zool.290115–124. 10.1002/jez.1041

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 60

  DardenteH.WoodS.EblingF.Sáenz de MieraC. (2019). An integrative view of mammalian seasonal neuroendocrinology.J. Neuroendocrinol.311–17. 10.1111/jne.12729

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 61

  DarrasV. M.Van HerckS. L. J. (2012). Iodothyronine deiodinase structure and function: from ascidians to humans.J. Endocrinol.215189–206. 10.1530/JOE-12-0204

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 62

  DarrasV. M.KotanenS. P.GerisK. L.KühnE. R. (1996). Plasma thyroid hormone levels and iodothyronine deiodinase activity following an acute glucocorticoid challenge in embryonic compared with posthatch chickens.Gen. Comp. Endocrinol.104203–212. 10.1006/gcen.1996.0163

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 63

  DarrasV. M.VisserT. J.BerghmanL. R.KühnE. R. (1992). Ontogeny of type I and type III deiodinase activities in embryonic and posthatch chicks: relationship with changes in plasma triiodothyronine and growth hormone levels.Comp. Biochem. Physiol. Part A Physiol.103131–136. 10.1016/0300-9629(92)90252-L

  • CrossRef
  • Google Scholar

• 64

  DasD.AyromlooiJ.BandyopadhyayD.BandyopadhyayS.NeogiA.SteinbergH. (1984). Potentiation of surfactant release in fetal lung by thyroid hormone action.J. Appl. Physiol.561621–1626.

  • Google Scholar

• 65

  DaveyJ. C.BeckerK. B.SchneiderM. J.St. GermainD. L.GaltonV. A. (1995). Cloning of a cDNA for the type II iodothyronine deiodinase.J. Biol. Chem.27026786–26789. 10.1074/jbc.270.45.26786

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 66

  de BruijnR.RomeroL. M. (2018). The role of glucocorticoids in the vertebrate response to weather.Gen. Comp. Endocrinol.26911–32. 10.1016/j.ygcen.2018.07.007

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 67

  De GroefB.GrommenS. V. H.DarrasV. M. (2013). Hatching the cleidoic egg: the role of thyroid hormones.Front. Endocrinol. (Lausanne)4:63. 10.3389/fendo.2013.00063

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 68

  De GroefB.Van Der GeytenS.DarrasV. M.KühnE. R. (2006). Role of corticotropin-releasing hormone as a thyrotropin-releasing factor in non-mammalian vertebrates.Gen. Comp. Endocrinol.14662–68. 10.1016/j.ygcen.2005.10.014

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 69

  de JesusE. G. T.ToledoJ. D.SimpasM. S. (1998). Thyroid hormones promote early metamorphosis in grouper (Epinephelus coioides) larvae.Gen. Comp. Endocrinol.11210–16. 10.1006/gcen.1998.7103

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 70

  de JesusE. G.InuiY.HiranoT. (1990). Cortisol enhances the stimulating action of thyroid hormones on dorsal fin-ray resorption of flounder larvae in vitro.Gen. Comp. Endocrinol.79167–173. 10.1016/0016-6480(90)90101-Q

  • CrossRef
  • Google Scholar

• 71

  de JesusE.HiranoT.InuiY. (1991). Changes in cortisol and thyroid hormone concentrations during early development and metamorphosis in the Japanese flounder, Paralichthys olivaceus.Gen. Comp. Endocrinol.82369–376.

  • Google Scholar

• 72

  De SouzaF. S. J.BumaschnyV. F.LowM. J.RubinsteinM. (2005). Subfunctionalization of expression and peptide domains following the ancient duplication of the proopiomelanocortin gene in teleost fishes.Mol. Biol. Evol.222417–2427. 10.1093/molbev/msi236

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 73

  DecherfS.SeugnetI.FiniJ. B.Clerget-FroidevauxM. S.DemeneixB. A. (2010). Disruption of thyroid hormone-dependent hypothalamic set-points by environmental contaminants.Mol. Cell. Endocrinol.323172–182. 10.1016/j.mce.2010.04.010

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 74

  DecuypereE.ScanesC.KühnE. (1983). Effects of glucocorticoids on circulating concentrations of thyroxine (t4) and triiodothyronine (t3) and on peripheral monodeiodination in pre- and post-hatching chicken.Horm. Metab. Res.15233–236.

  • Google Scholar

• 75

  DefoM. A.DouvilleM.GiraudoM.BrodeurP.BoilyM.HoudeM. (2018). RNA-sequencing to assess the health of wild yellow perch (Perca flavescens) populations from the St. Lawrence River, Canada.Environ. Pollut.2431657–1668. 10.1016/j.envpol.2018.09.133

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 76

  DehalP.BooreJ. L. (2005). Two rounds of whole genome duplication in the ancestral vertebrate.PLoS Biol.3:e314. 10.1371/journal.pbio.0030314

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 77

  DenverR. (2009). “Endocrinology of complex life cycles: amphibians,” in Hormones, Brain and Behavior, edsPfaffD.ArnoldA.EtgenA.RubinR.FahrbachS. (Amsterdam: Elsevier), 707–744.

  • Google Scholar

• 78

  DenverR. (2017). “Endocrinology of complex life cycles: amphibians,” in Hormones, Brain and Behavior, edsPfaffD.MarianJ. (Oxford: Academic Press), 145–148.

  • Google Scholar

• 79

  DenverR. J. (1993). Acceleration of anuran amphibian metamorphosis by corticotropin-releasing hormone-like peptides.Gen. Comp. Endocrinol.9138–51. 10.1006/gcen.1993.1102

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 80

  DenverR. J. (1997). Environmental stress as a developmental cue: corticotropin- releasing hormone is a proximate mediator of adaptive phenotypic plasticity in amphibian metamorphosis.Horm. Behav.31169–179. 10.1006/hbeh.1997.1400

  • CrossRef
  • Google Scholar

• 81

  DenverR. J. (2021). Stress hormones mediate developmental plasticity in vertebrates with complex life cycles.Neurobiol. Stress14:100301. 10.1016/j.ynstr.2021.100301

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 82

  DenverR. J.HuF.ScanlanT. S.FurlowJ. D. (2009). Thyroid hormone receptor subtype specificity for hormone-dependent neurogenesis in Xenopus laevis.Dev. Biol.326155–168. 10.1016/j.ydbio.2008.11.005

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 83

  DimondM.-T. (1954). The reactions of developing snapping turtles, Chelydra serpentina serpentina (Linné), to thiourea.J. Exp. Zool.12793–117.

  • Google Scholar

• 84

  DoresR. M.GarciaY. (2015). Views on the co-evolution of the melanocortin-2 receptor, MRAPs, and the hypothalamus/pituitary/adrenal-interrenal axis.Mol. Cell. Endocrinol.40812–22. 10.1016/j.mce.2014.12.022

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 85

  DoresR. M.LondravilleR. L.ProkopJ.DavisP.DeweyN.LesinskiN. (2014). Molecular evolution of GPCRs: melanocortin/melanocortin receptors.J. Mol. Endocrinol.52T29–T42. 10.1530/JME-14-0050

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 86

  DoresR.LecaudéS.BauerD.DanielsonP. (2002). Analyzing the evolution of the opioid/orphanin gene family.Mass Spectrom. Rev.21220–243. 10.1002/mas.10029

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 87

  DuboisJ.DussaultJ. (1977). Ontogenesis of thyroid function in the neonatal rat. Thyroxine and triiodothyronine production rates.Endocrinology101435–441.

  • Google Scholar

• 88

  DupouéA.RutschmannA.Le GalliardJ. F.ClobertJ.BlaimontP.SinervoB.et al (2018). Reduction in baseline corticosterone secretion correlates with climate warming and drying across wild lizard populations.J. Anim. Ecol.871331–1341. 10.1111/1365-2656.12843

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 89

  EalesJ.MorinP.TsangP.HaraT. (1993). Thyroid hormone deiodination in brain, liver, gill, heart and msucle of Atlantic salmon (Salmo salar) during the photoperiodically-induced parr-smolt transformation. II. Outer- and inner-ring 3,5,3’-triiodo-L-thyronine and 3,3’,5’-triiodothyronine-L-thyro.Gen. Comp. Endocrinol.90157–167.

  • Google Scholar

• 90

  EbbessonL. O. E.NilsenT. O.HelvikJ. V.TronciV.StefanssonS. O. (2011). Corticotropin-releasing factor neurogenesis during midlife development in salmon: genetic, environmental and thyroid hormone regulation.J. Neuroendocrinol.23733–741. 10.1111/j.1365-2826.2011.02164.x

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 91

  EinarsdóttirI. E.SilvaN.PowerD. M.SmáradóttirH.BjörnssonB. T. (2006). Thyroid and pituitary gland development from hatching through metamorphosis of a teleost flatfish, the Atlantic halibut.Anat. Embryol. (Berl)21147–60. 10.1007/s00429-005-0055-z

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 92

  Enriquez-UrzelaiU.San SebastiánO.GarrigaN.LlorenteG. A. (2013). Food availability determines the response to pond desiccation in anuran tadpoles.Oecologia173117–127. 10.1007/s00442-013-2596-9

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 93

  FaughtE.AluruN.VijayanM. M. (2016). “The molecular stress response,” in Biology of Stress in Fish – Fish Physiology, edsSchreckC. B.TortL.FarrellA. P.BraunerC. J. (Amsterdam: Elsevier Inc), 113–166. 10.1016/B978-0-12-802728-8.00004-7

  • CrossRef
  • Google Scholar

• 94

  FernieK. J.ChabotD.ChampouxL.BrimbleS.AlaeeM.MarteinsonS.et al (2017). Spatiotemporal patterns and relationships among the diet, biochemistry, and exposure to flame retardants in an apex avian predator, the peregrine falcon.Environ. Res.15843–53. 10.1016/j.envres.2017.05.035

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 95

  FilipssonK.BergmanE.GreenbergL.ÖsterlingM.WatzJ.ErlandssonA. (2020). Temperature and predator-mediated regulation of plasma cortisol and brain gene expression in juvenile brown trout (Salmo trutta).Front. Zool.17:25. 10.1186/s12983-020-00372-y

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 96

  FiniJ. B.MughalB. B.Le MévelS.LeemansM.LettmannM.SpirhanzlovaP.et al (2017). Human amniotic fluid contaminants alter thyroid hormone signalling and early brain development in Xenopus embryos.Sci. Rep.71–12. 10.1038/srep43786

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 97

  FiniJ.Le MevelS.TurqueN.PalmierK.ZalkoD.CravediJ.et al (2007). An in vivo multiwell-based fluorescent screen for monitoring vertebrate thyroid hormone disruption.Env. Sci. Technol.415908–5914. 10.1021/es0704129

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 98

  FlemingM. S.MaugarsG.LafontA.-G.RanconJ.FontaineR.Nourizadeh-LillabadiR.et al (2019). Functional divergence of thyrotropin beta-subunit paralogs gives new insights into salmon smoltification metamorphosis.Sci. Rep.9:4561. 10.1038/s41598-019-40019-5

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 99

  ForheadA. J.FowdenA. L. (2014). Thyroid hormones in fetal growth and prepartum maturation.J. Endocrinol.221R87–R103. 10.1530/JOE-14-0025

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 100

  ForheadA. J.CurtisK.KapteinE.VisserT. J.FowdenA. L. (2006). Developmental control of iodothyronine deiodinases by cortisol in the ovine fetus and placenta near term.Endocrinology1475988–5994. 10.1210/en.2006-0712

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 101

  ForrestD.SjobergM.VennstromB. (1990). Contrasting developmental and tissue-specific expression of α and β thyroid hormone receptor genes.EMBO J.91519–1528. 10.1002/j.1460-2075.1990.tb08270.x

  • CrossRef
  • Google Scholar

• 102

  FowdenA. L.ForheadA. J. (2009). Hormones as epigenetic signals in developmental programming.Exp. Physiol.94607–625. 10.1113/expphysiol.2008.046359

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 103

  FowdenA. L.ForheadA. J. (2015). Glucocorticoids as regulatory signals during intrauterine development.Exp. Physiol.1001477–1487. 10.1113/EP085212

