Bradley B. Jamieson1
Aleisha M. Moore2
Dayanara B. Lohr2
Simone X. Thomas1
Lique M. Coolen2
Michael N. Lehman2
Rebecca E. Campbell1
Richard Piet1,2*- 1Centre for Neuroendocrinology and Department of Physiology, University of Otago, Dunedin, New Zealand
- 2Brain Health Research Institute and Department of Biological Sciences, Kent State University, Kent, OH, United States
Polycystic ovary syndrome (PCOS) is associated with elevated androgen and luteinizing hormone (LH) secretion and with oligo/anovulation. Evidence indicates that elevated androgens impair sex steroid hormone feedback regulation of pulsatile LH secretion. Hyperandrogenemia in PCOS may also disrupt the preovulatory LH surge. The mechanisms through which this might occur, however, are not fully understood. Kisspeptin (KISS1) neurons of the rostral periventricular area of the third ventricle (RP3V) convey hormonal cues to gonadotropin-releasing hormone (GnRH) neurons. In rodents, the preovulatory surge is triggered by these hormonal cues and coincident timing signals from the central circadian clock in the suprachiasmatic nucleus (SCN). Timing signals are relayed to GnRH neurons, in part, via projections from SCN arginine-vasopressin (AVP) neurons to RP3VKISS1 neurons. Because rodent SCN cells express androgen receptors (AR), we hypothesized that these circuits are impaired by elevated androgens in a mouse model of PCOS. In prenatally androgen-treated (PNA) female mice, SCN Ar expression was significantly increased compared to that found in prenatally vehicle-treated mice. A similar trend was seen in the number of Avp-positive SCN cells expressing Ar. In the RP3V, the number of kisspeptin neurons was preserved. Anterograde tract-tracing, however, revealed reduced SCNAVP neuron projections to the RP3V and a significantly lower proportion of RP3VKISS1 neurons with close appositions from SCNAVP fibers. Functional assessments showed, on the other hand, that RP3VKISS1 neuron responses to AVP were maintained in PNA mice. These findings indicate that PNA changes some of the neural circuits that regulate the preovulatory surge. These impairments might contribute to ovulatory dysfunction in PNA mice modeling PCOS.
1 Introduction
Polycystic ovary syndrome (PCOS) is a complex and prevalent endocrine disorder, affecting up to 20% of women of reproductive age, and is the most common cause of anovulatory infertility (1, 2). PCOS is associated with clinical and/or biochemical signs of elevated androgen secretion, polycystic ovaries and oligo- or anovulation. The presence of two out of three of these symptoms is the currently accepted criterion for diagnosing PCOS (3, 4). Although the reproductive symptoms of PCOS are expressed in the periphery, some of these dysfunctions may have a central origin. Indeed, ovarian dysfunction in PCOS is thought to be brought about by impaired feedback regulation of the pulsatile gonadotropin-releasing hormone (GnRH) neuron drive on anterior pituitary gonadotropin release, causing follicular arrest and elevated androgen secretion (1, 5).
The etiology of PCOS is not well understood but likely results from the combination of genetic, developmental and environmental factors (6). It has been suggested that prenatal and/or early postnatal exposure to excess androgens might contribute to the abnormal programming of the hypothalamic-pituitary gonadal (HPG) axis and result in endocrine perturbations and ovulatory dysfunction in adult PCOS patients (7). This is supported by preclinical studies in which exposure to high androgens in utero induces PCOS-like symptoms in adult females of many species (8). Consistent with the idea that PCOS is associated with central dysregulation of the HPG axis, some of the reproductive and endocrine phenotypes induced by exposure to excess androgens are prevented by neuron-specific androgen receptor (AR) knockout in mice (9). In addition, we and others have reported that prenatal androgen exposure (PNA) is associated with anatomical, functional and molecular changes within the GnRH neuronal network, including to the kisspeptin (KISS1) neurons, in adulthood (10–19). Although arcuate nucleus kisspeptin neurons, critical in generating pulsatile luteinizing hormone (LH) secretion (20–23), are likely impaired by endocrine dysregulations associated with PCOS, the kisspeptin neurons involved in the preovulatory gonadotropin surge mechanism may also be affected, contributing to impaired ovulatory function in PCOS. How this might occur, however, has not been fully investigated.
In many species, including primates, estrogen positive feedback signals driving the preovulatory GnRH/LH surge are detected and relayed to the GnRH neurons, at least partially, by kisspeptin neurons located in the preoptic area (POA) of the hypothalamus (24–35). In female rodents, the LH surge occurs just before the daily onset of activity, ensuring optimal coordination of ovulation and sexual behavior (36–40). Generation and timing of the surge are dependent on axonal outputs from the suprachiasmatic nucleus (SCN) of the hypothalamus (41–43), where the central circadian clock is located (44–46). GnRH neurons receive direct innervation from vasoactive intestinal peptide (VIP)-expressing SCN neurons (47), which may drive their activity (48–50). Upstream of GnRH neurons, kisspeptin neurons in the rostral periventricular area of the third ventricle (RP3VKISS1) are innervated by arginine vasopressin (AVP)-expressing SCN neurons (51–53), which drive their activity on proestrus via the release of AVP (53). Although RP3VKISS1 neurons express the gene that encodes AR (Ar) (54), prior studies have reported little effect of PNA on Kiss1 expression in the RP3V or on RP3VKISS1 neuron numbers (18, 19, 55). On the other hand, AR is found in the rodent SCN (56) and androgen treatment of ovariectomized female rats upregulates its expression to levels comparable to those found in the male SCN (56, 57). It is, therefore, conceivable that PNA might affect androgen signaling in the SCN, thereby altering the circuits that generate the preovulatory surge.
We hypothesized here that PNA alters the SCN to RP3VKISS1 neuron circuit in adult female mice. Using RNAscope®, we observed that Ar expression is upregulated in the SCN of adult PNA female mice. Adeno-associated virus (AAV)-mediated conditional anterograde tract-tracing revealed that this is associated with fewer projections from SCNAVP neurons to RP3VKISS1 neurons. However, we observed that the function of the SCNAVP→RP3VKISS1 neuron circuit was not measurably changed on diestrus. This suggests that PNA might prevent the estrous cycle-dependent plasticity in the output of this circuit, which drives kisspeptin neuron firing on proestrus (53). We propose that these changes negatively affect the circuits that initiate the preovulatory surge and, therefore, contribute to ovulatory dysfunction in female PNA mice.
2 Materials and methods
2.1 Animals and prenatal androgen treatment
All animals used in this study were adult female mice (3 – 6 months old), including C57BL/6J mice (Jackson Laboratory stock #000664), mice that express the Cre recombinase enzyme (cre) in AVP neurons (Avp-cre; Jackson Laboratory stock #023530), mice that express humanized renilla green fluorescent protein (hrGFP) in kisspeptin neurons (Kiss1-hrGFP; Jackson Laboratory stock #023425) (58) and Avp-cre mice that also express Kiss1-hrGFP (Avp-cre:Kiss1-hrGFP). Avp-cre mice were generated by mating Avp-cre+/- with Avp-cre-/- parents. Avp-cre:Kiss1-hrGFP mice were obtained from matings of Avp-cre+/- with Kiss1-hrGFP positive (Kiss-hrGFPpos) parents or from matings of Avp-cre+/-:Kiss1-hrGFPpos with Kiss1-hrGFPpos parents. Kiss1-hrGFP mice were offspring of these matings that were Avp-cre-/- and Kiss1-hrGFPpos.
To induce PCOS-like symptoms in female mice, we used the well-established and well-characterized PNA model (14, 59). Time-mated pregnant dams were injected subcutaneously with either 100 µL of sesame oil containing dihydrotestosterone (DHT, 250 µg) to generate PNA offspring or 100 µL of sesame oil alone (as a vehicle control, VEH) on gestational days 16 to 18. The female offspring were used in experiments. Mice were group-housed with littermates under controlled temperature (22 ± 2°C) and lighting (12 h light/dark cycle) conditions with ad libitum access to food and water. Mice were assigned to experiments based on their genotype and treatment. All experiments were approved by the Kent State Institutional Animal Care and Use Committee and by the University of Otago Animal Ethics Committee.
2.2 Determination of estrous cycle stage
Estrous cycle stage was determined by vaginal lavage (4 μL H2O) or by collecting vaginal cells using a small metal loop. This was carried out between zeitgeber time (ZT) 2-4. Vaginal smears were stained with toluidine blue or methylene blue. Cytology was examined under light microscopy at 10× magnification to identify estrous cycle stage (60). As reported previously (14, 59), PNA mice did not have regular cycles. In a subset of four PNA and four VEH mice monitored over a 14 day period, VEH mice exhibited clear estrous cycles, spending on average 25.0 ± 2.1% of the cycle in diestrus and 25.0 ± 4.6% in proestrus, whereas PNA mice spent 76.8 ± 8.4% of their estrous cycles in diestrus. We never detected a proestrous stage in PNA mice.
2.3 Stereotaxic surgery and viral vector injection
Avp-cre and Avp-cre:Kiss1-hrGFP mice were anesthetized with isoflurane and placed in a stereotaxic apparatus (Kopf Instruments, Tujunga, CA, USA). Viral vectors were bilaterally injected (400 nL/side) at a rate of 100 nL/min into the SCN (from bregma: 0.5 mm anterior, ± 0.2 mm lateral, 5.8 mm in depth from surface of the skull) with a 1 mL Hamilton syringe. The needle was left in situ for 3 min before, and 10 min after injections. Viral vectors were AAV-DJ-EF1-DIO-mCherry (AAV-DIO-mCherry; 5.05×1013 GC/mL) and AAV-DJ-EF1-DIO-hChR2(E123T/T159C)-p2a-mCherry-WPRE (AAV-DIO-ChR2-mCherry; 1.60×1013 GC/mL) (61, 62).