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 104

  FowdenA. L.ValenzuelaO. A.VaughanO. R.JellymanJ. K.ForheadA. J. (2016). Glucocorticoid programming of intrauterine development.Domest. Anim. Endocrinol.56S121–S132. 10.1016/j.domaniend.2016.02.014

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 105

  FreireR.Van DortS.RogersL. J. (2006). Pre- and post-hatching effects of corticosterone treatment on behavior of the domestic chick.Horm. Behav.49157–165. 10.1016/j.yhbeh.2005.05.015

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 106

  FrigerioD.MoestlE.KotrschalK. (2001). Excreted metabolites of gonadal steroid hormones and corticosterone in greylag geese (Anser anser) from hatching to fledging.Gen. Comp. Endocrinol.124246–255. 10.1006/gcen.2001.7706

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 107

  FurlowJ. D.NeffE. S. (2006). A developmental switch induced by thyroid hormone: Xenopus laevis metamorphosis.Trends Endocrinol. Metab.1740–47. 10.1016/j.tem.2006.01.007

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 108

  GalasL.RaoultE.TononM. C.OkadaR.JenksB. G.CastañoJ. P.et al (2009). TRH acts as a multifunctional hypophysiotropic factor in vertebrates.Gen. Comp. Endocrinol.16440–50. 10.1016/j.ygcen.2009.05.003

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 109

  Galay-BurgosM.PowerD. M.LlewellynL.SweeneyG. E. (2008). Thyroid hormone receptor expression during metamorphosis of Atlantic halibut (Hippoglossus hippoglossus).Mol. Cell. Endocrinol.28156–63. 10.1016/j.mce.2007.10.009

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 110

  GaltonV. (1989). The role of 3,5,3’-triiodothyronine in the physiological action of thyroxine in the premetamorphic tadpole.Endocrinol. Endocrinol.1242427–2433.

  • Google Scholar

• 111

  GaltonV. (1990). Mechanisms underlying the acceleration of thyroid hormone-induced tadpole metamorphosis by corticosterone.Endocrinology1272997–3002. 10.1210/endo-127-6-2997

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 112

  GaltonV. A.HiebertA. (1987). The ontogeny of the enzyme systems for the 5- and 5-deiodination of thyroid hormones in chick embryo liver.Endocrinology1202604–2610. 10.1210/endo-120-6-2604

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 113

  GilbertM. E.O’ShaughnessyK. L.AxelstadM. (2020). Regulation of thyroid-disrupting chemicals to protect the developing brain.Endocrinology (United States)1611–17. 10.1210/endocr/bqaa106

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 114

  GilbertW. M.Eby-WilkensE.PlopperC.WhitsettJ. A.TarantalA. F. (2001). Fetal monkey surfactants after intra-amniotic or maternal administration of betamethasone and thyroid hormone.Obstet. Gynecol.98466–470. 10.1016/S0029-7844(01)01417-X

  • CrossRef
  • Google Scholar

• 115

  GilmourK. M. (2005). Mineralocorticoid receptors and hormones: fishing for answers.Endocrinology14644–46. 10.1210/en.2004-1390

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 116

  GirouxM.SchlenkD. (2021). The effects of temperature and salinity on the endocrinology in two life stages of juvenile rainbow/steelhead trout (Oncorhynchus mykiss).J. Fish. Biol.99513–523. 10.1111/jfb.14741

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 117

  GlennemeierK. A.DenverR. J. (2002). Developmental changes in interrenal responsiveness in anuran amphibians.Integr. Comp. Biol.42565–573. 10.1093/icb/42.3.565

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 118

  GodartM.FrauC.FarhatD.GiolitoM.JamardC.Le NevéC.et al (2021). Murine intestinal stem cells are highly sensitive to modulation of the T3/TRα1-dependent pathway.Development148:dev194357.

  • Google Scholar

• 119

  Gomez-MestreI.KulkarniS.BuchholzD. R. (2013). Mechanisms and consequences of developmental acceleration in tadpoles responding to pond drying.PLoS One8:e84266. 10.1371/journal.pone.0084266

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 120

  GonzalezL.BallardP.ErtzeyR.WilliamsM. (1986). Glucocorticoids and thyroid hormones stimulate biochemical and morphological differentiation of human fetal lung in organ culture.J. Clin. Endocrinol. Metab.62678–691.

  • Google Scholar

• 121

  GoreA.ChappellV.FentonS.FlawsJ.NadalA.PrinsG.et al (2015). Executive summary to EDC-2: the endocrine society’s second scientific statement on endocrine-disrupting chemicals.Endocr. Rev.36593–602. 10.1210/er.2015-1093

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 122

  GorissenM.FlikG. (2016). “The endocrinology of the stress response in fish: an adaptation-physiological view,” in Biology of Stress In Fish: Fish Physiology, Vol. 35edsSchreckC.TortL.FarrellA.BraunerC. (London: Elsevier), 75–111.

  • Google Scholar

• 123

  GrimaldiA.BuisineN.MillerT.ShiY. B.SachsL. M. (2013). Mechanisms of thyroid hormone receptor action during development: lessons from amphibian studies.Biochim. Biophys. Acta Gen. Subj.18303882–3892. 10.1016/j.bbagen.2012.04.020

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 124

  GroneB. P.MaruskaK. P. (2015). Divergent evolution of two corticotropin-releasing hormone (CRH) genes in teleost fishes.Front. Neurosci.9:365. 10.3389/fnins.2015.00365

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 125

  GrossowiczN. (1946). Influence of thiourea on development of the chick embryo.Proc. Soc. Exp. Biol. Med.63151–152.

  • Google Scholar

• 126

  GudernatchJ. (1912). Feeding experiments on tadpoles. I. The influence of specific organs given as food on growth and differentiation. A contribution to the knowledge of organs with internal secretion.Arch. Entwicklungsmech. Org.35457–483.

  • Google Scholar

• 127

  GuilleminR.RosenbergB. (1955). Humoral hypothalamic control of anterior pituitary: a study with combined tissue cultures.Endocrinology57599–607.

  • Google Scholar

• 128

  GuilleminR.YamazakiE.GardD. A.JutiszM.SakizE. (1963). In vitro secretion of thyrotropin (TSH): stimulation by a hypothalamic peptide (TRF).Endocrinology73564–572. 10.1210/endo-73-5-564

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 129

  GuilleminR.YamazakiE.JutoszM.SakizE. (1962). Présence dans un extrait de tissus hypothalamiques d’une substance stimulant la sécrétion de l’hormone hypophysaire thyréotrope (TSH). Première purification par filtration sur gel Sephadex.C. R. Acad. Sci. Paris2551018–1020.

  • Google Scholar

• 130

  HabaG.NishigoriH.TezukaY.KagamiK.SugiyamaT.NishigoriH. (2011). Effect of antithyroid drug on chick embryos during the last week of development: delayed hatching and decreased cerebellar acetylcholinesterase activity.J. Obstet. Gynaecol. Res.371549–1556. 10.1111/j.1447-0756.2011.01573.x

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 131

  HaitinaT.KlovinsJ.AnderssonJ.FredrikssonR.LagerströmM. C.LarhammarD.et al (2004). Cloning, tissue distribution, pharmacology and three-dimensional modelling of melanocortin receptors 4 and 5 in rainbow trout suggest close evolutionary relationship of these subtypes.Biochem. J.380475–486. 10.1042/BJ20031934

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 132

  HallidayR.ButtleH. R. (1968). The effects of cortisone acetate on the length of the gestation period and the survival of foetal Scottish Blackface lambs.J. Endocrinol.41447–448. 10.1677/joe.0.0410447

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 133

  HaradaM.YoshinagaT.OjimaD.IwataM. (2008). cDNA cloning and expression analysis of thyroid hormone receptor in the coho salmon Oncorhynchus kisutch during smoltification.Gen. Comp. Endocrinol.155658–667. 10.1016/j.ygcen.2007.09.004

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 134

  HarrisA.FangS.ProskyJ.BravermanL.VagenakisA. (1978). Decreased outer ring monodeiodination of thyroxine and reverse triiodothyronine in fetal and neonatal rats.Endocrinology1032216–2222.

  • Google Scholar

• 135

  HarrisR. M.DijkstraP. D.HofmannH. A. (2014). Complex structural and regulatory evolution of the pro-opiomelanocortin gene family.Gen. Comp. Endocrinol.195107–115. 10.1016/j.ygcen.2013.10.007

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 136

  HarveyP. (2016). Adrenocortical endocrine disruption.J. Steroid Biochem. Mol. Biol.155199–206. 10.1016/j.jsbmb.2014.10.009

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 137

  HayesT.ChanR.LichtP. (1993). Interactions of temperature and steroids on larval growth, development, and metamorphosis in a toad (Bufo boreas).J. Exp. Zool.266206–215. 10.1002/jez.1402660306

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 138

  HaywardL. S.RichardsonJ. B.GroganM. N.WingfieldJ. C. (2006). Sex differences in the organizational effects of corticosterone in the egg yolk of quail.Gen. Comp. Endocrinol.146144–148. 10.1016/j.ygcen.2005.10.016

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 139

  HeijlenM.HoubrechtsA. M.BagciE.Van HerckS. L. J.KersseboomS.EsquerraC. V.et al (2014). Knockdown of type 3 iodothyronine deiodinase severely perturbs both embryonic and early larval development in zebrafish.Endocrinology1551547–1559. 10.1210/en.2013-1660

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 140

  HelbingC. C.CrumpK.BaileyC. M.KohnoS.VeldhoenN.BryanT.et al (2006). Isolation of the alligator (Alligator mississippiensis) thyroid hormone receptor α and β transcripts and their responsiveness to thyroid stimulating hormone.Gen. Comp. Endocrinol.149141–150. 10.1016/j.ygcen.2006.05.019

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 141

  HenriksenR.RettenbacherS.GroothuisT. G. G. (2013). Maternal corticosterone elevation during egg formation in chickens (Gallus gallus domesticus) influences offspring traits, partly via prenatal undernutrition.Gen. Comp. Endocrinol.19183–91. 10.1016/j.ygcen.2013.05.028

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 142

  HinsonJ. P.RavenP. W. (2006). Effects of endocrine-disrupting chemicals on adrenal function.Best Pract. Res. Clin. Endocrinol. Metab.20111–120. 10.1016/j.beem.2005.09.006

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 143

  HoarW. (1976). Smolt transformation: evolution, behaviour, and physiology.J. Fish. Res. Board Can.331234–1252.

  • Google Scholar

• 144

  HoarW. S. (1988). The physiology of smolting salmonids.Fish Physiol.11275–343. 10.1016/S1546-5098(08)60216-2

  • CrossRef
  • Google Scholar

• 145

  HolbechH.MatthiessenP.HansenM.SchüürmannG.KnapenD.ReuverM.et al (2020). ERGO: breaking down the wall between human health and environmental testing of endocrine disrupters.Int. J. Mol. Sci.21:2954. 10.3390/ijms21082954

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 146

  HolzerG.RouxN.LaudetV. (2017). Evolution of ligands, receptors and metabolizing enzymes of thyroid signaling.Mol. Cell. Endocrinol.4595–13. 10.1016/j.mce.2017.03.021

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 147

  HottaY.AritakiM.OhtaK.TagwaM.TanakaM. (2001a). Development of the digestive system and metamorphosis relating hormones in spotted halibut larvae and early juveniles.Nippon Suisan Gakkai.6740–48.

  • Google Scholar

• 148

  HottaY.AritakiM.TagawaM.TanakaM. (2001b). Changes in tissue thyroid hormone levels of metamorphosing spotted halibut Verasper variegatus reared at different temperatures.Fish. Sci.671119–1124. 10.1046/j.1444-2906.2001.00369.x

  • CrossRef
  • Google Scholar

• 149

  HsuB. Y.DijkstraC.DarrasV. M.de VriesB.GroothuisT. G. G. (2017). Maternal thyroid hormones enhance hatching success but decrease nestling body mass in the rock pigeon (Columba livia).Gen. Comp. Endocrinol.240174–181. 10.1016/j.ygcen.2016.10.011

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 150

  HsuB.-Y.SarraudeT.Cossin-SevrinN.CrombecqueM.StierA.RuuskanenS. (2020). Testing for context-dependent effects of prenatal thyroid hormones on offspring survival and physiology: an experimental temperature manipulation.Sci. Rep.10:14563.