2.4 Multiplex fluorescent in situ hybridization
RNAscope® (ACDBio, Newark, CA, USA) multiplex fluorescent ISH was used to assess the expression of Ar in the SCN. C57BL/6J female VEH (n=5) and PNA (n=5) mice were killed by intraperitoneal (ip) pentobarbital overdose (ZT6-8) and perfused through the heart with 4% paraformaldehyde (PFA). Brains were extracted and incubated at 4°C for 24 hours in the same fixative. Brains were then sunk in 10%, 20% and 30% sucrose in 0.1M phosphate buffer saline (PBS), rapidly frozen in OCT and stored at -80°C until cryosectioning coronal sections onto superfrost charged slides at 12 μm thickness. Sections were stored at -80°C until use. The assay was performed following the manufacturer’s instructions (ACDBio; 323100-USM) with RNAscope ® probes designed to detect Ar (Cat. #316991) and Avp (Cat. #401391), which were labelled with red (Cy3) and green (Fluorescein) TSA Plus fluorophores, respectively, after signal amplification steps. Finally, cell nuclei were counterstained using 4′,6-diamidino-2-phenylindole (DAPI; ACDBio) and slides were coverslipped using ProLong Gold Antifade Mountant (Fisher Scientific, Cat. #P36930).
2.5 Immunohistochemistry
Avp-cre mice injected with AAV-DIO-mCherry were killed by pentobarbital overdose (ip; ZT4-6) and perfused through the heart with 4% PFA. 40 µm thick coronal brain sections were cut through the RP3V and SCN, of which one in three slices were processed for free-floating IHC. Antibodies used were rabbit anti-mCherry (1:5000; AbCam, Cat. #ab167453) visualized with donkey anti-rabbit AlexaFluor-568 (1:200; ThermoFisher Scientific, Cat. #A10042), and sheep anti-kisspeptin (1:1000; Gift from Prof. Alain Caraty, AC053) visualized with biotinylated donkey anti-sheep (1:1000; ThermoFisher Scientific, Cat. #A16045) revealed by streptavidin AlexaFluor-488 (1:1000; ThermoFisher Scientific, Cat. #S32354).
2.6 Confocal microscopy and image analysis
For ISH, two sections containing the SCN were imaged per animal using an Olympus FV3000 confocal microscope. A 20x objective was used to enable imaging of the unilateral SCN. Optical sections with a 2 μm step size were acquired using 405 nm, 488 nm and 550 nm lasers. For IHC, brain slices were imaged using an inverted Nikon A1R confocal microscope (Nikon Instruments Inc., Tokyo, Japan), with lasers of 488 and 543 nm wavelengths. Z-stack images were taken through the RP3V and SCN. Images were taken at 10× (1 µm Z-step, 1 AU pinhole, 0.5 NA) or 40× (0.5 µm Z-step, 1 AU pinhole, 0.9 NA) magnification. Images were analyzed offline using the FIJI software (63).
2.6.1 SCN cell Ar gene expression analysis
Ar and AVP mRNA expression was quantified in DAPI-labelled cells in the unilateral SCN of two sections per animal. Cells within the SCN were deemed positive for Ar or Avp expression when three or more mRNA puncta overlayed DAPI. The number of Ar-only cells, Avp-only cells and cells coexpressing Avp and Ar were counted, and the percentages of SCN Avp-positive neurons co-expressing Ar and of Ar-positive cells co-expressing Avp were calculated. In addition, the number of Ar puncta within AVP and non-AVP cells was quantified. For all analyses, calculations were averaged for each female and the mean coexpression levels calculated per group.
2.6.2 Axonal projection analyses
mCherry-immunoreactive (ir) projection fiber density was measured on two sets of 10× Z-stack images through the RP3V, including the anteroventral periventricular nucleus (AVPV) and the periventricular preoptic nucleus (PVpo). Maximum projection images were binarized (threshold: 1-1.5%). A region of interest (ROI) extending from the ventral side of the section to the dorsal edge of the third ventricle and 100 μm lateral to the wall of the third ventricle was drawn to include the RP3V in each maximum projection image. The percentage of area covered by mCherry-ir fluorescent pixels (pixel density) was measured in each ROI. This value was averaged across the two RP3V sections in each mouse. To estimate the extent of transfection in the SCN, pixel density was measured within two ROIs delineating the bilateral SCN in a single slice through the middle of its rostro-caudal extent. Measurements were carried out on both sides of the brain. As previously (53), injections that resulted in mCherry-ir covering greater than 5% of the area of at least one ROI were considered successful. For quantifying innervation of the RP3V of VEH and PNA mice, only those animals with successful uni- or bilateral transfection were included, and innervation reported on the side of the brain ipsilateral to the most transfected SCN. In analyses correlating RP3V innervation to SCN transfection in VEH or PNA mice, values obtained on both sides of the brain of all mice in each group were included (n = 18 hemibrains in 9 mice each).
2.6.3 Cell counting and close apposition quantifications
RP3V kisspeptin-ir neurons were imaged at 40× magnification in the same sections as above. Kisspeptin-ir somata were counted bilaterally in two sets of Z-stacks containing the AVPV or PVpo. Close appositions between mCherry-ir fibers and kisspeptin-ir somata were quantified on the side ipsilateral to the most transfected SCN. Individual kisspeptin-ir somata were digitally magnified 4 times and inspected in successive single confocal planes of the Z-stack to determine the presence of appositions between a red fiber and a green soma with no black pixel in-between, as described previously (16, 53, 64). The proportion of kisspeptin-ir neurons with at least one apposition, expressed as a percentage, was calculated for the two RP3V slices and averaged in each mouse.
2.7 Brain slice preparation and electrophysiology
Avp-cre:Kiss1-hrGFP and Kiss1-hrGFP mice were killed by cervical dislocation (ZT3-5), decapitated and their brains quickly removed as described previously (53). Coronal brain slices (200 µm thick) containing the RP3V or the SCN were cut using a vibratome (VT1000S, Leica) in an ice-cold slicing solution containing (in mM): 87 NaCl, 2.5 KCl, 25 NaHCO3, 1.25 NaH2PO4, 0.5 CaCl2, 6 MgCl2, 25 glucose and 75 sucrose. Brain slices were left to incubate at 30°C for at least 1 hour in artificial cerebrospinal fluid (aCSF) containing (in mM): 120 NaCl, 3 KCl, 26 NaHCO3, 1 NaH2PO4, 2.5 CaCl2, 1.2 MgCl2 and 10 glucose. All solutions were equilibrated to pH 7.4 with a mixture of 95% O2/5% CO2. Individual slices were then placed under an upright epifluorescence microscope (Scientifica, UK) and constantly perfused (1.5 mL/min) with warm (~30°C) aCSF. In AAV-DIO-ChR2-mCherry injected mice, we first confirmed that the SCN was sufficiently transfected by visualizing mCherry expression using light-emitting diode (LED; CoolLED, UK) illumination (excitation 542-582 nm, emission 604-679 nm). RP3V GFP-expressing neurons were visualized using brief LED illumination (GFP: excitation 446-486 nm, emission 500-550 nm) and subsequently approached with recording electrodes using infrared differential interference contrast illumination. Because the ChR2 excitation spectrum overlaps that of GFP, low intensity LED illumination was used (~0.8 mW) and a waiting period of at least 10 min following identification of a GFP-expressing neuron was allowed before recordings started (32, 53). Recordings were made with borosilicate glass electrodes (tip resistance: 2-5 MΩ), pulled using a Model P-97 Flaming/Brown micropipette puller (Sutter Instruments, USA). Electrophysiological signals were recorded using a Multiclamp 700A or 700B amplifier (Molecular Devices, USA), filtered at 2 kHz, and digitized at 10 kHz using a Digidata 1322a or 1440a (Molecular Devices, USA). Signal acquisition and analysis was performed with pClamp 9 or 10 (Molecular Devices, USA). Action potential firing was recorded in voltage-clamp mode (no holding potential applied) in the loose-seal, cell-attached configuration (12-20 MΩ seal resistance). Glass microelectrodes were filled with aCSF and the recording configuration was achieved by applying the lowest amount of suction required to detect spikes. To activate ChR2, trains (20 Hz for 60 s) of LED blue light pulses (5 ms duration; 446-486 nm; ~14 mW) were driven by a Master-9 stimulus pattern generator (AMPI, Israel) and delivered to the slice through a 40× immersion objective (0.8 NA, Olympus). In experiments testing the effect of exogenous AVP on spontaneous firing, 500 nM AVP (Tocris-Bioscience, Cat. #2935) was bath applied for 2 minutes after a 2-minute baseline, before being washed out for at least 5 minutes. AVP was dissolved in water to a stock concentration, kept at -20°C until use, and diluted to the appropriate concentration in aCSF. All recordings were carried out between ZT4-10.
Loose seal, cell-attached recordings were analyzed in ClampFit (pClamp, Molecular Devices). Individual spikes, corresponding to action potentials, were detected using the threshold crossing method. Spike initiation time stamps were organized into 10 s bins and the mean firing rate calculated for each bin. In optogenetics experiments, baseline firing rate was the mean firing rate prior to stimulation, immediate response was the mean firing rate during light stimulation and delayed response was the mean firing rate in the bin with greatest deviation from baseline as well as during the two preceding and two following bins in the five minutes post-stimulation. For AVP bath applications, baseline firing rate was the mean firing rate prior to the application whereas the delayed effect was measured as above during the five minutes after the application. If mean firing rates changed by greater than twice the standard deviation of baseline firing (2×SD), this was recorded as an excitatory or inhibitory effect. For those recordings where mean firing rates did not change by greater than 2×SD, measurements were taken at the time when firing deviated the most from baseline during the relevant recording time periods (immediate or delayed).