  • Google Scholar

• 151

  HuF.KnoedlerJ. R.DenverR. J. (2016). A mechanism to enhance cellular responsivity to hormone action: krüppel-like factor 9 promotes thyroid hormone receptor-β autoinduction during postembryonic brain development.Endocrinology1571683–1693. 10.1210/en.2015-1980

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 152

  HwangJ. I.MoonM. J.ParkS.KimD. K.ChoE. B.HaN.et al (2013). Expansion of secretin-like G protein-coupled receptors and their peptide ligands via local duplications before and after two rounds of whole-genome duplication.Mol. Biol. Evol.301119–1130. 10.1093/molbev/mst031

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 153

  HylkaV. W.DoneenB. A. (1983). Ontogeny of embryonic chicken lung: Effects of pituitary gland, corticosterone, and other hormones upon pulmonary growth and synthesis of surfactant phospholipids.Gen. Comp. Endocrinol.52108–120. 10.1016/0016-6480(83)90163-6

  • CrossRef
  • Google Scholar

• 154

  IkutaK.AidaK.OkumotoN.HanyuI. (1985). Effects of thyroxine and methyltestosterone on smoltification of masu salmon (Oncorhynchus masou).Aquaculture45289–303. 10.1016/0044-8486(85)90276-5

  • CrossRef
  • Google Scholar

• 155

  InuiY.MiwaS. (1985). Thyroid hormone induces metamorphosis of flounder larvae.Gen. Comp. Endocrinol.60450–454. 10.1016/0016-6480(85)90080-2

  • CrossRef
  • Google Scholar

• 156

  InuiY.MiwaS. (2012). “Metamorphosis of flatfish (pleuronectiformes),” in Metamorphosis In Fish, edsDufourS.RousseauK.KapoorB. (Saint Helier: Science Publishers), 107–153.

  • Google Scholar

• 157

  IrachiS.HallD. J.FlemingM. S.MaugarsG.BjörnssonB. T.DufourS.et al (2021). Photoperiodic regulation of pituitary thyroid-stimulating hormone and brain deiodinase in Atlantic salmon.Mol. Cell. Endocrinol.519:111056. 10.1016/j.mce.2020.111056

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 158

  IsornaE.ObregonM. J.CalvoR. M.VázquezR.PendónC.FalcónJ.et al (2009). Iodothyronine deiodinases and thyroid hormone receptors regulation during flatfish (Solea senegalensis) metamorphosis.J. Exp. Zool. Part B Mol. Dev. Evol.312231–246. 10.1002/jez.b.21285

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 159

  ItohK.WatanabeK.WuX.SuzukiT. (2010). Three members of the iodothyronine deiodinase family, dio1, dio2 and dio3, are expressed in spatially and temporally specific patterns during metamorphosis of the flounder Paralichthys olivaceus.Zoolog. Sci.27574–580.

  • Google Scholar

• 160

  IwataM.YamauchiK.NishiokaR.LinR.BernH. (1990). Effects of thyroxine, growth hormone and cortisol on salinity preference of juvenile coho salmon (Oncorhynchus kisutch).Mar. Behav. Physiol.17191–201.

  • Google Scholar

• 161

  IzazA.PanT.WangL.ZhangH.DuanS.LiE.et al (2021). Molecular cloning, characterization, and gene expression behavior of glucocorticoid and mineralocorticoid receptors from the Chinese alligator (Alligator sinensis).J. Exp. Zool. B Mol. Dev. Evol.33650–72.

  • Google Scholar

• 162

  IzumoS.MahdaviV. (1988). Thyroid hormone receptor α isoforms generated by alternative splicing differentially activate myosin HC gene transcription.Nature334539–542. 10.1038/334539a0

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 163

  JanczakA. M.BraastadB. O.BakkenM. (2006). Behavioural effects of embryonic exposure to corticosterone in chickens.Appl. Anim. Behav. Sci.9669–82. 10.1016/j.applanim.2005.04.020

  • CrossRef
  • Google Scholar

• 164

  JaraF.ThurmanL.MontiglioP.SihA.GarciaT. (2019). Warming-induced shifts in amphibian phenology and behavior lead to altered predator-prey dynamics.Oecologia189803–813. 10.1007/s00442-019-04360-w

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 165

  JaudetG. J.HateyJ. L. (1984). Variations in aldosterone and corticosterone plasma levels during metamorphosis in Xenopus laevis tadpoles.Gen. Comp. Endocrinol.5659–65. 10.1016/0016-6480(84)90061-3

  • CrossRef
  • Google Scholar

• 166

  JellymanJ. K.FletcherA. J. W.FowdenA. L.GiussaniD. A. (2020). Glucocorticoid maturation of fetal cardiovascular function.Trends Mol. Med.26170–184. 10.1016/j.molmed.2019.09.005

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 167

  JenningsD. H.MooreM. C.KnappR.MatthewsL.OrchinikM. (2000). Plasma steroid-binding globulin mediation of differences in stress reactivity in alternative male phenotypes in tree lizards, Urosaurus ornatus.Gen. Comp. Endocrinol.120289–299. 10.1006/gcen.2000.7564

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 168

  JenssenB. (2006). Endocrine-disrupting chemicals and climate change: A worst-case combination for arctic marine mammals and seabirds?Env. Heal. Perspect.114 Suppl76–80. 10.1289/ehp.8057

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 169

  Jolivet-JaudetG.Leloup-HâteyJ. (1986). Corticosteroid binding in plasma of Xenopus laevis. Modifications during metamorphosis and growth.J. Steroid Biochem.25343–350. 10.1016/0022-4731(86)90245-1

  • CrossRef
  • Google Scholar

• 170

  JonesI.RogersS. A.KilleP.SweeneyG. E. (2002). Molecular cloning and expression of thyroid hormone receptor alpha during salmonid development.Gen. Comp. Endocrinol.125226–235. 10.1006/gcen.2001.7745

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 171

  KalliecharanR.HallB. K. (1974). A developmental study of the levels of progesterone, corticosterone, cortisol, and cortisone circulating in plasma of chick embryos.Gen. Comp. Endocrinol.24364–372. 10.1016/0016-6480(74)90149-X

  • CrossRef
  • Google Scholar

• 172

  KanahoY. I.EndoD.ParkM. K. (2006). Molecular characterization of thyroid hormone receptors from the leopard gecko, and their differential expression in the skin.Zool. Sci.23549–556. 10.2108/zsj.23.549

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 173

  KiilerichP.KristiansenK.MadsenS. S. (2007). Hormone receptors in gills of smolting Atlantic salmon, Salmo salar: expression of growth hormone, prolactin, mineralocorticoid and glucocorticoid receptors and 11β-hydroxysteroid dehydrogenase type 2.Gen. Comp. Endocrinol.152295–303. 10.1016/j.ygcen.2006.12.018

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 174

  KikuyamaS.NikiK.MayumiM. (1982). Retardation of thyroxine-induced metamorphosis by Amphenone B in toad tadpoles.Endocrinol Jpn.29659–662.

  • Google Scholar

• 175

  KingsburyJ.EmeryS.AdamsA. (1955). Effects of thiourea on the adrenal glands of chick embryos.Endocrinology56299–304.

  • Google Scholar

• 176

  KloasW.ReineckeM.HankeW. (1997). Stage-dependent changes in adrenal steroids and catecholamines during development in Xenopus laevis.Gen. Comp. Endocrinol.108416–426. 10.1006/gcen.1997.6998

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 177

  KobayashiH. (1958). Effect of desoxycorticosterone acetate on metamorphosis induced by throxine in anuran tadpoles.Endocrinology62371–377. 10.1210/endo-62-4-371

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 178

  KobayashiY.ChibaH.YamanomeT.SchiöthH. B.TakahashiA. (2011). Melanocortin receptor subtypes in interrenal cells and corticotropic activity of α-melanocyte-stimulating hormones in barfin flounder, Verasper moseri.Gen. Comp. Endocrinol.170558–568. 10.1016/j.ygcen.2010.11.019

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 179

  KortenkampA.AxelstadM.BaigA. H.BergmanÅBornehagC. G.CenijnP.et al (2020). Removing critical gaps in chemical test methods by developing new assays for the identification of thyroid hormone system-disrupting chemicals—the athena project.Int. J. Mol. Sci.21:3123. 10.3390/ijms21093123

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 180

  KrainL. P.DenverR. J. (2004). Developmental expression and hormonal regulation of glucocorticoid and thyroid hormone receptors during metamorphosis in Xenopus laevis.J. Endocrinol.18191–104. 10.1677/joe.0.1810091

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 181

  KriefS.BernyP.GumisirizaF.GrossR.DemeneixB.FiniJ. B.et al (2017). Agricultural expansion as risk to endangered wildlife: pesticide exposure in wild chimpanzees and baboons displaying facial dysplasia.Sci. Total Environ.598647–656. 10.1016/j.scitotenv.2017.04.113

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 182

  KriefS.Inglesias-GonzalezA.AppenzellerB.OkimatJ.FiniJ.-B.DemeneixB.et al (2020). Road impact in a protected area with rich biodiversity: the case of the Sebitoli road in Kibale National Park, Uganda.Env. Sci. Pollut. Res. Int.2727914–27925. 10.1007/s11356-020-09098-0

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 183

  KudoH.TsuneyoshiY.NagaeM.AdachiS.YamauchiK.UedaH.et al (1994). Detection of thyroid hormone receptors in the olfactory system and brain of wild masu salmon, Oncorhynchus masou (Brevoort), during smolting by in vitro autoradiography.Aquac. Res.25171–181. 10.1111/are.1994.25.s2.171

  • CrossRef
  • Google Scholar

• 184

  KulkarniS. S.BuchholzD. R. (2012). Beyond synergy: Corticosterone and thyroid hormone have numerous interaction effects on gene regulation in Xenopus tropicalis tadpoles.Endocrinology1535309–5324. 10.1210/en.2012-1432

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 185

  KulkarniS. S.BuchholzD. R. (2014). Corticosteroid signaling in frog metamorphosis.Gen. Comp. Endocrinol.203225–231. 10.1016/j.ygcen.2014.03.036

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 186

  KulkarniS. S.DenverR. J.Gomez-MestreI.BuchholzD. R. (2017). Genetic accommodation via modified endocrine signalling explains phenotypic divergence among spadefoot toad species.Nat. Commun.81–6. 10.1038/s41467-017-00996-5

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 187

  KulkarniS.BuchholzD. (2013). Developmental programs and endocrine disruption in frog metamorphosis: the perspective from microarray analysis.Curr. Top. Dev. Biol.103329–364. 10.1016/B978-0-12-385979-2.00012-5

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 188

  KwokA. H. Y.WangY.WangC. Y.LeungF. C. (2007). Cloning of chicken glucocorticoid receptor (GR) and characterization of its expression in pituitary and extrapituitary tissues.Poult. Sci.86423–430. 10.1093/ps/86.2.423

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 189

  LafontA.HardmanL.DirksR.von den ThillartG.TomkiewiczJ.DufourS. (2014). “Characterization and regulation during reproduction of four nuclear corticosteroid receptors in the European eel, Anguilla anguilla,” in Proceedings of the 10th International Symposium on Reproductive Physiology of Fish, olhão.

  • Google Scholar

• 190

  LamersW. H.MoorenP. G.GriepH.EndertE.DegenhartH. J.CharlesR. (1986). Hormones in perinatal rat and spiny mouse: relation to altricial and precocial timing of birth.Am. J. Physiol. Endocrinol. Metab.251E78–E85. 10.1152/ajpendo.1986.251.1.e78

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 191

  LangdonJ. S.ThorpeJ. E.RobertsR. J. (1984). Effects of cortisol and acth on gill Na+/K+-ATPase, SDH and chloride cells in juvenile atlantic salmon Salmo salar L.Comp. Biochem. Physiol. Part A Physiol.779–12. 10.1016/0300-9629(84)90004-5

  • CrossRef
  • Google Scholar

• 192

  LanghorneP.SimpsonT. (1981). “Natural changes in serum cortisol in Atlantic salmon (Salmo salar L.) during parr-smolt transformation,” in Stress and Fish, ed.PickeringA. (Cambridge, MA: Academic Press), 349–350.

  • Google Scholar

• 193

  LanghorneP.SimpsonT. H. (1986). The interrelationship of cortisol, Gill (Na + K) ATPase, and homeostasis during the Parr-Smolt transformation of atlantic salmon (Salmo salar L.).Gen. Comp. Endocrinol.61203–213. 10.1016/0016-6480(86)90198-X

  • CrossRef
  • Google Scholar

• 194

  LazcanoI.OrozcoA. (2018). Revisiting available knowledge on teleostean thyroid hormone receptors.Gen. Comp. Endocrinol.265128–132. 10.1016/j.ygcen.2018.03.022

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 195

  Le RoyA.SeebacherF. (2020). Mismatched light and temperature cues disrupt locomotion and energetics via thyroid-dependent mechanisms.Conserv. Physiol.81–11. 10.1093/conphys/coaa051

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 196

  LeeS.JiK.ChoiK. (2014). Effects of water temperature on perchlorate toxicity to the thyroid and reproductive system of Oryzias latipes.Ecotoxicol. Environ. Saf.108311–317. 10.1016/j.ecoenv.2014.07.016

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 197

  LeemansM.CouderqS.DemeneixB.FiniJ. B. (2019). Pesticides with potential thyroid hormone-disrupting effects: a review of recent data.Front. Endocrinol. (Lausanne)10:743. 10.3389/fendo.2019.00743

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 198

  LeloupI.BuscagliaM.de LuzeA. (1981). [Modulation of T4 to T3 conversion. Comparative aspects (author’s transl)].Ann. Endocrinol. (Paris)42454–460.

  • Google Scholar

• 199

  LeloupJ.BuscagliaM. (1977). Triiodothyronine, hormone of amphibian metamorphosis.Comptes Rendus Hebd. Des Seances L Acad. Des Sci. Ser. D2842261–2263.

  • Google Scholar

• 200

  LemaS. C.ChowM. I.ResnerE. J.WestmanA. A.MayD.DittmanA. H.et al (2016). Endocrine and metabolic impacts of warming aquatic habitats: Differential responses between recently isolated populations of a eurythermal desert pupfish.Conserv. Physiol.41–17. 10.1093/conphys/cow047

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 201

  LiX.LiZ.DengY.ZhangJ.LiJ.WangY. (2020). Characterization of a novel thyrotropin-releasing hormone receptor, TRHR3, in chickens.Poult. Sci.991643–1654. 10.1016/j.psj.2019.10.062

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 202

  LienS.KoopB. F.SandveS. R.MillerJ. R.KentM. P.NomeT.et al (2016). The Atlantic salmon genome provides insights into rediploidization.Nature533200–205. 10.1038/nature17164

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 203

  LigginsG. C. (1968). Premature parturition after infusion of corticotrophin or cortisol into foetal lambs.J. Endocrinol.42323–329. 10.1677/joe.0.0420323

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 204

  LigginsG. C. (1969). Premature delivery of foetal lambs infused with glucocorticoids.J. Endocrinol.45515–523. 10.1677/joe.0.0450515

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 205

  LigginsG.SchellenbergJ.-C.ManzalM.KittermanJ. A.LeeC.-C. (1988). Synergism of cortisol and thyrotropin-releasing hormone in lung maturation in fetal sheep.J. Appl. Physiol.651880–1884.

  • Google Scholar

• 206

  LimaA.FerreiraL.SilvaD.GomesF.TitonS. (2020). Thermal sensitivity of Bullfrog’s immune response kept at different temperatures.J. Exp. Zool. A Ecol. Integr. Physiol.333767–778. 10.1002/jez.2436

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 207

  LittleA. G. (2021). Thyroid hormone regulation of thermal acclimation in ectotherms: physiological mechanisms and ecoevolutionary implications.Mol. Cell. Endocrinol.530:111285. 10.1016/j.mce.2021.111285

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 208

  LittleA. G.KunisueT.KannanK.SeebacherF. (2013). Thyroid hormone actions are temperature-specific and regulate thermal acclimation in zebrafish (Danio rerio).BMC Biol.11:26. 10.1186/1741-7007-11-26

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 209

  LittleA. G.LoughlandI.SeebacherF. (2020). What do warming waters mean for fish physiology and fisheries?J. Fish Biol.97328–340. 10.1111/jfb.14402

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 210

  LittleA.SeebacherF. (2014). Thyroid hormone regulates cardiac performance during cold acclimation in zebrafish (Danio rerio).J. Exp. Biol.217718–725. 10.1242/jeb.096602

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 211

  LoganD. W.Bryson-RichardsonR. J.PagánK. E.TaylorM. S.CurrieP. D.JacksonI. J. (2003). The structure and evolution of the melanocortin and MCH receptors in fish and mammals.Genomics81184–191. 10.1016/S0888-7543(02)00037-X

  • CrossRef
  • Google Scholar

• 212

  LorgenM.CasadeiE.KrólE.DouglasA.BirnieM. J.EbbessonL. O. E.et al (2015). Functional divergence of type 2 deiodinase paralogs in the Atlantic salmon.Curr. Biol.25936–941. 10.1016/j.cub.2015.01.074

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 213

  LovejoyD. A.BalmentR. J. (1999). Evolution and physiology of corticotropin-releasing factor (CRF) family of neuropeptides in vertebrates.Gen. Comp.Endocrinol.1151–22.

  • Google Scholar

• 214

  LovejoyD. A.ChangB. S. W.LovejoyN. R.del CastilloJ. (2014). Molecular evolution of GPCRs: CRH/CRH receptors.J. Mol. Endocrinol.52T46–T60. 10.1530/JME-13-0238

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 215

  Luzeena RajaG.Divya SubhashreeK.LiteC.SantoshW.BarathiS. (2019). Transient exposure of methylparaben to zebrafish (Danio rerio) embryos altered cortisol level, acetylcholinesterase activity and induced anxiety-like behaviour.Gen. Comp. Endocrinol.27953–59. 10.1016/j.ygcen.2018.11.001

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 216

  MadsenS. S. (1990). The role of cortisol and growth hormone in seawater adaptation and development of hypoosmoregulatory mechanisms in sea trout parr (Salmo trutta trutta).Gen. Comp. Endocrinol.791–11. 10.1016/0016-6480(90)90082-W

  • CrossRef
  • Google Scholar

• 217

  ManchadoM.InfanteC.RebordinosL.CañavateJ. P. (2009). Molecular characterization, gene expression and transcriptional regulation of thyroid hormone receptors in Senegalese sole.Gen. Comp. Endocrinol.160139–147. 10.1016/j.ygcen.2008.11.001

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 218

  MännistöT.MendolaP.ReddyU.LaughonS. K. (2013). Neonatal outcomes and birth weight in pregnancies complicated by maternal thyroid disease.Am. J. Epidemiol.178731–740. 10.1093/aje/kwt031

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 219

  MarchandO.DuffraisseM.TriqueneauxG.SafiR.LaudetV. (2004). Molecular cloning and developmental expression patterns of thyroid hormone receptors and T3 target genes in the turbot (Scophtalmus maximus) during post-embryonic development.Gen. Comp. Endocrinol.135345–357. 10.1016/j.ygcen.2003.10.012

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 220

  MarchandO.SafiR.EscrivaH.Van RompaeyE.PrunetP.LaudetV. (2001). Molecular cloning and characterization of thyroid hormone receptors in teleost fish.J. Mol. Endocrinol.2651–65. 10.1677/jme.0.0260051

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 221

  MarieC. (1981). Ontogenesis of the adrenal glucocorticoids and of the target function of the enzymatic tyrosine transaminase activity in the chick embryo.J. Endocrinol.90193–200.

  • Google Scholar

• 222

  MashalyM. M. (1991). Effect of exogenous corticosterone on chicken embryonic development.Poult. Sci.70371–374. 10.3382/ps.0700371

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 223

  MaugarsG.DufourS.Cohen-TannoudjiJ. L.QuératB. (2014). Multiple thyrotropin b-subunit and thyrotropin receptor-related genes arose during vertebrate evolution.PLoS One9:e111361. 10.1371/journal.pone.0111361

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 224

  MaugarsG.MauvoisX.RousseauK.DufourS. (2016). “Evolution of the corticotropin-releasing hormone paralogs in teleosts,” in Proceedings of the 8th International Symposium on Fish Endocrinology, Gothenburg.

  • Google Scholar

• 225

  MazuraisD.DucouretB.TujagueM.ValotaireY.D’CottaH.GallaisC.et al (1998). Regulation of the glucocorticoid receptor mRNA levels in the gills of Atlantic salmon (Salmo salar) during smoltification.Bull. Fr. Pêche Piscic.350–351499–510.

  • Google Scholar

• 226

  McBrideJ.HiggsD.FagerlundU.BuckleyJ. (1982). Thyroid hormones and steroid hormones: potential for control of growth and smoltification of salmonids.Aquaculture28201–210.

  • Google Scholar

• 227

  McCormickS. D. (2001). Endocrine control of osmoregulation in teleost fish.Am. Zool.41781–794. 10.1093/icb/41.4.781

  • CrossRef
  • Google Scholar

• 228

  McCormickS. D. (2012). Smolt physiology and endocrinology.Fish Physiol.32199–251. 10.1016/B978-0-12-396951-4.00005-0

  • CrossRef
  • Google Scholar

• 229

  McCormickS. D.DickhoffW. W.DustonJ.NishiokaR. S.BernH. A. (1991). Developmental differences in the responsiveness of gill Na+, K+-ATPase to cortisol in salmonids.Gen. Comp. Endocrinol.84308–317. 10.1016/0016-6480(91)90054-A

  • CrossRef
  • Google Scholar

• 230

  McCormickS. D.LernerD. T.MonetteM. Y.Nieves-PuigdollerK.KellyJ. T.BjörnssonB. T. (2009). Taking it with you when you go: how perturbations to the freshwater environment, including temperature, dams, and contaminants, affect marine survival of salmon.Am. Fish. Soc. Symp.69195–214.

  • Google Scholar

• 231

  McCormickS. D.RegishA.O’DeaM. F.ShrimptonJ. M. (2008). Are we missing a mineralocorticoid in teleost fish? Effects of cortisol, deoxycorticosterone and aldosterone on osmoregulation, gill Na+,K+-ATPase activity and isoform mRNA levels in Atlantic salmon.Gen. Comp. Endocrinol.15735–40. 10.1016/j.ygcen.2008.03.024

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 232

  McGlashanJ. K.ThompsonM. B.Van DykeJ. U.SpencerR. J. (2017). Thyroid hormones reduce incubation period without developmental or metabolic costs in murray river short-necked turtles (Emydura macquarii).Physiol. Biochem. Zool.9034–46. 10.1086/689744

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 233

  McLeanM.BisitsA.DaviesJ.WoodsR.LowryP.SmithR. (1995). A placental clock controlling the length of human pregnancy.Nat. Med.1460–463. 10.1038/nm0595-460

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 234

  McLeeseJ. M.JohnssonJ.HuntleyT. F. M.ClarkeW. C.WeisbartM. (1994). Seasonal changes in osmoregulation, cortisol, and cortisol receptor activity in the gills of parr/smolt of steelhead trout and steelhead-rainbow trout hybrids, Oncorhynchus mykiss.Gen. Comp. Endocrinol.93103–113. 10.1006/gcen.1994.1012

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 235

  McNabbF. M. A. (2006). Avian thyroid development and adaptive plasticity.Gen. Comp. Endocrinol.14793–101. 10.1016/j.ygcen.2005.12.011

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 236

  McNabbF. M. A.StantonF. W.DickenS. G. (1984). Post-hatching thyroid development and body growth in precocial vs altricial birds.Comp. Biochem. Physiol. Part A Physiol.78629–635. 10.1016/0300-9629(84)90609-1

  • CrossRef
  • Google Scholar

• 237

  MedlerK. F.LanceV. A. (1998). Sex differences in plasma corticosterone levels in alligator (Alligator mississippiensis) embryos.J. Exp. Zool.280238–244.