2.8 Statistical analyses
Statistics were performed using Prism 9.0 (GraphPad). Data are presented in text and figures as mean ± SEM, or linear regression line of best fit ± 95% confidence interval. Comparisons between VEH and PNA were made using unpaired t-tests. Comparisons of linear regression slopes between VEH and PNA was carried out using ANCOVA. Within the VEH and PNA groups, comparisons between two time points were undertaken with paired t-tests while comparisons of more than two time points were carried out with one-way ANOVA. For electrophysiology experiments, proportions of responding cells were compared using chi-squared tests, with the number of individual recordings as the sample size. In RNAscope® and tract-tracing experiments, proportions were compared with unpaired t-tests, and the number of animals was the sample size. Differences were considered statistically significant for a p-value less than 0.05.
3 Results
3.1 PNA increases Ar expression in SCN cells
Using RNAscope®, we first quantified Ar mRNA expression in the SCN of five diestrous VEH and five diestrous PNA mice. Ar mRNA expression was seen throughout the SCN, although it appeared more concentrated in the core subdivision (Figure 1A). PNA significantly increased the total number of Ar-expressing SCN cells (VEH: 108.7 ± 22.54; PNA: 170.3 ± 5.06, p = 0.029 unpaired t-test; Figures 1A, B). The total number of Avp-expressing cells was similar in VEH (90.80 ± 8.08) and PNA mice (105.10 ± 7.24; p = 0.22 unpaired t-test). Interestingly, Ar particles were detected in subsets of Avp-expressing SCN neurons in both groups of mice (Figure 1A). There tended to be a greater number of Avp-expressing cells also containing Ar mRNA particles in PNA, but this did not reach significance (VEH: 35.7 ± 10.67; PNA: 56.9 ± 3.34; p = 0.095, unpaired t-test; Figures 1A, B). The number of cells expressing Ar but not Avp, however, was significantly greater in PNA (VEH: 73.0 ± 12.78; PNA: 113.4 ± 6.65; p = 0.023 unpaired t-test, Figures 1A, B). The proportion of Avp-expressing cells also expressing Ar tended to be higher in PNA (VEH: 38.68 ± 7.44%; PNA: 54.04 ± 3.66%; p = 0.07 unpaired t-test) but the proportion of Ar cells expressing Avp was unchanged (VEH: 30.64 ± 4.22%; PNA: 33.86 ± 2.76%; p = 0.54 unpaired t-test; Figure 1C). Lastly, numbers of Ar mRNA particles were not affected by PNA in Avp+ (VEH: 4.86 ± 0.25 vs PNA: 5.34 ± 0.24, p = 0.21 unpaired t-test) or in Avp- cells (VEH Avp-: 6.52 ± 0.74; vs PNA Avp-: 6.78 ± 0.61; p = 0.79, unpaired t-test; Figure 1D).
Figure 1 PNA increases Ar expression in the SCN of female mice. (A) (Left) Example confocal images of sections from VEH and PNA mice, showing expression of Avp (green) and Ar (red) mRNA in the SCN. (Right) DAPI counterstain merged with Avp and Ar staining revealed Ar-positive cells containing (filled arrowheads) or not (empty arrowheads) Avp mRNA. (B) Summary graph of the numbers of SCN cells expressing transcripts for Avp (Avp+), Ar (Ar+), Ar and Avp (Ar+ and Avp+), or Ar only (Ar+ and Avp-) in VEH and PNA mice. (C) Summary of the proportions of Avp-containing cells also expressing Ar [(Ar+ + Avp+)/Avp+] and of Ar-containing cells also expressing Avp [(Ar+ + Avp+)/Ar+] in the SCN of VEH and PNA mice. (D) Summary graph of the numbers of Ar particles in SCN cells with and without Avp expression. *p < 0.05 unpaired t-tests.
Together, these data confirm that Ar is expressed in the SCN of female mice, including in a subset of Avp-expressing cells. Importantly, our observations also reveal that PNA increases Ar-expression in the adult SCN.
3.2 PNA treatment decreases SCNAVP neuron projections to RP3VKISS1 neurons
We next sought to determine the impact of PNA treatment on the SCNAVP→RP3VKISS1 neuron circuit. Nine VEH and nine PNA Avp-cre females received stereotaxic injections of AAV-DIO-mCherry in the SCN. This resulted in cre-mediated recombination and expression of mCherry in AVP neurons as reported previously (53). Mice were perfused with fixative on diestrus at least 2 weeks later. Of these, eight VEH and six PNA mice had sufficient transfection in the SCN (see methods). Levels of transfection on the most transfected side of the brain, as assessed by SCN mCherry-ir, were similar in VEH (18.10 ± 2.12% of SCN area covered with mCherry-ir) and in PNA mice (16.10 ± 2.56%; p = 0.55, unpaired t-test vs VEH; Figures 2A, C). As reported previously (53), mCherry-ir projection fibers were detected in the RP3V of VEH and PNA mice (Figure 2B). Fiber density on the side ipsilateral to the most transfected SCN, however, was significantly lower in PNA (6.98 ± 0.98% of RP3V area covered with mCherry-ir) than in VEH mice (12.82 ± 2.25%; p = 0.04, unpaired t-test vs PNA; Figure 2C). A significant correlation was found between SCN transfection and RP3V mCherry-ir fiber innervation in VEH and PNA mice (p < 0.0001, R2 = 0.84 and p = 0.004, R2 = 0.41, respectively; linear regressions), indicating that these fibers originate in the SCN, as seen previously (52, 53). The slope of the linear regression was significantly lower in PNA than in VEH mice (0.24 [95% confidence interval 0.09-0.40] and 0.85 [95% confidence interval 0.65-1.05], respectively; n = 18 hemibrains in PNA and in VEH mice; p < 0.0001 ANCOVA; Figure 2D) reflecting the lower fiber density in the RP3V of PNA mice.
Figure 2 PNA decreases innervation of the RP3V by SCNAVP neuron projection fibers. (A) Example maximum projection images showing mCherry-ir neurons (red) in the SCN of VEH and PNA Avp-cre mice injected with AAV-DIO-mCherry. White dashed lines delineate the SCN, the third ventricle (3V) and optic chiasm (OX). (B) Maximum projection images showing mCherry-ir SCNAVP neuron fibers in the RP3V of the VEH and PNA mice shown in (A). White dashed lines delineate the RP3V, 3V and OX. (C) Bar graphs summarizing SCN transfection (left) and RP3V innervation by mCherry-expressing SCNAVP neuron projection fibers (right) in VEH and PNA Avp-cre mice with successful SCN transfection. (D) Linear regression analyses of mCherry-ir fiber density in the RP3V in relation to SCN transfection in VEH and PNA mice. *p < 0.05 unpaired t-test; ****p < 0.0001 ANCOVA.
We then examined close appositions between mCherry-ir fibers and kisspeptin-ir RP3V somata. RP3VKISS1 cell counts were similar in VEH (28.52 ± 1.29 cells per slice; n = 8) and PNA mice (25.00 ± 2.12; n = 8; p = 0.18 unpaired t-test; Figures 3A, B). mCherry-ir fibers were seen surrounding kisspeptin-ir neurons in the RP3V of VEH and PNA mice (Figure 3A). The proportion of kisspeptin-ir neurons with at least one mCherry-ir fiber apposition, however, was significantly smaller in PNA (28.34 ± 4.28%, n = 6) than in VEH mice (44.26 ± 3.61%, n = 8; p = 0.015, unpaired t-test; Figures 3A, C). Consequently, the mean number of mCherry-ir appositions per kisspeptin-ir neuron was significantly lower in PNA (0.42 ± 0.07) than in VEH mice (0.74 ± 0.07; p = 0.008, unpaired t-test; Figure 3D). The number of appositions per innervated kisspeptin-ir neuron, on the other hand, tended to be lower but was not statistically different (VEH: 1.65 ± 0.07; PNA: 1.45 ± 0.07; p = 0.078, unpaired t-test; Figure 3E). Therefore, while the proportion of innervated kisspeptin-ir neurons is lower in PNA mice, those innervated kisspeptin neurons receive, on average, a similar number of putative inputs as in VEH mice.
Figure 3 PNA reduces SCNAVP neuron fiber innervation of RP3VKISS1 neurons. (A) Example maximum projection images showing mCherry-ir SCNAVP neuron fibers (red) around kisspeptin-ir neurons (green) in the RP3V of VEH and PNA Avp-cre mice injected in the SCN with AAV-DIO-mCherry. Example appositions between mCherry-ir SCNAVP neuron fibers and kisspeptin-ir somata are indicated with filled arrowheads. i) and ii) show single confocal planes and orthogonal views for two kisspeptin-ir neurons with appositions. Empty arrowheads point to kisspeptin-ir somata that do not receive such appositions. (B) Bar graph summarizing the average number of kisspeptin-ir neurons per section in the RP3V of VEH and PNA mice. (C) Mean proportion of kisspeptin-ir neuron somata with at least one close apposition by an mCherry-ir fiber. (D, E) Average numbers of appositions per kisspeptin-ir neuron (D) and per innervated kisspeptin-ir neuron (E). *p < 0.05 and **p < 0.01 unpaired t-tests.
Together, these observations indicate that SCNAVP neuron projections to RP3VKISS1 neurons are reduced in PNA mice.
3.3 AVP excites RP3VKISS1 neurons to a similar extent in VEH and PNA mice
We previously reported that exogenous AVP and AVP release from SCNAVP neuron projection fibers stimulate RP3VKISS1 neuron action potential firing (53, 65). We, thus, next examined the function of the SCNAVP→RP3VKISS1 circuit in PNA and VEH mice. These experiments were carried out in diestrous mice as proestrus was not detected in PNA mice.