  • Google Scholar

• 238

  MekuchiM.SaitoY.AokiY.MasudaT.IigoM.YanagisawaT. (2011). Molecular cloning, gene structure, molecular evolution and expression analyses of thyrotropin-releasing hormone receptors from medaka (Oryzias latipes).Gen. Comp. Endocrinol.170374–380. 10.1016/j.ygcen.2010.10.013

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 239

  MetzJ. R.GevenE. J. W.Van Den BurgE. H.FlikG. (2005). ACTH, α-MSH, and control of cortisol release: cloning, sequencing, and functional expression of the melanocortin-2 and melanocortin-5 receptor in Cyprinus carpio.Am. J. Physiol. Regul. Integr. Comp. Physiol.289814–826. 10.1152/ajpregu.00826.2004

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 240

  MeyerA.SchartlM. (1999). Gene and genome duplications in vertebrates: the one-to-four (-to-eight in fish) rule and the evolution of novel gene functions.Curr. Opin. Cell Biol.11699–704. 10.1016/S0955-0674(99)00039-3

  • CrossRef
  • Google Scholar

• 241

  MirandaL. A.AffanniJ. M.PazD. A. (2000). Corticotropin-releasing factor accelerates metamorphosis in Bufo arenarum: effect on pituitary ACTH and TSH cells.J. Exp. Zool.286473–480.

  • Google Scholar

• 242

  MiwaS.InuiY. (1983). Effects of thyroxine and thiourea on the parr-smolt transformation of amago salmon (Oncorhynchus rhodurus).Bull. Natl. Res. Inst. Aquac.441–52.

  • Google Scholar

• 243

  MiwaS.InuiY. (1985). Effects of l-thyroxine and ovine growth hormone on smoltification of amago salmon (Oncorhynchus rhodurus).Gen. Comp. Endocrinol.58436–442. 10.1016/0016-6480(85)90116-9

  • CrossRef
  • Google Scholar

• 244

  MiwaS.InuiY. (1987). Effects of various doses of thyroxine and triiodothyronine on the metamorphosis of flounder (Paralichthys olivaceus).Gen. Comp. Endocrinol.67356–363. 10.1016/0016-6480(87)90190-0

  • CrossRef
  • Google Scholar

• 245

  MiwaS.TagawaM.InuiY.HiranoT. (1988). Thyroxine surge in metamorphosing flounder larvae.Gen. Comp. Endocrinol.70158–163. 10.1016/0016-6480(88)90105-0

  • CrossRef
  • Google Scholar

• 246

  MizunoS.UraK.OnoderaY.FukadaH.MisakaN.HaraA.et al (2001). Changes in transcript levels of gill cortisol receptor during smoltification in Wild Masu Salmon, Oncorhynchus masou.Zool. Sci.18853–860. 10.2108/zsj.18.853

  • CrossRef
  • Google Scholar

• 247

  MommsenT. P.VijayanM. M.MoonT. W. (1999). Cortisol in teleosts: dynamics, mechanisms of action, and metabolic regulation.Rev. Fish Biol. Fish.9211–268. 10.1023/A:1008924418720

  • CrossRef
  • Google Scholar

• 248

  MooreC. S.CristolD. A.MadduxS. L.Varian-RamosC. W.BradleyE. L. (2014). Lifelong exposure to methylmercury disrupts stress-induced corticosterone response in zebra finches (Taeniopygia guttata).Environ. Toxicol. Chem.331072–1076. 10.1002/etc.2521

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 249

  MoreiraL.DiamanteG.GirouxM.CoffinS.XuE.Moledo de Souza AbessaD.et al (2018). Impacts of salinity and temperature on the thyroidogenic effects of the biocide diuron in Menidia beryllina.Env. Sci. Technol.523146–3155. 10.1021/acs.est.7b04970

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 250

  MulayS.GiannopoulosG.SolomonS. (1973). Corticosteroid levels in mother an dfetus of the rabbit during gestation.Endocrinology931342–1348.

  • Google Scholar

• 251

  NagaeM.FudaH.HaraA.SaneyoshiM.YamauchiK. (1994). Changes in serum concentrations of immunoglobulin M (IgM), cortisol and thyroxine (T4) during Smoltification in the Masu Salmon Oncorhynchus masou.Fish. Sci.60241–242. 10.2331/fishsci.60.241

  • CrossRef
  • Google Scholar

• 252

  NakaneY.YoshimuraT. (2019). Photoperiodic regulation of reproduction in vertebrates.Annu. Rev. Anim. Biosci.7173–194.

  • Google Scholar

• 253

  NakanoM.HasunumaI.MinagawaA.IwamuroS.YamamotoK.KikuyamaS.et al (2018). Possible involvement of thyrotropin-releasing hormone receptor 3 in the release of prolactin in the metamorphosing bullfrog larvae.Gen. Comp. Endocrinol.26736–44. 10.1016/j.ygcen.2018.05.029

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 254

  NisenbaumL.MartinP.FuentesM.BesseauL.MagnanouE.McCormickS.et al (2020). Effects of a temperature rise on melatonin and thyroid hormones during smoltification of Atlantic salmon, Salmo salar.J. Comp. Physiol. B190731–748. 10.1007/s00360-020-01304-2

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 255

  O’ShaughnessyK. L.GilbertM. E. (2020). Thyroid disrupting chemicals and developmental neurotoxicity – new tools and approaches to evaluate hormone action.Mol. Cell. Endocrinol.518:110663. 10.1016/j.mce.2019.110663

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 256

  OlivereauM. (1975). Histophysiologie de l’axe hypophyso-corticosurrenalien chez le saumon de l’Atlantique (Cycle en eau douce, vie thalassique et reproduction).Gen. Comp. Endocrinol.279–27.

  • Google Scholar

• 257

  OlsonJ. M.McNabbF. M. A.JablonskiM. S.FerrisD. V. (1999). Thyroid development in relation to the development of endothermy in the red-winged blackbird (Agelaius phoeniceus).Gen. Comp. Endocrinol.116204–212. 10.1006/gcen.1999.7363

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 258

  OnJ. S. W.ArokiarajA. W. R.ChowB. K. C. (2019). Molecular evolution of CRH and CRHR subfamily before the evolutionary origin of vertebrate.Peptides120:170087. 10.1016/j.peptides.2019.04.014

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 259

  OrozcoA.Valverde-RC. (2005). Thyroid hormone deiodination in fish.Thyroid15799–813. 10.1089/thy.2005.15.799

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 260

  OrozcoA.ValverdeR. C.OlveraA.GarcíaG. C. (2012). Iodothyronine deiodinases: a functional and evolutionary perspective.J. Endocrinol.215207–219. 10.1530/JOE-12-0258

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 261

  Ortiz-SantaliestraM.MarcoA. (2015). Influence of dissolved oxygen conditions on toxicity of ammonium nitrate to larval natterjack toads.Arch. Env. Contam. Toxicol.6995–103. 10.1007/s00244-014-0126-3

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 262

  OrtonF.TylerC. R. (2015). Do hormone-modulating chemicals impact on reproduction and development of wild amphibians?Biol. Rev.901100–1117. 10.1111/brv.12147

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 263

  OwensD.MorrisY. (1985). The comparative endocrinology of sea turtles.Copeia3723–735.

  • Google Scholar

• 264

  ParisM.LaudetV. (2008). The history of a developmental stage: metamorphosis in chordates.Genesis46657–672. 10.1002/dvg.20443

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 265

  ParisiC.GuerrieroG. (2019). Antioxidative defense and fertility rate in the assessment of reprotoxicity risk posed by global warming.Antioxidants8:622. 10.3390/antiox8120622

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 266

  ParkD.FreelK. L.DanielsK. D.PropperC. R. (2016). Interactions between a small chronic increase in diel water temperature and exposure to a common environmental contaminant on development of Arizona tiger salamander larvae.Gen. Comp. Endocrinol.23869–77. 10.1016/j.ygcen.2016.06.021

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 267

  PatelJ.LandersK.LiH.MortimerR. H.RichardK. (2011). Thyroid hormones and fetal neurological development.J. Endocrinol.2091–8. 10.1530/JOE-10-0444

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 268

  PetrovićT. G.KijanovićA.TomaševićN. K.GavrićJ. P.DespotovićS. G.GavrilovićB. R.et al (2021). Effects of desiccation on metamorphic climax in Bombina variegata: changes in levels and patterns of oxidative stress parameters.Animals11:953. 10.3390/ani11040953

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 269

  PinskyM.EikesetA.McCauleyD.PayneJ.SundayJ. (2019). Greater vulnerability to warming of marine versus terrestrial ectotherms.Nature569108–111. 10.1038/s41586-019-1132-4

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 270

  PorterT. E.GhavamS.MuchowM.BossisI.EllestadL. (2007). Cloning of partial cDNAs for the chicken glucocorticoid and mineralocorticoid receptors and characterization of mRNA levels in the anterior pituitary gland during chick embryonic development.Domest. Anim. Endocrinol.33226–239. 10.1016/j.domaniend.2006.05.006

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 271

  PottingerT. G. (2017). Modulation of the stress response in wild fish is associated with variation in dissolved nitrate and nitrite.Environ. Pollut.225550–558. 10.1016/j.envpol.2017.03.021

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 272

  PréauL.FiniJ. B.Morvan-DuboisG.DemeneixB. (2015). Thyroid hormone signaling during early neurogenesis and its significance as a vulnerable window for endocrine disruption.Biochim. Biophys. Acta Gene Regul. Mech.1849112–121. 10.1016/j.bbagrm.2014.06.015

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 273

  PremdasF.EalesJ. (1976). The influence of TSH and ACTH on purine and pteridine deposition in the skin of rainbow trout (Salmo gairdneri).Can. J. Zool.54576–581.

  • Google Scholar

• 274

  QuanJ.KangY.LuoZ.ZhaoG.MaF.LiL.et al (2020). Identification and characterization of long noncoding RNAs provide insight into the regulation of gene expression in response to heat stress in rainbow trout (Oncorhynchus mykiss).Comp. Biochem. Physiol. Part D Genomics Proteomics36:100707. 10.1016/j.cbd.2020.100707

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 275

  RacicA.TylanC.LangkildeT. (2020). Effects of temperature on plasma corticosterone in a native lizard.Sci. Rep.101–8. 10.1038/s41598-020-73354-z

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 276

  RadchukV.ReedT.TeplitskyC.van de PolM.CharmantierA.HassallC.et al (2019). Adaptive responses of animals to climate change are most likely insufficient.Nat. Commun.101–14. 10.1038/s41467-019-10924-4

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 277

  RaineJ. C.CameronC.VijayanM. M.MacKenzieD. S.LeatherlandJ. F. (2005). Effect of fasting on thyroid hormone levels, and TRα and TRβ mRNA accumulation in late-stage embryo and juvenile rainbow trout, Oncorhynchus mykiss.Comp. Biochem. Physiol. A Mol. Integr. Physiol.140452–459. 10.1016/j.cbpb.2005.02.007

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 278

  RanjanM.WongJ.ShiY. B. (1994). Transcriptional repression of Xenopus TRβ gene is mediated by a thyroid hormone response element located near the start site.J. Biol. Chem.26924699–24705. 10.1016/s0021-9258(17)31447-3

  • CrossRef
  • Google Scholar

• 279

  ReddingJ. M.PatiñoR.SchreckC. B. (1991). Cortisol effects on plasma electrolytes and thyroid hormones during smoltification in coho salmon Oncorhynchus kisutch.Gen. Comp. Endocrinol.81373–382. 10.1016/0016-6480(91)90164-2

  • CrossRef
  • Google Scholar

• 280

  ReddyP. K.LamT. J. (1991). Effect of thyroid hormones on hatching in the tilapia, Oreochromis mossambicus.Gen. Comp. Endocrinol.81484–491.