Overall, we observed that RP3VKISS1 neuron baseline spontaneous action potential firing was similar in brain slices from VEH (1.55 ± 0.28 Hz; n = 22 in 5 mice) and PNA (1.29 ± 0.30 Hz; n = 21 in 4 mice; p = 0.53, unpaired t-test) Avp-cre:Kiss1-hrGFP and Kiss1-hrGFP mice. In slices from Avp-cre:Kiss1-hrGFP mice that received SCN injections of AAV-DIO-ChR2-mCherry, ChR2-expressing SCNAVP neuron projection fibers were stimulated with a train of blue light pulses (20 Hz for 60 seconds; Figure 4A). As reported previously (53), this had no effect on action potential firing during the stimulus, but increased firing thereafter in subsets of cells (Figures 4B–D). Overall, however, and in agreement with our previous observations in diestrous mice (53), optogenetic stimulation of SCNAVP neuron fibers had no significant effect on RP3VKISS1 neuron firing in VEH or in PNA mice (Table 1) and neither the proportion of cells excited (VEH: 50%, PNA: 30%; p = 0.36 chi-squared test) nor the overall changes in firing (percentage of baseline firing; immediate response during stimulation, VEH: 108.10 ± 10.55% and PNA: 93.37 ± 12.66%; delayed response after stimulation, VEH: 111.3 ± 13.20% and PNA: 99.22 ± 10.99%; p = 0.38 and 0.49, respectively, unpaired t-tests; n = 10 in 3 mice each; Figures 4B–D) significantly differed in VEH and PNA mice. Similarly, exogenous AVP (500 nM) stimulated RP3VKISS1 neuron action potential firing (Figure 5A) as seen previously (53, 65), and these responses were comparable in VEH and PNA mice (normalized to baseline firing; VEH: 216.70 ± 20.80% and PNA: 310.80 ± 91.48%; p = 0.31 unpaired t-test; n = 12 in 3 VEH mice and 11 in 3 PNA mice; Figure 5B; Table 2). The proportion of RP3VKISS1 neurons excited by AVP appeared smaller in PNA mice, but this did not reach significance (72.70% in PNA and 100.00% in VEH; p = 0.052, chi-squared test; Figure 5C).
Figure 4 SCNAVP→RP3VKISS1 neuron circuit function in diestrous VEH and PNA mice. (A) Experimental set-up. Cre-dependent AAV-DIO-ChR2-mCherry vectors were injected in the SCN of Avp-cre:Kiss1-hrGFP female mice. GFP-expressing neurons were targeted for cell-attached recordings in brain slices containing the RP3V and SCNAVP neuron projection fibers stimulated with trains of blue LED light pulses. The recording protocol, with timing of light stimulation and periods considered for analysis [immediate (Imm.) and delayed (Del.)], is illustrated in the lower panel. (B) Example traces showing spontaneous action potential firing of RP3VKISS1 neurons from VEH and PNA mice. Blue boxes indicate when the light stimulation occurred. (C) Summary graph of normalized RP3VKISS1 neuron firing rate during (Imm.) and within 5 minutes after (Del.) optogenetic stimulation in VEH and PNA mice. (D) Proportions of RP3VKISS1 neurons displaying responses during and after optogenetic stimulation in VEH and PNA mice. Numbers in bars are cell numbers. Scale bars = 50 pA/60 s.
Table 1 Summary of RP3VKiss1 neuron responses to optogenetic stimulation of SCNAVP neuron projection fibers in VEH and PNA mice.
Figure 5 RP3VKISS1 neuron responses to exogenous AVP are maintained in PNA mice. (A) Example traces illustrating the effect of exogenous AVP (green bars) on RP3VKISS1 neuron action potential firing in slices from VEH (top) and PNA (bottom) mice. (B) Bar graph summarizing AVP-induced changes in RP3VKISS1 neuron firing rate in VEH and PNA mice. (C) Proportions of RP3VKISS1 neurons responding to exogenous AVP in VEH and PNA mice. Numbers in bars are cell numbers. Scale bars = 50 pA/60 s.
Table 2 Summary of RP3VKiss1 neuron responses to exogenous AVP in VEH and PNA mice.
Together, these findings indicate that PNA did not measurably change the function of the SCNAVP→RP3VKISS1 neuron circuit at baseline, in diestrous mice.
4 Discussion
We explored the possibility that the circuits that control ovulation in females are altered in a PNA mouse model of PCOS. Here, we report that a proportion of SCN cells express Ar mRNA. This includes SCN Avp-expressing cells, some of which may be involved in the circuit that controls the preovulatory LH surge through their projections to RP3VKISS1 neurons (51–53). Importantly, we observed that prenatal androgen treatment results in increased Ar expression in the SCN of adult female mice. This indicates that SCN cells, including SCNAVP neurons, may be responsive to circulating androgens and, moreover, that PNA might increase the sensitivity of subsets of SCN cells to circulating androgens. This is associated with evidence for fewer fiber projections from SCNAVP neurons to the RP3V and for fewer RP3VKISS1 neurons receiving innervation from SCNAVP neurons in PNA mice. In addition to anatomical alterations of the SCNAVP→RP3VKISS1 neuron circuit, the absence of estrous cycles likely prevented the expression of the estrous cycle-dependent plasticity that drives kisspeptin neuron activity on proestrus (53). The functionality of the circuit at baseline, however, was not measurably affected. Together, these observations reveal that PNA promotes alterations in gene expression and efferent projections within a circuit involved in regulating the preovulatory surge. These alterations might contribute to ovulatory dysfunction in this model of PCOS.
4.1 SCN Ar expression
We observed expression of the Ar gene in the SCN of VEH and PNA female mice. This is consistent with previous studies that reported Ar mRNA and AR-ir in the SCN of female rats and mice (56, 57, 66). In female rats, AR-ir is found primarily in the core SCN, with little immunoreactivity in AVP neurons (56). We find here, however, that greater than 35% of Avp-expressing SCN cells also express Ar in female mice. This could reflect expression of Ar at levels too low for IHC detection of AR-ir. This might also be due to species differences as it was previously reported that the mouse SCN displays greater numbers of AR-ir cells than the rat SCN (57). The identity of Avp-negative SCN cells that express Ar is unknown. Among the possible subsets of SCN cells, it is tempting to speculate that some of these are vasoactive intestinal peptide-expressing neurons, which project directly to GnRH neurons (47), or prokineticin 2-expressing neurons, which might play a role in the LH surge (67). Further experiments will be required to fully characterize SCN Ar-expressing neurons.
Along with these previous reports, our finding that Ar is expressed in the SCN of female mice, including in SCNAVP neurons, suggests that the SCN may be sensitive to variations in androgen levels. Elevated circulating testosterone seen in PNA mice (14, 59) might, therefore, have an impact on SCN cells. Consistent with this idea, we observed increased Ar expression in the SCN of PNA mice. A similar trend was seen in the number of Avp-positive SCN cells expressing Ar, although this did not reach statistical significance. Interestingly, PNA also increases AR expression in the RP3V (16), a region of the hypothalamus involved in the preovulatory surge (68), and we note that RP3VKISS1 neurons do express Ar (54). Whether AR expression is altered specifically in RP3VKISS1 neurons in PNA mice, however, remains to be seen. Together with the results of our RNAscope® experiment, these observations suggest that PNA might increase sensitivity to circulating androgens within the circuits that initiate the preovulatory surge.
The role of AR in SCN function in females is unclear. In male rats, androgen receptor activation restores gonadectomy-induced alterations in circadian activity rhythms (56). In PNA females, however, excess androgen is not associated with impaired circadian wheel running or with alteration in SCN clock gene expression rhythms. Interestingly, however, PNA impairs the coordination between SCN rhythms and peripheral clock rhythms, suggesting that the synchronizing output of the SCN might be altered (69). Curiously, the link between circadian function and excess androgen might be bidirectional as chronic exposure to constant light results in PCOS-like symptoms, including elevated testosterone secretion, in rats (70).
4.2 SCNAVP→RP3VKISS1 neuron circuit in adult PNA females
Using AAV-mediated anterograde tract-tracing, we observed here that the projections of SCNAVP neurons to RP3VKISS1 neurons, observed previously by us and others (51–53), are substantially reduced in adult PNA female mice. Decreased innervation of RP3VKISS1 neurons by SCNAVP neurons is unlikely to result from PNA-induced alterations in SCN AVP expression. First, Avp gene expression was not measurably affected by PNA in our RNAscope® experiment, where we counted similar numbers of Avp-expressing neurons with comparable numbers of mRNA particles in VEH and PNA. Second, in our anterograde tract-tracing experiment, transfection of cre-expressing SCNAVP neurons with AAV-DIO-mCherry was comparable between VEH and PNA. The decreased density of mCherry-ir fibers in the RP3V and numbers of close appositions to RP3VKISS1 neurons therefore likely reflect decreased axonal projections from SCNAVP neurons.
PNA and other preclinical PCOS animal models have revealed alterations in afferent circuits to GnRH neurons and to kisspeptin neurons in the arcuate nucleus and POA of rodents and sheep (12, 14–17, 71, 72). Our finding that SCNAVP neuron projections to RP3VKISS1 neurons are reduced in PNA mice is reminiscent of observations made in sheep in which innervation of POA kisspeptin neurons is decreased in adult PNA ewes (17), although brain areas where this innervation originates are likely distinct in sheep and in rodents, perhaps reflecting the independence of the LH surge from time-of-day signals in the sheep (73). In addition, previous studies of mouse arcuate nucleus kisspeptin neurons revealed that PNA is associated with decreased glutamatergic and γ-aminobutyric acid (GABA)ergic innervation as well as reduced input from several hypothalamic areas (15), suggesting that both hypothalamic kisspeptin neuron populations might be dysregulated. On the other hand, PNA increases GABAergic synaptic input to GnRH neurons (14, 16). The functional significance of this differential pattern of rewiring to GnRH and kisspeptin neurons by PNA is unknown.