  • Google Scholar

• 281

  ReynsG. E.VenkenK.Morreale De EscobarG.KühnE. R.DarrasV. M. (2003). Dynamics and regulation of intracellular thyroid hormone concentrations in embryonic chicken liver, kidney, brain, and blood.Gen. Comp. Endocrinol.13480–87. 10.1016/S0016-6480(03)00220-X

  • CrossRef
  • Google Scholar

• 282

  RichmanN. H.Tai de DiazS.NishiokaR. S.PrunetP.BernH. A. (1987). Osmoregulatory and endocrine relationships with chloride cell morphology and density during smoltification in coho salmon (Oncorhynchus kisutch).Aquaculture60265–285. 10.1016/0044-8486(87)90293-6

  • CrossRef
  • Google Scholar

• 283

  RobertsonO. (1949). Production of silvery smolt stage in rainbow trout by intramuscular injection of mammalian thyroid extract and thyrotropic hormone.J. Exp. Zool.110337–355.

  • Google Scholar

• 284

  RomanoffA.LauferH. (1956). The effect of injected thiourea on the development of some organs of the chick embryo.Endocrinology59611–619. 10.1210/endo-59-6-611

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 285

  RondeauE. B.MinkleyD. R.LeongJ. S.MessmerA. M.JantzenJ. R.Von SchalburgK. R.et al (2014). The genome and linkage map of the northern pike (Esox lucius): conserved synteny revealed between the salmonid sister group and the neoteleostei.PLoS One9:e102089. 10.1371/journal.pone.0102089

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 286

  RousseauJ. P.Buteau-PoulinA.KinkeadR. (2019). Maternal thyroid hormone deficiency and cardiorespiratory disorder in rat pups.Exp. Neurol.320:112960. 10.1016/j.expneurol.2019.112960

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 287

  RousseauK.MartinP.BoeufG.DufourS. (2012). “Salmonid secondary metamorphosis: smoltification,” in Metamorphosis in Fish, edsDufourS.RousseauK.KapporB. (St Helier: Science Publishers), 167–215.

  • Google Scholar

• 288

  RouttiH.AtwoodT. C.BechshoftT.BoltunovA.CiesielskiT. M.DesforgesJ. P.et al (2019). State of knowledge on current exposure, fate and potential health effects of contaminants in polar bears from the circumpolar Arctic.Sci. Total Environ.6641063–1083. 10.1016/j.scitotenv.2019.02.030

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 289

  RuboliniD.RomanoM.BoncoraglioG.FerrariR. P.MartinelliR.GaleottiP.et al (2005). Effects of elevated egg corticosterone levels on behavior, growth, and immunity of yellow-legged gull (Larus michahellis) chicks.Horm. Behav.47592–605. 10.1016/j.yhbeh.2005.01.006

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 290

  RupikW. (2011). Structural and ultrastructural differentiation of the thyroid gland during embryogenesis in the grass snake Natrix natrix L. (Lepidosauria, Serpentes).Zoology114284–297. 10.1016/j.zool.2011.05.002

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 291

  RuthsatzK.DausmannK. H.DreesC.BeckerL. I.HartmannL.ReeseJ.et al (2020). Altered thyroid hormone levels affect the capacity for temperature-induced developmental plasticity in larvae of Rana temporaria and Xenopus laevis.J. Therm. Biol.90:102599. 10.1016/j.jtherbio.2020.102599

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 292

  RuuskanenS.GroothuisT. G. G.SchaperS. V.DarrasV. M.de VriesB.VisserM. E. (2016). Temperature-induced variation in yolk androgen and thyroid hormone levels in avian eggs.Gen. Comp. Endocrinol.23529–37. 10.1016/j.ygcen.2016.05.026

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 293

  RuuskanenS.HsuB. Y.NordA. (2021). Endocrinology of thermoregulation in birds in a changing climate.Mol. Cell. Endocrinol.519:111088. 10.1016/j.mce.2020.111088

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 294

  SachsL. M.BuchholzD. R. (2017). Frogs model man: in vivo thyroid hormone signaling during development.Genesis55e23000. 10.1002/dvg.23000

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 295

  SachsL. M.BuchholzD. R. (2019). Insufficiency of thyroid hormone in frog metamorphosis and the role of glucocorticoids.Front. Endocrinol. (Lausanne)10:287. 10.3389/fendo.2019.00287

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 296

  SachsL.DamjanovskiS.JonesP.LiQ.AmanoT.UedaS.et al (2000). Dual functions of thyroid hormone receptors during Xenopus development.Comp. Biochem. Physiol. B Biochem. Mol. Biol.126199–211.

  • Google Scholar

• 297

  SaffranM.SchallyA.BenfeyB. (1955). Stimulation of the release of corticotropin from the adenohypophysis by a neurohypophysial factor.Endocrinology57439–444.

  • Google Scholar

• 298

  SainoN.RomanoM.FerrariR. P.MartinelliR.MøllerA. P. (2005). Stressed mothers lay eggs with high corticosterone levels which produce low-quality offspring.J. Exp. Zool. Part A Comp. Exp. Biol.303998–1006. 10.1002/jez.a.224

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 299

  SaitoY.MekuchiM.KobayashiN.KimuraM.AokiY.MasudaT.et al (2011). Molecular cloning, molecular evolution and gene expression of cDNAs encoding thyrotropin-releasing hormone receptor subtypes in a teleost, the sockeye salmon (Oncorhynchus nerka).Gen. Comp. Endocrinol.17480–88. 10.1016/j.ygcen.2011.07.011

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 300

  SalisP.RouxN.HuangD.MarcionettiA.MouginotP.ReynaudM.et al (2021). Thyroid hormones regulate the formation and environmental plasticity of white bars in clownfishes.Proc. Natl. Acad. Sci. U.S.A.1181–9. 10.1073/pnas.2101634118

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 301

  SangildP. T.FowdenA. L.TrahairJ. F. (2000). How does the foetal gastrointestinal tract develop in preparation for enteral nutrition after birth?Livest. Prod. Sci.66141–150. 10.1016/S0301-6226(00)00221-9

  • CrossRef
  • Google Scholar

• 302

  SapJ.MuñozA.DammK.GoldbergY.GhysdaelJ.LeutzA.et al (1986). The c-erb-A protein is a high-affinity receptor for thyroid hormone.Nature324635–640. 10.1038/324635a0

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 303

  SarraudeT.HsuB. Y.GroothuisT.RuuskanenS. (2020). Testing the short-and long-term effects of elevated prenatal exposure to different forms of thyroid hormones.PeerJ81–25. 10.7717/peerj.10175

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 304

  SaundersR. L.McCormickS. D.HendersonE. B.EalesJ. G.JohnstonC. E. (1985). The effect of orally administered 3,5,3′-triiodo-L-thyronine on growth and salinity tolerance of Atlantic salmon (Salmo salar L.).Aquaculture45143–156. 10.1016/0044-8486(85)90265-0

  • CrossRef
  • Google Scholar

• 305

  SchaafM. J. M.ChampagneD.Van LaanenI. H. C.Van WijkD. C. W. A.MeijerA. H.MeijerO. C.et al (2008). Discovery of a functional glucocorticoid receptor β-isoform in zebrafish.Endocrinology1491591–1598. 10.1210/en.2007-1364

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 306

  SchellenbergJ.LigginsG.ManzaiM.KittermanJ.LeeC. (1988). Synergistic hormonal effects on lung maturation in fetal sheep.J. Appl. Physiol.6594–100.

  • Google Scholar

• 307

  SchmidtJ.AndreeR.DavisK.TreeseS.SatterleeD. (2009). Influence of maternal corticosterone treatment on incubation length of eggs laid by Japanese quail hens selected for divergent adrenocortical stress responsiveness.Br. Poult. Sci.50739–747. 10.1080/00071660903317571

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 308

  SchreiberA. M.SpeckerJ. L. (1998). Metamorphosis in the summer flounder, Paralichthys dentatus: stage-specific developmental response to altered thyroid status.Gen. Comp. Endocrinol.111156–166.

  • Google Scholar

• 309

  SchreiberV.EckertovaA.FrancZ.KociJ.RybakM.KmentovaV. (1961). Effect of a fraction of bovine hypothalamic extract on the release of TSH by rat adenohypophyses in vitro.Experientia17264–265.

  • Google Scholar

• 310

  SchriksM.van der LindenS. C.StoksP. G. M.van der BurgB.PuijkerL.de VoogtP.et al (2013). Occurrence of glucocorticogenic activity in various surface waters in The Netherlands.Chemosphere93450–454. 10.1016/j.chemosphere.2013.04.091

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 311

  ScottT. R.JohnsonW. A.SatterleeD. G.GildersleeveR. P. (1981). Circulating levels of corticosterone in the serum of developing chick embryos and newly hatched chicks.Poult. Sci.601314–1320. 10.3382/ps.0601314

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 312

  ShepherdleyC. A.DanielsC. B.OrgeigS.RichardsonS. J.EvansB. K.DarrasV. M. (2002). Glucocorticoids, thyroid hormones, and iodothyronine deiodinases in embryonic saltwater crocodiles.Am. J. Physiol. Regul. Integr. Comp. Physiol.2831155–1163. 10.1152/ajpregu.00015.2002

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 313

  ShiY. B. (2021). Life without thyroid hormone receptor.Endocrinology (United States)1621–12. 10.1210/endocr/bqab028

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 314

  ShiY. B.LiangV. C. T.ParkisonC.ChengS. Y. (1994). Tissue-dependent developmental expression of a cytosolic thyroid hormone protein gene in Xenopus: its role in the regulation of amphibian metamorphosis.FEBS Lett.35561–64. 10.1016/0014-5793(94)01173-7

  • CrossRef
  • Google Scholar

• 315

  ShibataY.TanizakiY.ZhangH.LeeH.DassoM.ShiY. B. (2021). Thyroid hormone receptor is essential for larval epithelial apoptosis and adult epithelial stem cell development but not adult intestinal morphogenesis during Xenopus tropicalis metamorphosis.Cells10:536. 10.3390/cells10030536

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 316

  ShibataY.WenL.OkadaM.ShiY. (2020). Organ-specific requirements for thyroid hormone receptor ensure temporal coordination of tissue-specific transformations and completion of Xenopus Metamorphosis.Thyroid30300–313. 10.1089/thy.2019.0366

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 317

  ShibusawaK.SaitoS.FukudaM.KawaiT.YoshimuraF. (1955). On the role of the hypothalamic-neurohypophyseal neurosecretion in the liberation of the adenohypophyseal hormines.Endocrinol. Jpn.247–56.

  • Google Scholar

• 318

  ShinH. S.ChoiY. J.KimN. N.LeeJ.UedaH.ChoiC. Y. (2014). Effects of exogenous cortisol and seawater adaptation on thyroid hormone receptors in the smolt stage of the sockeye salmon, Oncorhynchus nerka.Ichthyol. Res.619–16. 10.1007/s10228-013-0365-8

  • CrossRef
  • Google Scholar

• 319

  ShrimptonJ. M. (1996). Relationship between size, gill corticosteroid receptors, Na+-K+ ATPase activity and smolting in juvenile coho salmon (Oncorhynchus kisutch) in autumn and spring.Aquaculture147127–140. 10.1016/S0044-8486(96)01390-7

  • CrossRef
  • Google Scholar

• 320

  ShrimptonJ. M.McCormickS. D. (1998). Seasonal differences in plasma cortisol and gill corticosteroid receptors in upper and lower mode juvenile Atlantic salmon.Aquaculture168205–219. 10.1016/S0044-8486(98)00350-0

  • CrossRef
  • Google Scholar

• 321

  ShrimptonJ. M.McCormickS. D. (1999). Responsiveness of gill Na+/K+-ATPase to cortisol is related to gill corticosteroid receptor concentration in juvenile rainbow trout.J. Exp. Biol.202987–995.

  • Google Scholar

• 322

  ShrimptonJ. M.McCormickS. D. (2003). Environmental and endocrine control of gill corticosteroid receptor number and affinity in Atlantic salmon (Salmo salar) during smolting.Aquaculture22283–99. 10.1016/S0044-8486(03)00104-2

  • CrossRef
  • Google Scholar

• 323

  ShrimptonJ.RandallD. (1994). Downregulation of corticosteroid receptors in gills of coho salmon due to stress and cortisol treatment.Am. J. Physiol. Integr. Comp. Physiol.267R432–R438.