Despite clear anatomical alterations in the projections of SCNAVP neurons to RP3VKISS1 neurons, we did not detect any measurable changes in the function of this circuit. First, spontaneous action potential firing of RP3VKISS1 neurons was similar in brain slices from VEH and PNA mice. This is consistent with a recent report that PNA does not have a measurable impact on arcuate nucleus kisspeptin neuron firing (74) but in sharp contrast with previous observations that GnRH neuron firing is substantially increased by PNA (13, 75). These findings suggest that PNA may not directly alter baseline excitability in kisspeptin neurons as it does in GnRH neurons. Second, we observed that RP3VKISS1 neuron action potential firing was stimulated by AVP to a similar extent in VEH and PNA mice. This indicates that AVP to vasopressin 1a receptor signaling in RP3VKISS1 neurons (53, 65) is not substantially altered in PNA animals. Further, using selective optogenetic stimulation of SCNAVP neuron projections to RP3VKISS1 neurons, we observed that PNA did not change the function of this circuit during diestrus. We have previously reported that the output of the SCNAVP→RP3VKISS1 neuron circuit varies considerably across the estrous cycle, driving kisspeptin neuron activity on proestrus but not on diestrus (53). It is, therefore, possible that PNA, in addition to altering SCN Ar expression and impairing the projections from SCNAVP neurons to RP3VKISS1 cells, prevents the full expression of plasticity within this circuit by disrupting estrous cycles. We note that changes in this circuit might also affect female sexual behavior, as RP3VKISS1 neurons also regulate lordosis in rodents (76).
4.3 Ontogeny of PNA-induced impairments in the SCNAVP→RP3VKISS1 neuron circuit
Although early neonatal administration of androgen or estrogen hormones to female rats potently suppresses Kiss1 expression in the preoptic area (77, 78), the impact of exposure to elevated androgens on RP3VKISS1 neuron numbers and/or Kiss1 expression is variable in animal models of PCOS [reviewed in (79)]. In the RP3V of adult PNA female rodents, Kiss1 expression is unaltered (18, 55) while numbers of kisspeptin-ir neurons are reported as similar or decreased (18, 19). We find here, using immunofluorescence, that numbers of RP3VKISS1 neurons are similar in adult diestrous VEH and PNA females. This suggests that PNA does not affect the development and/or maintenance of kisspeptin expression in the RP3V, despite their expression of Ar (54). It is worth noting, however, that Kiss1 mRNA and kisspeptin are first expressed in the RP3V postnatally (26, 80, 81), days after the initial exposure to androgens in utero, and that RP3VKISS1 neuron numbers reach adult-like levels (26) prior to or around the time of the observed increase in circulating testosterone in postnatal PNA females (71), providing a potential explanation for our observations.
Exposure to androgens in utero results in changes in GnRH neuron gene expression, in reprogramming of estrogen and progesterone negative feedback and in rewiring of GABAergic inputs to GnRH neurons prior to puberty (16, 59, 71, 82). In contrast, other pieces of evidence support the presence of post-pubertal effects of elevated testosterone in adult female PNA mice. Administration of an AR antagonist to adult PNA female mice indeed restores normal GABAergic synaptic input to GnRH neurons and estrous cyclicity (14, 71), whereas ovariectomy reverses and DHT restores elevated GnRH neuron action potential firing in adult PNA mice (75). The timeline of development of SCNAVP neuron projections to RP3VKISS1 neurons is currently unknown. We speculate, however, that establishment of these projections might occur concurrently with the pubertal increase in kisspeptin expression in the RP3V, in parallel with the increase in VIP innervation of GnRH neurons seen in female rats (83) and in preparation for the first estrus. If this were the case, it would suggest that the effects of PNA and elevated androgens on this circuit might be occurring after the pubertal transition as circulating testosterone becomes significantly elevated sometime between postnatal day 40 and 50 (71). Supporting this idea, ovariectomy and estrogen replacement in ovariectomized PNA females restores positive feedback and the LH surge (59), suggesting that abnormal sex steroid secretion, possibly including testosterone, by the adult PNA ovary contributes to reversibly disrupt, but not to re-program, the circuits that mediate estrogen positive feedback. Our observations suggest that this might include the SCNAVP→RP3VKISS1 neuron circuit. Lastly, despite our observations that Ar is expressed in the SCN, including in Avp-expressing cells, and that SCN Ar expression is increased in adult PNA females, whether or not impairments in the SCNAVP→RP3VKISS1 neuron circuit are dependent on AR activation remains to be seen. As PNA may lower circulating estrogen, although not always (16, 18, 19, 59), and estrogen replacement increases the proportion of RP3VKISS1 neurons innervated by AVP-ir fibers in ovariectomized mice (51), we cannot fully rule out that alterations in the SCNAVP→RP3VKISS1 neuron circuit result from PNA-induced dysregulation of estrogen positive feedback effects on this circuit. Further experiments are required to disentangle these potential effects of gonadal steroids in PNA mice.
4.4 Relevance to clinical PCOS
Preclinical animal models of PCOS have provided valuable insight into the pathogenesis of this disorder and progressed our understanding of its neuroendocrine underpinnings [reviewed in (8)]. While impairments in feedback regulation of pulsatile GnRH and LH secretion reported in some of these models correlate well with the pathophysiology of human PCOS, it may be argued that the impact of PNA on the circuits involved in generating the preovulatory surge in female rodents does not. Indeed, although the human preovulatory LH surge requires GnRH receptor signaling (84), GnRH might only play a permissive role in the human preovulatory LH surge (85) and GnRH secretion might, in fact, decrease during the surge (86). Moreover, it is unknown if kisspeptin neurons in the human POA (87) play any role in the preovulatory surge. On the other hand, there is evidence of positive feedback-like effects of estrogen on these neurons (35), while kisspeptin administration induces surge-like increases in LH secretion in women (88). A potential role of the central circadian clock in impaired fertility is supported by reports that circadian disruptions may negatively impact gonadotropin secretion and the menstrual cycle (89–92) and may be associated with PCOS (93). In addition, the preovulatory surge initiates preferentially in the morning in women (94–98), and is time-locked to the diurnal cortisol peak (98), which is controlled by the circadian clock (99). Further, AR expression has been reported in the SCN of men and women (100). Although it is unknown if the timing of the preovulatory surge in women involves projections from the SCN to the GnRH neuronal network and POA kisspeptin neurons, it is tempting to speculate that elevated testosterone might have an impact on the output of the central circadian clock in PCOS patients similar to what we observed in adult PNA female mice. In support of this idea, PCOS may be associated with altered melatonin secretory rhythms, which are controlled by the central circadian clock (101), and this dysregulation correlates with testosterone levels in patients (102, 103).
5 Conclusion
The results reported here indicate that PNA results in alterations of projections from SCNAVP neurons to RP3VKISS1 neurons in adulthood. As this circuit is thought to play a key role in generating the preovulatory surge in female rodents [reviewed in (104)] by driving the activity of RP3VKISS1 neurons and, downstream, GnRH neurons (32, 53, 65), these impairments might contribute to ovulatory dysfunction in this animal model of PCOS.
Data availability statement
The raw data supporting the conclusions of this article will be made available by the authors, without undue reservation.
Ethics statement
The animal study was reviewed and approved by the Animal Ethics Committee, University of Otago and the Institutional Animal Care and Use Committee, Kent State University.
Author contributions
BJ, AM, RC and RP designed the research. BJ, AM, DL and ST carried out the research. BJ, AM, RC and RP analyzed the data. AM, LC and ML contributed laboratory space, reagents and analysis tools. BJ, AM, ML, RC and RP wrote drafts of the article and approved final version to be submitted.
Funding
This work was supported by grants from the Health Research Council of New Zealand (grant #16-027 to RP and RC) and from NICHD (grant #R00HD096120 to AM). BJ was supported by a University of Otago PhD Scholarship.
Acknowledgments
We thank members of the Piet and Campbell laboratories for their comments on earlier drafts of this manuscript. Publication of this study was supported by the Department of Biological Sciences and the Open Access Publishing Fund at Kent State University.
Conflict of interest
The authors declare that the research was conducted in the absence of any commercial or financial relationships that could be construed as a potential conflict of interest.