  • Google Scholar

• 324

  SiegelH. S.GouldN. R. (1976). Chick embryonic plasma proteins and binding capacity for corticosterone.Dev. Biol.50510–516. 10.1016/0012-1606(76)90169-X

  • CrossRef
  • Google Scholar

• 325

  SilverM.FowdenA. L. (1989). Pituitary-adrenocortical activity in the fetal pig in the last third of gestation.Q. J. Exp. Physiol.74197–206. 10.1113/expphysiol.1989.sp003255

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 326

  SilverinB.RudasP. (1996). Thyroid hormones in nestling great tits (Parus major).Gen. Comp. Endocrinol.103138–141. 10.1006/gcen.1996.0104

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 327

  SinhaM. D.RingerR. K.ColemanT. H.ZindelH. C. (1959). The effect of injected thiouracil on body weight and hatchability of the chick embryo.Poult. Sci.381405–1409. 10.3382/ps.0381405

  • CrossRef
  • Google Scholar

• 328

  SirakovM.PlaterotiM. (2011). The thyroid hormones and their nuclear receptors in the gut: from developmental biology to cancer.Biochim. Biophys. Acta Mol. Basis Dis.1812938–946. 10.1016/j.bbadis.2010.12.020

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 329

  SirakovM.KressE.NadjarJ.PlaterotiM. (2014). Thyroid hormones and their nuclear receptors: new players in intestinal epithelium stem cell biology?Cell. Mol. Life Sci.712897–2907. 10.1007/s00018-014-1586-3

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 330

  SirsatT. S.DzialowskiE. M. (2020). Manipulating plasma thyroid hormone levels at hatching alters development of endothermy and ventilation in Pekin duck (Anas platyrhynchos domestica).J. Exp. Biol.223(Pt 22):jeb237701. 10.1242/jeb.237701

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 331

  SjöbergM.VennströmB.ForrestD. (1992). Thyroid hormone receptors in chick retinal development: differential expression of mRNAs for α and N-terminal variant β receptors.Development11439–47.

  • Google Scholar

• 332

  SolbakkenJ. S.NorbergB.WatanabeK.PittmanK. (1999). Thyroxine as a mediator of metamorphosis of Atlantic halibut, Hippoglossus hippoglossus.Environ. Biol. Fishes5653–65. 10.1023/a:1007542526040

  • CrossRef
  • Google Scholar

• 333

  SpaanK.HaigisA. C.WeissJ.LegradiJ. (2019). Effects of 25 thyroid hormone disruptors on zebrafish embryos: a literature review of potential biomarkers.Sci. Total Environ.6561238–1249. 10.1016/j.scitotenv.2018.11.071

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 334

  SpeckerJ. L. (1982). Interrenal function and smoltification.Aquaculture2859–66. 10.1016/0044-8486(82)90008-4

  • CrossRef
  • Google Scholar

• 335

  SpeckerJ. L.EalesJ. G.TagawaM.TylerW. A. (2000). Parr-smolt transformation in Atlantic salmon: thyroid hormone deiodination in liver and brain and endocrine correlates of change in rheotactic behavior.Can. J. Zool.78696–705. 10.1139/z99-258

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 336

  SpeckerJ.SchreckC. (1982). Changes in plasma corticosteroids during smoltification of coho salmon Oncorhynchus kisutch.Gen. Comp. Endocrinol.4653–58.

  • Google Scholar

• 337

  SpirhanzlovaP.FiniJ. B.DemeneixB.Lardy-FontanS.Vaslin-ReimannS.LalereB.et al (2019). Composition and endocrine effects of water collected in the Kibale national park in Uganda.Environ. Pollut.251460–468. 10.1016/j.envpol.2019.05.006

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 338

  St. GermainD. L.SchwartzmanR. A.CroteauW.KanamoriA.WangZ.BrownD. D.et al (1994). A thyroid hormone-regulated gene in Xenopus laevis encodes a type III iodothyronine 5-deiodinase.Proc. Natl. Acad. Sci. U.S.A917767–7771. 10.1073/pnas.91.16.7767

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 339

  StarckJ.RicklefsR. (1998). “Patterns of development: the altricial-precocial spectrum,” in Avian Growth And Development, edsStarckJ.RicklefsR. (Oxford: Oxford Univ. Press), 3–30.

  • Google Scholar

• 340

  SteegbornC.SchweizerU. (2020). Structure and mechanism of iodothyronine deiodinases - what we know, what we don’t know, and what would be nice to know.Exp. Clin. Endocrinol. Diabetes128375–378. 10.1055/a-1022-9916

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 341

  StenzelD.HuttnerW. B. (2013). Role of maternal thyroid hormones in the developing neocortex and during human evolution.Front. Neuroanat.7:19. 10.3389/fnana.2013.00019

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 342

  SternerZ. R.ShewadeL. H.MertzK. M.SturgeonS. M.BuchholzD. R. (2020). Glucocorticoid receptor is required for survival through metamorphosis in the frog Xenopus tropicalis.Gen. Comp. Endocrinol.291:113419. 10.1016/j.ygcen.2020.113419

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 343

  SullivanL. C.OrgeigS.DanielsC. B. (2002a). Control of the development of the pulmonary surfactant system in the saltwater crocodile, Crocodylus porosus.Am. J. Physiol. Regul. Integr. Comp. Physiol.2831164–1176. 10.1152/ajpregu.00009.2002

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 344

  SullivanL. C.OrgeigS.DanielsC. B. (2002b). Regulation of pulmonary surfactant secretion in the developing lizard, Pogona vitticeps.Comp. Biochem. Physiol. A Mol. Integr. Physiol.133539–546. 10.1016/S1095-6433(02)00187-3

  • CrossRef
  • Google Scholar

• 345

  SullivanL. C.OrgeigS.WoodP. G.DanielsC. B. (2001). The ontogeny of pulmonary surfactant secretion in the embryonic green sea turtle (Chelonia mydas).Physiol. Biochem. Zool.74493–501. 10.1086/322158

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 346

  SullivanL.OrgeigS.DanielsC. (2003). The role of extrinsic and intrinsic factors in the evolution of the control of pulmonary surfactant maturation during development in the amniotes.Physiol. Biochem. Zool.76281–295.

  • Google Scholar

• 347

  SunB. J.LiT.MuY.McGlashanJ. K.GeorgesA.ShineR.et al (2016). Thyroid hormone modulates offspring sex ratio in a turtle with temperature-dependent sex determination.Proc. R. Soc. B Biol. Sci.283:20161206. 10.1098/rspb.2016.1206

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 348

  SundellH.GrayM.RelierJ.-P.KovarI.CattertonW.SwittL.et al (1979). The effects of ACTH on lung maturation in fetal lambs.Am. J. Pathol.97393–410.

  • Google Scholar

• 349

  SundellK.JutfeltF.ÁgústssonT.OlsenR. E.SandblomE.HansenT.et al (2003). Intestinal transport mechanisms and plasma cortisol levels during normal and out-of-season parr-smolt transformation of Atlantic salmon Salmo salar.Aquaculture222265–285. 10.1016/S0044-8486(03)00127-3

  • CrossRef
  • Google Scholar

• 350

  SundströmG.DreborgS.LarhammarD. (2010). Concomitant duplications of opioid peptide and receptor genes before the origin of jawed vertebrates.PLoS One5:e10512. 10.1371/journal.pone.0010512

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 351

  SuzukiM. R.KikuyamaS. (1983). Corticoids augment nuclear binding capacity for triiodothyronine in bullfrog tadpole tail fins.Gen. Comp. Endocrinol.52272–278. 10.1016/0016-6480(83)90122-3

  • CrossRef
  • Google Scholar

• 352

  SweetingR. M.AlexanderG. P.EalesJ. G.McKeownB. A. (1994). Hepatic and branchial thyroid hormone deiodinase activities associated with the parr-smolt transformation of coho salmon (Oncorhynchus kisutch).Gen. Comp. Endocrinol.94171–181. 10.1006/gcen.1994.1073

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 353

  SzékelyD.CogǎlniceanuD.SzékelyP.Armijos-OjedaD.Espinosa-MogrovejoV.DenoëlM. (2020). How to recover from a bad start: size at metamorphosis affects growth and survival in a tropical amphibian.BMC Ecol.20:24. 10.1186/s12898-020-00291-w

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 354

  TagawaM.MiwaS.InuiiY.de JesusE.HiranoT. (1990). Changes in thyroid hormone concentrations during early development and metamorphosis of the flounder, Paralichthys olivaceus.Zool. Sci.793–96.

  • Google Scholar

• 355

  TailleboisL.KeithP.ValadeP.TorresP.BalocheS.DufourS.et al (2011). Involvement of thyroid hormones in the control of larval metamorphosis in (Teleostei: Gobioidei) at the time of river recruitment.Gen. Comp. Endocrinol.173281–288. 10.1016/j.ygcen.2011.06.008

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 356

  TakeuchiS.TakahashiS. (1998). Melanocortin receptor genes in the chicken–tissue distributions.Gen. Comp. Endocrinol.112220–231. 10.1006/gcen.1998.7167

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 357

  TanabeY. (1982). Ontogenetic aspect of steroidogenesis by gonads and adrenals of ducks and its role on sex differentiation.J. Yamashina Inst. Ornithol.14151–156. 10.3312/jyio1952.14.151

  • CrossRef
  • Google Scholar

• 358

  TanabeY.SaitoN.NakamuraT. (1986). Ontogenetic steroidogenesis by testes, ovary, and adrenals of embryonic and postembryonic chickens (Gallus domesticus).Gen. Comp. Endocrinol.63456–463. 10.1016/0016-6480(86)90146-2

  • CrossRef
  • Google Scholar

• 359

  TanabeY.YanoT.NakamuraT. (1983). Steroid hormone synthesis and secretion by testes, ovary, and adrenals of embryonic and postembryonic ducks.Gen. Comp. Endocrinol.49144–153. 10.1016/0016-6480(83)90018-7

  • CrossRef
  • Google Scholar

• 360

  TanangonanJ. B.TagawaM.TanakaM.HiranoT. (1989). Changes in tissue thyroxine level of metamorphosing japanese flounder Paralichthys olivaceus reared at different temperatures.Nippon Suisan Gakkai.55485–490. 10.2331/suisan.55.485

  • CrossRef
  • Google Scholar

• 361

  TelemecoR. S.AddisE. A. (2014). Temperature has species-specific effects on corticosterone in alligator lizards.Gen. Comp. Endocrinol.206184–192. 10.1016/j.ygcen.2014.07.004

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 362

  ThambirajahA. A.KoideE. M.ImberyJ. J.HelbingC. C. (2019). Contaminant and environmental influences on thyroid hormone action in amphibian metamorphosis.Front. Endocrinol. (Lausanne)10:276. 10.3389/fendo.2019.00276

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 363

  ThompsonC.WeinbergerC.LeboR.EvansR. (1987). Identification of a novel thyroid hormone receptor expressed in the mammalian central nervous system.Science2371610–1614. 10.1126/science.3629259

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 364

  TipsmarkC. K.JørgensenC.Brande-LavridsenN.EngelundM.OlesenJ. H.MadsenS. S. (2009). Effects of cortisol, growth hormone and prolactin on gill claudin expression in Atlantic salmon.Gen. Comp. Endocrinol.163270–277. 10.1016/j.ygcen.2009.04.020

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 365

  TonaK.OnagbesanO.BruggemanV.De SmitL.FigueiredoD.DecuypereE. (2007). Non-ventilation during early incubation in combination with dexamethasone administration during late incubation: 1. Effects on physiological hormone levels, incubation duration and hatching events.Domest. Anim. Endocrinol.3332–46. 10.1016/j.domaniend.2006.04.002

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 366

  TrahairJ. F.PerryR. A.RobinsonP. M. (1987a). Studies on the maturation of the small intestine in the fetal sheep. I. The effects of bilateral adrenalectomy.Q. J. Exp. Physiol.7261–69.