Publisher’s note
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References
1. Azziz R, Carmina E, Chen Z, Dunaif A, Laven JS, Legro RS, et al. Polycystic ovary syndrome. Nat Rev Dis Primers (2016) 2:16057. doi: 10.1038/nrdp.2016.57
2. Lizneva D, Suturina L, Walker W, Brakta S, Gavrilova-Jordan L, Azziz R. Criteria, prevalence, and phenotypes of polycystic ovary syndrome. Fertil Steril (2016) 106(1):6–15. doi: 10.1016/j.fertnstert.2016.05.003
3. Rotterdam E-S. Revised 2003 consensus on diagnostic criteria and long-term health risks related to polycystic ovary syndrome (PCOS). Hum Reprod (2004) 19(1):41–7. doi: 10.1093/humrep/deh098
4. Teede HJ, Misso ML, Costello MF, Dokras A, Laven J, Moran L, et al. Recommendations from the international evidence-based guideline for the assessment and management of polycystic ovary syndrome. Fertil Steril (2018) 110(3):364–79. doi: 10.1016/j.fertnstert.2018.05.004
5. McCartney CR, Campbell RE, Marshall JC, Moenter SM. The role of gonadotropin-releasing hormone neurons in polycystic ovary syndrome. J Neuroendocrinol (2022) 34(5):e13093. doi: 10.1111/jne.13093
6. Goodarzi MO, Dumesic DA, Chazenbalk G, Azziz R. Polycystic ovary syndrome: Etiology, pathogenesis and diagnosis. Nat Rev Endocrinol (2011) 7(4):219–31. doi: 10.1038/nrendo.2010.217
7. Abbott DH, Dumesic DA, Franks S. Developmental origin of polycystic ovary syndrome - a hypothesis. J Endocrinol (2002) 174(1):1–5. doi: 10.1677/joe.0.1740001
8. Stener-Victorin E, Padmanabhan V, Walters KA, Campbell RE, Benrick A, Giacobini P, et al. Animal models to understand the etiology and pathophysiology of polycystic ovary syndrome. Endocr Rev (2020) 41(4):bnaa010. doi: 10.1210/endrev/bnaa010
9. Caldwell ASL, Edwards MC, Desai R, Jimenez M, Gilchrist RB, Handelsman DJ, et al. Neuroendocrine androgen action is a key extraovarian mediator in the development of polycystic ovary syndrome. Proc Natl Acad Sci USA (2017) 114(16):E3334–E43. doi: 10.1073/pnas.1616467114
10. Burger LL, Wagenmaker ER, Phumsatitpong C, Olson DP, Moenter SM. Prenatal androgenization alters the development of GnRH neuron and preoptic area rna transcripts in female mice. Endocrinology (2020) 161(11):bqaa166. doi: 10.1210/endocr/bqaa166
11. Cheng G, Coolen LM, Padmanabhan V, Goodman RL, Lehman MN. The Kisspeptin/Neurokinin B/Dynorphin (KNDy) cell population of the arcuate nucleus: Sex differences and effects of prenatal testosterone in sheep. Endocrinology (2010) 151(1):301–11. doi: 10.1210/en.2009-0541
12. Porter DT, Moore AM, Cobern JA, Padmanabhan V, Goodman RL, Coolen LM, et al. Prenatal testosterone exposure alters gabaergic synaptic inputs to GnRH and KNDy neurons in a sheep model of polycystic ovarian syndrome. Endocrinology (2019) 160(11):2529–42. doi: 10.1210/en.2019-00137
13. Roland AV, Moenter SM. Prenatal androgenization of female mice programs an increase in firing activity of gonadotropin-releasing hormone (GnRH) neurons that is reversed by metformin treatment in adulthood. Endocrinology (2011) 152(2):618–28. doi: 10.1210/en.2010-0823
14. Sullivan SD, Moenter SM. Prenatal androgens alter gabaergic drive to gonadotropin-releasing hormone neurons: Implications for a common fertility disorder. Proc Natl Acad Sci U.S.A. (2004) 101(18):7129–34. doi: 10.1073/pnas.0308058101
15. Moore AM, Lohr DB, Coolen LM, Lehman MN. Prenatal androgen exposure alters KNDy neurons and their afferent network in a model of polycystic ovarian syndrome. Endocrinology (2021) 162(11):bqab158. doi: 10.1210/endocr/bqab158
16. Moore AM, Prescott M, Marshall CJ, Yip SH, Campbell RE. Enhancement of a robust arcuate gabaergic input to gonadotropin-releasing hormone neurons in a model of polycystic ovarian syndrome. Proc Natl Acad Sci U.S.A. (2015) 112(2):596–601. doi: 10.1073/pnas.1415038112
17. Cernea M, Padmanabhan V, Goodman RL, Coolen LM, Lehman MN. Prenatal testosterone treatment leads to changes in the morphology of KNDy neurons, their inputs, and projections to GnRH cells in female sheep. Endocrinology (2015) 156(9):3277–91. doi: 10.1210/en.2014-1609
18. Osuka S, Iwase A, Nakahara T, Kondo M, Saito A, Bayasula, et al. Kisspeptin in the hypothalamus of 2 rat models of polycystic ovary syndrome. Endocrinology (2017) 158(2):367–77. doi: 10.1210/en.2016-1333
19. Hu Q, Jin J, Zhou H, Yu D, Qian W, Zhong Y, et al. Crocetin attenuates dht-induced polycystic ovary syndrome in mice via revising kisspeptin neurons. BioMed Pharmacother (2018) 107:1363–9. doi: 10.1016/j.biopha.2018.08.135
20. Wakabayashi Y, Nakada T, Murata K, Ohkura S, Mogi K, Navarro VM, et al. Neurokinin b and dynorphin a in kisspeptin neurons of the arcuate nucleus participate in generation of periodic oscillation of neural activity driving pulsatile gonadotropin-releasing hormone secretion in the goat. J Neurosci (2010) 30(8):3124–32. doi: 10.1523/JNEUROSCI.5848-09.2010
21. Clarkson J, Han SY, Piet R, McLennan T, Kane GM, Ng J, et al. Definition of the hypothalamic GnRH pulse generator in mice. Proc Natl Acad Sci U.S.A. (2017) 114(47):E10216–E23. doi: 10.1073/pnas.1713897114
22. Moore AM, Coolen LM, Lehman MN. In vivo imaging of the GnRH pulse generator reveals a temporal order of neuronal activation and synchronization during each pulse. Proc Natl Acad Sci USA (2022) 119(6):e2117767119. doi: 10.1073/pnas.2117767119
23. Nagae M, Uenoyama Y, Okamoto S, Tsuchida H, Ikegami K, Goto T, et al. Direct evidence that KNDy neurons maintain gonadotropin pulses and folliculogenesis as the GnRH pulse generator. Proc Natl Acad Sci U.S.A. (2021) 118(5):e2009156118. doi: 10.1073/pnas.2009156118
24. Smith JT, Li Q, Pereira A, Clarke IJ. Kisspeptin neurons in the ovine arcuate nucleus and preoptic area are involved in the preovulatory luteinizing hormone surge. Endocrinology (2009) 150(12):5530–8. doi: 10.1210/en.2009-0712
25. Smith JT, Popa SM, Clifton DK, Hoffman GE, Steiner RA. Kiss1 neurons in the forebrain as central processors for generating the preovulatory luteinizing hormone surge. J Neurosci (2006) 26(25):6687–94. doi: 10.1523/JNEUROSCI.1618-06.2006
26. Clarkson J, Herbison AE. Postnatal development of kisspeptin neurons in mouse hypothalamus; sexual dimorphism and projections to gonadotropin-releasing hormone neurons. Endocrinology (2006) 147(12):5817–25. doi: 10.1210/en.2006-0787
27. Clarkson J, d'Anglemont de Tassigny X, Moreno AS, Colledge WH, Herbison AE. Kisspeptin-Gpr54 signaling is essential for preovulatory gonadotropin-releasing hormone neuron activation and the luteinizing hormone surge. J Neurosci (2008) 28(35):8691–7. doi: 10.1523/JNEUROSCI.1775-08.2008
28. Smith JT, Shahab M, Pereira A, Pau KY, Clarke IJ. Hypothalamic expression of Kiss1 and gonadotropin inhibitory hormone genes during the menstrual cycle of a non-human primate. Biol Reprod (2010) 83(4):568–77. doi: 10.1095/biolreprod.110.085407
29. Tomikawa J, Homma T, Tajima S, Shibata T, Inamoto Y, Takase K, et al. Molecular characterization and estrogen regulation of hypothalamic Kiss1 gene in the pig. Biol Reprod (2010) 82(2):313–9. doi: 10.1095/biolreprod.109.079863
30. Hoffman GE, Le WW, Franceschini I, Caraty A, Advis JP. Expression of fos and in vivo median eminence release of lhrh identifies an active role for preoptic area kisspeptin neurons in synchronized surges of LH and LHRH in the ewe. Endocrinology (2011) 152(1):214–22. doi: 10.1210/en.2010-0066
31. Matsuda F, Nakatsukasa K, Suetomi Y, Naniwa Y, Ito D, Inoue N, et al. The luteinising hormone surge-generating system is functional in male goats as in females: Involvement of kisspeptin neurones in the medial preoptic area. J Neuroendocrinol (2015) 27(1):57–65. doi: 10.1111/jne.12235
32. Piet R, Kalil B, McLennan T, Porteous R, Czieselsky K, Herbison AE. Dominant neuropeptide cotransmission in kisspeptin-gaba regulation of GnRH neuron firing driving ovulation. J Neurosci (2018) 38(28):6310–22. doi: 10.1523/JNEUROSCI.0658-18.2018
33. Watanabe Y, Uenoyama Y, Suzuki J, Takase K, Suetomi Y, Ohkura S, et al. Oestrogen-induced activation of preoptic kisspeptin neurones may be involved in the luteinising hormone surge in male and female Japanese monkeys. J Neuroendocrinol (2014) 26(12):909–17. doi: 10.1111/jne.12227
34. Vargas Trujillo M, Kalil B, Ramaswamy S, Plant TM. Estradiol upregulates kisspeptin expression in the preoptic area of both the male and female rhesus monkey (Macaca mulatta): Implications for the hypothalamic control of ovulation in highly evolved primates. Neuroendocrinology (2017) 105(1):77–89. doi: 10.1159/000448520
35. Rumpler E, Skrapits K, Takacs S, Gocz B, Trinh SH, Racz G, et al. Characterization of kisspeptin neurons in the human rostral hypothalamus. Neuroendocrinology (2021) 111(3):249–62. doi: 10.1159/000507891
36. Murr SM, Geschwind II, Bradford GE. Plasma LH and FSH during different oestrous cycle conditions in mice. J Reprod Fertil (1973) 32(2):221–30. doi: 10.1530/jrf.0.0320221
37. Mahoney MM, Sisk C, Ross HE, Smale L. Circadian regulation of gonadotropin-releasing hormone neurons and the preovulatory surge in luteinizing hormone in the diurnal rodent, Arvicanthis niloticus, and in a nocturnal rodent, Rattus norvegicus. Biol Reprod (2004) 70(4):1049–54. doi: 10.1095/biolreprod.103.021360
38. Mahoney MM, Smale L. A daily rhythm in mating behavior in a diurnal murid rodent Arvicanthis niloticus. Horm Behav (2005) 47(1):8–13. doi: 10.1016/j.yhbeh.2004.07.006
39. Monroe SE, Rebar RW, Gay VL, Midgley AR Jr. Radioimmunoassay determination of luteinizing hormone during the estrous cycle of the rat. Endocrinology (1969) 85(4):720–4. doi: 10.1210/endo-85-4-720
40. Turgeon J, Greenwald GS. Preovulatory levels of plasma LH in the cyclic hamster. Endocrinology (1972) 90(3):657–62. doi: 10.1210/endo-90-3-657
41. Wiegand SJ, Terasawa E. Discrete lesions reveal functional heterogeneity of suprachiasmatic structures in regulation of gonadotropin secretion in the female rat. Neuroendocrinology (1982) 34(6):395–404. doi: 10.1159/000123335
42. Meyer-Bernstein EL, Jetton AE, Matsumoto SI, Markuns JF, Lehman MN, Bittman EL. Effects of suprachiasmatic transplants on circadian rhythms of neuroendocrine function in golden hamsters. Endocrinology (1999) 140(1):207–18. doi: 10.1210/endo.140.1.6428
43. de la Iglesia HO, Meyer J, Schwartz WJ. Lateralization of circadian pacemaker output: Activation of left- and right-sided luteinizing hormone-releasing hormone neurons involves a neural rather than a humoral pathway. J Neurosci (2003) 23(19):7412–4. doi: 10.1523/JNEUROSCI.23-19-07412.2003
44. Moore RY, Eichler VB. Loss of a circadian adrenal corticosterone rhythm following suprachiasmatic lesions in the rat. Brain Res (1972) 42(1):201–6. doi: 10.1016/0006-8993(72)90054-6
45. Stephan FK, Zucker I. Circadian rhythms in drinking behavior and locomotor activity of rats are eliminated by hypothalamic lesions. Proc Natl Acad Sci U.S.A. (1972) 69(6):1583–6. doi: 10.1073/pnas.69.6.1583
46. Lehman MN, Silver R, Gladstone WR, Kahn RM, Gibson M, Bittman EL. Circadian rhythmicity restored by neural transplant. immunocytochemical characterization of the graft and its integration with the host brain. J Neurosci (1987) 7(6):1626–38.
47. van der Beek EM, Wiegant VM, van der Donk HA, van den Hurk R, Buijs RM. Lesions of the suprachiasmatic nucleus indicate the presence of a direct vasoactive intestinal polypeptide-containing projection to gonadotrophin-releasing hormone neurons in the female rat. J Neuroendocrinol (1993) 5(2):137–44. doi: 10.1111/j.1365-2826.1993.tb00373.x
48. van der Beek EM, van Oudheusden HJ, Buijs RM, van der Donk HA, van den Hurk R, Wiegant VM. Preferential induction of c-fos immunoreactivity in vasoactive intestinal polypeptide-innervated gonadotropin-releasing hormone neurons during a steroid-induced luteinizing hormone surge in the female rat. Endocrinology (1994) 134(6):2636–44. doi: 10.1210/endo.134.6.8194489
49. Christian CA, Moenter SM. Vasoactive intestinal polypeptide can excite gonadotropin-releasing hormone neurons in a manner dependent on estradiol and gated by time of day. Endocrinology (2008) 149(6):3130–6. doi: 10.1210/en.2007-1098
50. Piet R, Dunckley H, Lee K, Herbison AE. Vasoactive intestinal peptide excites GnRH neurons in male and female mice. Endocrinology (2016) 157(9):3621–30. doi: 10.1210/en.2016-1399
51. Vida B, Deli L, Hrabovszky E, Kalamatianos T, Caraty A, Coen CW, et al. Evidence for suprachiasmatic vasopressin neurones innervating kisspeptin neurones in the rostral periventricular area of the mouse brain: Regulation by oestrogen. J Neuroendocrinol (2010) 22(9):1032–9. doi: 10.1111/j.1365-2826.2010.02045.x
52. Williams WP 3rd, Jarjisian SG, Mikkelsen JD, Kriegsfeld LJ. Circadian control of kisspeptin and a gated GnRH response mediate the preovulatory luteinizing hormone surge. Endocrinology (2011) 152(2):595–606. doi: 10.1210/en.2010-0943
53. Jamieson BB, Bouwer GT, Campbell RE, Piet R. Estrous cycle plasticity in the central clock output to kisspeptin neurons: Implications for the preovulatory surge. Endocrinology (2021) 162(6):bqab071. doi: 10.1210/endocr/bqab071
54. Stephens SBZ, Kauffman AS. Estrogen regulation of the molecular phenotype and active translatome of AVPV kisspeptin neurons. Endocrinology (2021) 162(9):bqab080. doi: 10.1210/endocr/bqab080
55. Caldwell AS, Eid S, Kay CR, Jimenez M, McMahon AC, Desai R, et al. Haplosufficient genomic androgen receptor signaling is adequate to protect female mice from induction of polycystic ovary syndrome features by prenatal hyperandrogenization. Endocrinology (2015) 156(4):1441–52. doi: 10.1210/en.2014-1887
56. Iwahana E, Karatsoreos I, Shibata S, Silver R. Gonadectomy reveals sex differences in circadian rhythms and suprachiasmatic nucleus androgen receptors in mice. Horm Behav (2008) 53(3):422–30. doi: 10.1016/j.yhbeh.2007.11.014
57. Jahan MR, Kokubu K, Islam MN, Matsuo C, Yanai A, Wroblewski G, et al. Species differences in androgen receptor expression in the medial preoptic and anterior hypothalamic areas of adult male and female rodents. Neuroscience (2015) 284:943–61. doi: 10.1016/j.neuroscience.2014.11.003
58. Cravo RM, Frazao R, Perello M, Osborne-Lawrence S, Williams KW, Zigman JM, et al. Leptin signaling in Kiss1 neurons arises after pubertal development. PLoS One (2013) 8(3):e58698. doi: 10.1371/journal.pone.0058698
59. Moore AM, Prescott M, Campbell RE. Estradiol negative and positive feedback in a prenatal androgen-induced mouse model of polycystic ovarian syndrome. Endocrinology (2013) 154(2):796–806. doi: 10.1210/en.2012-1954
60. Caligioni CS. Assessing reproductive status/stages in mice. Curr Protoc Neurosci (2009) Appendix 4:Appendix 4I. doi: 10.1002/0471142301.nsa04is48
61. Berndt A, Schoenenberger P, Mattis J, Tye KM, Deisseroth K, Hegemann P, et al. High-efficiency channelrhodopsins for fast neuronal stimulation at low light levels. Proc Natl Acad Sci U.S.A. (2011) 108(18):7595–600. doi: 10.1073/pnas.1017210108
62. Mattis J, Tye KM, Ferenczi EA, Ramakrishnan C, O'Shea DJ, Prakash R, et al. Principles for applying optogenetic tools derived from direct comparative analysis of microbial opsins. Nat Methods (2011) 9(2):159–72. doi: 10.1038/nmeth.1808
63. Schindelin J, Arganda-Carreras I, Frise E, Kaynig V, Longair M, Pietzsch T, et al. Fiji: An open-source platform for biological-image analysis. Nat Methods (2012) 9(7):676–82. doi: 10.1038/nmeth.2019
64. Yip SH, Boehm U, Herbison AE, Campbell RE. Conditional viral tract tracing delineates the projections of the distinct kisspeptin neuron populations to gonadotropin-releasing hormone (GnRH) neurons in the mouse. Endocrinology (2015) 156(7):2582–94. doi: 10.1210/en.2015-1131
65. Piet R, Fraissenon A, Boehm U, Herbison AE. Estrogen permits vasopressin signaling in preoptic kisspeptin neurons in the female mouse. J Neurosci (2015) 35(17):6881–92. doi: 10.1523/JNEUROSCI.4587-14.2015
66. Cara AL, Henson EL, Beekly BG, Elias CF. Distribution of androgen receptor mRNA in the prepubertal male and female mouse brain. J Neuroendocrinol (2021) 33(12):e13063. doi: 10.1111/jne.13063
67. Xiao L, Zhang C, Li X, Gong S, Hu R, Balasubramanian R, et al. Signaling role of prokineticin 2 on the estrous cycle of female mice. PLoS One (2014) 9(3):e90860. doi: 10.1371/journal.pone.0090860
68. Herbison AE. Estrogen positive feedback to gonadotropin-releasing hormone (GnRH) neurons in the rodent: The case for the rostral periventricular area of the third ventricle RP3V. Brain Res Rev (2008) 57(2):277–87. doi: 10.1016/j.brainresrev.2007.05.006
69. Mereness AL, Murphy ZC, Sellix MT. Developmental programming by androgen affects the circadian timing system in female mice. Biol Reprod (2015) 92(4):88. doi: 10.1095/biolreprod.114.126409
70. Kang X, Jia L, Shen X. Manifestation of hyperandrogenism in the continuous light exposure-induced PCOS rat model. BioMed Res Int (2015) 2015:943694. doi: 10.1155/2015/943694
71. Silva MS, Prescott M, Campbell RE. Ontogeny and reversal of brain circuit abnormalities in a preclinical model of PCOS. JCI Insight (2018) 3(7):e99405. doi: 10.1172/jci.insight.99405
72. Tata B, Mimouni NEH, Barbotin AL, Malone SA, Loyens A, Pigny P, et al. Elevated prenatal anti-mullerian hormone reprograms the fetus and induces polycystic ovary syndrome in adulthood. Nat Med (2018) 24(6):834–46. doi: 10.1038/s41591-018-0035-5
73. Goodman RL, Herbison AE, Lehman MN, Navarro VM. Neuroendocrine control of gonadotropin-releasing hormone: Pulsatile and surge modes of secretion. J Neuroendocrinol (2022) 34(5):e13094. doi: 10.1111/jne.13094
74. Gibson AG, Jaime J, Burger LL, Moenter SM. Prenatal androgen treatment does not alter the firing activity of hypothalamic arcuate kisspeptin neurons in female mice. eNeuro (2021):8(5):ENEURO.0306–21.2021. doi: 10.1523/ENEURO.0306-21.2021
75. Dulka EA, Burger LL, Moenter SM. Ovarian androgens maintain high GnRH neuron firing rate in adult prenatally-androgenized female mice. Endocrinology (2020) 161(1):bqz038. doi: 10.1210/endocr/bqz038
76. Hellier V, Brock O, Candlish M, Desroziers E, Aoki M, Mayer C, et al. Female sexual behavior in mice is controlled by kisspeptin neurons. Nat Commun (2018) 9(1):400. doi: 10.1038/s41467-017-02797-2