  • Google Scholar

• 367

  TrahairJ. F.PerryR. A.SilverM.RobinsonP. (1987b). Studies on the maturation of the small intestine in the fetal sheep. II. The effects of exogenous cortisol.Q. J. Exp. Physiol.7271–79. 10.1113/expphysiol.1987.sp003056

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 368

  TrahairJ.SangildP. (1997). Systemic and luminal influences on the perinatal development of the gut.Equine Vet. J.2940–50.

  • Google Scholar

• 369

  TrudeauV. L.ThomsonP.ZhangW. S.ReynaudS.Navarro-MartinL.LangloisV. S. (2020). Agrochemicals disrupt multiple endocrine axes in amphibians.Mol. Cell. Endocrinol.513:110861. 10.1016/j.mce.2020.110861

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 370

  TsengC.JohnsonL. (1986). Role of thyroxine in functional gastric development.Am. J. Physiol.251G111–G116.

  • Google Scholar

• 371

  UraK.HaraA.YamauchiK. (1994). Serum thyroid hormone, guanine and protein profiles during smoltification and after thyroxine treatment in the masu salmon, Oncorhynchus masou.Comp. Biochem. Physiol. Part A Physiol.107607–612. 10.1016/0300-9629(94)90359-X

  • CrossRef
  • Google Scholar

• 372

  UsalM.VeyrencS.Darracq–Ghitalla-CiockM.RegnaultC.SrodaS.FiniJ. B.et al (2021). Transgenerational metabolic disorders and reproduction defects induced by benzo[a]pyrene in Xenopus tropicalis.Environ. Pollut.269:116109. 10.1016/j.envpol.2020.116109

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 373

  ValeW.SpiessJ.RivierC.RivierJ. (1981). Characterization of a 41-residue ovine hypothalamic peptide that stimulates secretion of corticotropin and β-endorphin.Science2131394–1397. 10.1097/00006254-198205000-00013

  • CrossRef
  • Google Scholar

• 374

  Van HerckS. L. J.DelbaereJ.BourgeoisN. M. A.McAllanB. M.RichardsonS. J.DarrasV. M. (2015). Expression of thyroid hormone transporters and deiodinases at the brain barriers in the embryonic chicken: insights into the regulation of thyroid hormone availability during neurodevelopment.Gen. Comp. Endocrinol.21430–39. 10.1016/j.ygcen.2015.02.021

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 375

  Van RensburgS. J. (1967). Gestation in sheep after foetal adrenalectomy and cortisol acetate administration.J. Endocrinol.3883–84.

  • Google Scholar

• 376

  Van TuylM.BlommaartP. E.De BoerP. A. J.WertS. E.RuijterJ. M.IslamS.et al (2004). Prenatal exposure to thyroid hormone is necessary for normal postnatal development of murine heart and lungs.Dev. Biol.272104–117. 10.1016/j.ydbio.2004.03.042

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 377

  Vargas-ChacoffL.DannF.PaschkeK.Oyarzún-SalazarR.NualartD.MartínezD.et al (2021). Freshening effect on the osmotic response of the Antarctic spiny plunderfish Harpagifer antarcticus.J. Fish. Biol.981558–1571. 10.1111/jfb.14676

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 378

  VästermarkÅSchiöthH. B. (2011). The early origin of melanocortin receptors, agouti-related peptide, agouti signalling peptide, and melanocortin receptor-accessory proteins, with emphasis on pufferfishes, elephant shark, lampreys, and amphioxus.Eur. J. Pharmacol66061–69. 10.1016/j.ejphar.2010.10.106

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 379

  VeilletteP. A.YoungG. (2005). Tissue culture of sockeye salmon intestine: functional response of Na +-K+-ATPase to cortisol.Am. J. Physiol. Regul. Integr. Comp. Physiol.2881598–1605. 10.1152/ajpregu.00741.2004

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 380

  VermaG.KhanM. F.AkhtarW.AlamM. M.AkhterM.ShaquiquzzamanM. (2018). Molecular interactions of bisphenols and analogs with glucocorticoid biosynthetic pathway enzymes: an in silico approach.Toxicol. Mech. Methods2845–54. 10.1080/15376516.2017.1356415

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 381

  VijayanM.LeatherlandJ. (1989). Cortisol-induced changes in plasma glucose, protein, and thyroid hormone levels, and liver glycogen content of coho salmon (Oncorhynchus kisutch Walbaum).Can. J. Zool.672746–2750.

  • Google Scholar

• 382

  VirtanenE.SoivioA. (1985). The patterns of T3, T4, cortisol and Na+K+-ATPase during smoltification of hatchery-reared Salmo salar and comparison with wild smolts.Aquaculture4597–109. 10.1016/0044-8486(85)90261-3

  • CrossRef
  • Google Scholar

• 383

  VýbohP.ZemanM.JurániM.BuyseJ.DecuypereE. (1996). Plasma thyroid hormone and growth hormone patterns in precocial Japanese quail and altricial European starlings during postnatal development.Comp. Biochem. Physiol. C Pharmacol. Toxicol. Endocrinol.11423–27. 10.1016/0742-8413(95)02106-X

  • CrossRef
  • Google Scholar

• 384

  WadaH. (2008). Glucocorticoids: Mediators of vertebrate ontogenetic transitions.Gen. Comp. Endocrinol.156441–453. 10.1016/j.ygcen.2008.02.004

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 385

  WalpitaC. N.Van der GeytenS.RurangwaE.DarrasV. M. (2007). The effect of 3,5,3’-triiodothyronine supplementation on zebrafish (Danio rerio) embryonic development and expression of iodothyronine deiodinases and thyroid hormone receptors.Gen. Comp. Endocrinol.152206–214.

  • Google Scholar

• 386

  WangJ.LiJ.ZhangX.SunX. (2012). Transcriptome analysis reveals the time of the fourth round of genome duplication in common carp (Cyprinus carpio).BMC Genomics13:96. 10.1186/1471-2164-13-96

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 387

  WarburtonD.PartonL.BuckleyS.CosicoL.EnnsG.SalunaT. (1988). Combined effects of corticosteroid, thyroid hormones, and (β-agonist on surfactant, pulmonary mechanics, and β-receptor binding in fetal lamb lung.Pediatr. Res.24166–170. 10.1203/00006450-198808000-00005

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 388

  WeberB. M.BowersE. K.TerrellK. A.FalconeJ. F.ThompsonC. F.SakalukS. K. (2018). Pre- and postnatal effects of experimentally manipulated maternal corticosterone on growth, stress reactivity and survival of nestling house wrens.Funct. Ecol.321995–2007. 10.1111/1365-2435.13126

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 389

  WeinbergerC.ThompsonC. C.OngE. S.LeboR.GruolD. J.EvansR. M. (1986). The c-erb-A gene encodes a thyroid hormone receptor.Nature324641–646. 10.1038/324641a0

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 390

  WeissS. L.JohnstonG.MooreM. C. (2007). Corticosterone stimulates hatching of late-term tree lizard embryos.Comp. Biochem. Physiol. A Mol. Integr. Physiol.146360–365. 10.1016/j.cbpa.2006.11.009

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 391

  WeitzelJ. M.ViergutzT.AlbrechtD.BruckmaierR.SchmickeM.TuchschererA.et al (2017). Hepatic thyroid signaling of heat-stressed late pregnant and early lactating cows.J. Endocrinol.234129–141. 10.1530/JOE-17-0066

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 392

  WenL.HeC.SifuentesC. J.DenverR. J. (2019). Thyroid hormone receptor alpha is required for thyroid hormone-dependent neural cell proliferation during tadpole metamorphosis.Front. Endocrinol. (Lausanne)10:396. 10.3389/fendo.2019.00396

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 393

  WentworthB. C.HusseinM. O. (1985). Serum corticosterone levels in embryos, newly hatched, and young turkey poults.Poult. Sci.642195–2201. 10.3382/ps.0642195

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 394

  WilliamsG. (2011). Extrathyroidal expression of TSH receptor.Ann. Endocrinol.7268–73.

  • Google Scholar

• 395

  WilsonJ.BerntsenH. F.ZimmerK. E.VerhaegenS.FrizzellC.RopstadE.et al (2016). Do persistent organic pollutants interact with the stress response? Individual compounds, and their mixtures, interaction with the glucocorticoid receptor.Toxicol. Lett.241121–132. 10.1016/j.toxlet.2015.11.014

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 396

  WiseP. M.FryeB. E. (1973). Functional development of the hypothalamo-hypophyseal-adrenal cortex axis in the chick embryo, Gallus domesticus.J. Exp. Zool.185277–291. 10.1002/jez.1401850302

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 397

  YamadaT.DonaiH.OkauchiM.TagawaM.ArakiK. (2011). Induction of ambicoloration by exogenous cortisol during metamorphosis of spotted halibut Verasper variegatus.Comp. Biochem. Physiol. B Biochem. Mol. Biol.160174–180. 10.1016/j.cbpb.2011.08.004

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 398

  YamanoK.InuiY. (1995). cDNA cloning of thyroid hormone receptor beta for the Japanese flounder.Gen. Comp. Endocrinol.99197–203.

  • Google Scholar

• 399

  YamanoK.MiwaS. (1998). Differential gene expression of thyroid hormone receptor α and β in fish development.Gen. Comp. Endocrinol.10975–85. 10.1006/gcen.1997.7011

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 400

  YamanoK.ArakaiK.SekikawaK.InuiY. (1994). Cloning of thyroid hormone receptor genes expressed in metamorphosing flounder.Dev. Genet.15378–382.

  • Google Scholar

• 401

  YaoitaY.BrownD. D. (1990). A correlation of thyroid hormone receptor gene expression with amphibian metamorphosis.Genes Dev.41917–1924. 10.1101/gad.4.11.1917

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 402

  YaoitaY.ShiY.-B.BrownD. D. (1990). Xenopus laevis α and β thyroid hormone receptors.Proc. Natl. Acad. Sci. U.S.A.877090–7094.

  • Google Scholar

• 403

  YoonB. H.RomeroR.JunJ. K.MaymonE.MazorM.ParkJ. S. (1998). An increase in fetal plasma cortisol but not dehydroepiandrosterone sulfate is followed by the onset of preterm labor in patients with preterm premature rupture of the membranes.Am. J. Obstet. Gynecol.1791107–1114.

  • Google Scholar

• 404

  YoshimuraT. (2013). Thyroid hormone and seasonal regulation of reproduction.Front. Neuroendocrinol.34:157–166. 10.1016/j.yfrne.2013.04.002

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 405

  YoungG. (1986). Cortisol secretion in vitro by the interrenal of coho salmon (Oncorhynchus kisutch) during smoltification relationship with plasma thyroxine and plasma cortisol.Gen. Comp. Endocrinol.63191–200. 10.1016/0016-6480(86)90156-5

  • CrossRef
  • Google Scholar

• 406

  YoungG.BjörnssonB.PrunetP.LinR.BernH. (1989). Smoltification and seawater adaptation in coho salmon (Oncorhynchus kisutch): plasma prolactin, growth hormone, thyroid hormones, and cortisol.Gen. Comp. Endocrinol.74335–345.

  • Google Scholar

• 407

  ZenaL. A.DillonD.HuntK. E.NavasC. A.BuckC. L.BícegoK. C. (2020). Hormonal correlates of the annual cycle of activity and body temperature in the South-American tegu lizard (Salvator merianae).Gen. Comp. Endocrinol.285:113295. 10.1016/j.ygcen.2019.113295

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 408

  ZimmerC.BoogertN. J.SpencerK. A. (2013). Developmental programming: cumulative effects of increased pre-hatching corticosterone levels and post-hatching unpredictable food availability on physiology and behaviour in adulthood.Horm. Behav.64494–500. 10.1016/j.yhbeh.2013.07.002

  • Pubmed Abstract
  • CrossRef
  • Google Scholar

• 409

  ZoellerR. T.TanS. W.TylR. W. (2007). General background on the hypothalamic-pituitary-thyroid (HPT) axis.Crit. Rev. Toxicol.3711–53. 10.1080/10408440601123446

  • Pubmed Abstract
  • CrossRef
  • Google Scholar