77. Kauffman AS, Gottsch ML, Roa J, Byquist AC, Crown A, Clifton DK, et al. Sexual differentiation of Kiss1 gene expression in the brain of the rat. Endocrinology (2007) 148(4):1774–83. doi: 10.1210/en.2006-1540
78. Homma T, Sakakibara M, Yamada S, Kinoshita M, Iwata K, Tomikawa J, et al. Significance of neonatal testicular sex steroids to defeminize anteroventral periventricular kisspeptin neurons and the GnRH/LH surge system in male rats. Biol Reprod (2009) 81(6):1216–25. doi: 10.1095/biolreprod.109.078311
79. Ruddenklau A, Campbell RE. Neuroendocrine impairments of polycystic ovary syndrome. Endocrinology (2019) 160(10):2230–42. doi: 10.1210/en.2019-00428
80. Kumar D, Freese M, Drexler D, Hermans-Borgmeyer I, Marquardt A, Boehm U. Murine arcuate nucleus kisspeptin neurons communicate with GnRH neurons in utero. J Neurosci (2014) 34(10):3756–66. doi: 10.1523/JNEUROSCI.5123-13.2014
81. Semaan SJ, Murray EK, Poling MC, Dhamija S, Forger NG, Kauffman AS. Bax-dependent and bax-independent regulation of Kiss1 neuron development in mice. Endocrinology (2010) 151(12):5807–17. doi: 10.1210/en.2010-0783
82. Berg T, Silveira MA, Moenter SM. Prepubertal development of gabaergic transmission to gonadotropin-releasing hormone (GnRH) neurons and postsynaptic response are altered by prenatal androgenization. J Neurosci (2018) 38(9):2283–93. doi: 10.1523/JNEUROSCI.2304-17.2018
83. Kriegsfeld LJ, Silver R, Gore AC, Crews D. Vasoactive intestinal polypeptide contacts on gonadotropin-releasing hormone neurones increase following puberty in female rats. J Neuroendocrinol (2002) 14(9):685–90. doi: 10.1046/j.1365-2826.2002.00818.x
84. Dubourdieu S, Charbonnel B, D'Acremont MF, Carreau S, Spitz IM, Bouchard P. Effect of administration of a gonadotropin-releasing hormone (GnRH) antagonist (Nal-glu) during the periovulatory period: The luteinizing hormone surge requires secretion of GnRH. J Clin Endocrinol Metab (1994) 78(2):343–7. doi: 10.1210/jcem.78.2.8106622
85. Crowley WF Jr., McArthur JW. Simulation of the normal menstrual cycle in Kallman's syndrome by pulsatile administration of luteinizing hormone-releasing hormone (Lhrh). J Clin Endocrinol Metab (1980) 51(1):173–5. doi: 10.1210/jcem-51-1-173
86. Hall JE, Taylor AE, Martin KA, Rivier J, Schoenfeld DA, Crowley WF Jr. Decreased release of gonadotropin-releasing hormone during the preovulatory midcycle luteinizing hormone surge in normal women. Proc Natl Acad Sci U.S.A. (1994) 91(15):6894–8. doi: 10.1073/pnas.91.15.6894
87. Hrabovszky E, Ciofi P, Vida B, Horvath MC, Keller E, Caraty A, et al. The kisspeptin system of the human hypothalamus: Sexual dimorphism and relationship with gonadotropin-releasing hormone and neurokinin B neurons. Eur J Neurosci (2010) 31(11):1984–98. doi: 10.1111/j.1460-9568.2010.07239.x
88. Jayasena CN, Abbara A, Comninos AN, Nijher GM, Christopoulos G, Narayanaswamy S, et al. Kisspeptin-54 triggers egg maturation in women undergoing in vitro fertilization. J Clin Invest (2014) 124(8):3667–77. doi: 10.1172/JCI75730
89. Danilenko KV, Samoilova EA. Stimulatory effect of morning bright light on reproductive hormones and ovulation: Results of a controlled crossover trial. PLoS Clin Trials (2007) 2(2):e7. doi: 10.1371/journal.pctr.0020007
90. Kripke DF, Elliott JA, Youngstedt SD, Parry BL, Hauger RL, Rex KM. Weak evidence of bright light effects on human LH and FSH. J Circadian Rhythms (2010) 8:5. doi: 10.1186/1740-3391-8-5
91. Lawson CC, Whelan EA, Lividoti Hibert EN, Spiegelman D, Schernhammer ES, Rich-Edwards JW. Rotating shift work and menstrual cycle characteristics. Epidemiology (2011) 22(3):305–12. doi: 10.1097/EDE.0b013e3182130016
92. Wang Y, Gu F, Deng M, Guo L, Lu C, Zhou C, et al. Rotating shift work and menstrual characteristics in a cohort of Chinese nurses. BMC Womens Health (2016) 16:24. doi: 10.1186/s12905-016-0301-y
93. Wang F, Xie N, Wu Y, Zhang Q, Zhu Y, Dai M, et al. Association between circadian rhythm disruption and polycystic ovary syndrome. Fertil Steril (2021) 115(3):771–81. doi: 10.1016/j.fertnstert.2020.08.1425
95. Seibel MM, Shine W, Smith DM, Taymor ML. Biological rhythm of the luteinizing hormone surge in women. Fertil Steril (1982) 37(5):709–11. doi: 10.1016/s0015-0282(16)46288-6
96. Testart J, Frydman R, Roger M. Seasonal influence of diurnal rhythms in the onset of the plasma luteinizing hormone surge in women. J Clin Endocrinol Metab (1982) 55(2):374–7. doi: 10.1210/jcem-55-2-374
97. Cahill DJ, Wardle PG, Harlow CR, Hull MG. Onset of the preovulatory luteinizing hormone surge: Diurnal timing and critical follicular prerequisites. Fertil Steril (1998) 70(1):56–9. doi: 10.1016/s0015-0282(98)00113-7
98. Kerdelhue B, Brown S, Lenoir V, Queenan JT Jr., Jones GS, Scholler R, et al. Timing of initiation of the preovulatory luteinizing hormone surge and its relationship with the circadian cortisol rhythm in the human. Neuroendocrinology (2002) 75(3):158–63. doi: 10.1159/000048233
99. Lightman SL, Birnie MT, Conway-Campbell BL. Dynamics of acth and cortisol secretion and implications for disease. Endocr Rev (2020) 41(3):bnaa002. doi: 10.1210/endrev/bnaa002
100. Fernandez-Guasti A, Kruijver FP, Fodor M, Swaab DF. Sex differences in the distribution of androgen receptors in the human hypothalamus. J Comp Neurol (2000) 425(3):422–35.
101. Amaral FGD, Cipolla-Neto J. A brief review about melatonin, a pineal hormone. Arch Endocrinol Metab (2018) 62(4):472–9. doi: 10.20945/2359-3997000000066
102. Jain P, Jain M, Haldar C, Singh TB, Jain S. Melatonin and its correlation with testosterone in polycystic ovarian syndrome. J Hum Reprod Sci (2013) 6(4):253–8. doi: 10.4103/0974-1208.126295
103. Simon SL, McWhirter L, Diniz Behn C, Bubar KM, Kaar JL, Pyle L, et al. Morning circadian misalignment is associated with insulin resistance in girls with obesity and polycystic ovarian syndrome. J Clin Endocrinol Metab (2019) 104(8):3525–34. doi: 10.1210/jc.2018-02385
Keywords: GnRH, LH surge, circadian, androgen receptor, PCOS, tract-tracing, electrophysiology
Citation: Jamieson BB, Moore AM, Lohr DB, Thomas SX, Coolen LM, Lehman MN, Campbell RE and Piet R (2022) Prenatal androgen treatment impairs the suprachiasmatic nucleus arginine-vasopressin to kisspeptin neuron circuit in female mice. Front. Endocrinol. 13:951344. doi: 10.3389/fendo.2022.951344
Received: 23 May 2022; Accepted: 06 July 2022;
Published: 05 August 2022.
Edited by:
Víctor M. Navarro, Harvard Medical School, United StatesReviewed by:
Yoshihisa Uenoyama, Nagoya University, JapanRichard Anthony DeFazio, University of Michigan, United States
Copyright © 2022 Jamieson, Moore, Lohr, Thomas, Coolen, Lehman, Campbell and Piet. This is an open-access article distributed under the terms of the Creative Commons Attribution License (CC BY). The use, distribution or reproduction in other forums is permitted, provided the original author(s) and the copyright owner(s) are credited and that the original publication in this journal is cited, in accordance with accepted academic practice. No use, distribution or reproduction is permitted which does not comply with these terms.
*Correspondence: Richard Piet, rpiet@kent.edu