Yao Lin
Liyun Chen1
Lijie Du
Haihong Li- 1Department of Plastic Surgery and Burn Center, Second Affiliated Hospital of Shantou University Medical College, Shantou, China
- 2Department of Wound Repair and Dermatologic Surgery, Taihe Hospital, Hubei University of Medicine, Shiyan, China
Eccrine sweat glands (ESGs) play an important role in temperature regulation by secreting sweat. Insufficiency or dysfunction of ESGs in a hot environment or during exercise can lead to hyperthermia, heat exhaustion, heatstroke, and even death, but the ability of ESGs to repair and regenerate themselves is very weak and limited. Repairing the damaged ESGs and regenerating the lost or dysfunctional ESGs poses a challenge for dermatologists and bum surgeons. To promote and accelerate research on the repair and regeneration of ESGs, we summarized the development, structure and function of ESGs, and current strategies to repair and regenerate ESGs based on stem cells, scaffolds, and possible signaling pathways involved.
Introduction
As warm-blooded animals, humans regulate body temperature through various regulatory mechanisms. Among them, ESGs play an important role in cooling down body temperature by secreting primarily water that contains electrolytes (Saga, 2002). Human skin has two major types of sweat glands: eccrine and apocrine. The apocrine sweat glands are appendage of the hair follicle and release a cloudy, viscous fluid through the follicle orifice, which exclusively present in highly localized hairy axillary regions, and they are non-thermoregulatory (Sato et al., 1989). Some patients lack ESGs due to severe burns or genetic factors, while some patients suffered from congenital or acquired factors resulting in ESG dysfunction. If the human body has no way to sweat, it means that any hot weather or acute activity can cause them to get heatstroke or even die. Therefore, we focus on the wound repair and regeneration of ESGs in this review.
First, it is necessary to understand the normal structure and functions of ESGs. On the surface of the body, ESGs are small but very numerous (Sato et al., 1989), which directly open to the skin surface. During exercise, fever or hot environments, humans are able to dissipate heat through sweat to maintain body temperature within the optimal range (Shibasaki et al., 2006). In contrast, for most domestic mammals, most of their body surface lack ESGs. Mouse is the common model for ESG study because of the similarity of human ESG structure and function, which has ESGs solely present in the pads of their paws (Lu et al., 2012).
The ESGs are small tubular structures situated in epidermis and dermis. They comprise a relatively straight duct led to the skin surface and a secretory coil deep in the dermis. The duct of the ESG is a straight channel, and the secretory portion of the ESG is a distinctive, coiled tubular structure (Figure 1).
Figure 1. Structure and cellular constituents of ESGs. The ESG is comprised of a relatively straight duct led to the skin surface and a secretory coil deep in the dermis (left panel). The duct is formed of two layers of cells: the basal (outer) and luminal (inner) cells, where ions are partially reabsorbed (right upper panel). There are three types of cells in the secretory coil: clear cells, dark cells, and myoepithelial cells (right lower panel).
There are three types of cells in the secretory coil: clear cells, dark cells, and myoepithelial cells. Myoepithelial cells provide power support for sweat secretion and support the glands mechanically (Sato, 1977; Sato et al., 1989). The secretory cells can be classified into clear cells and dark cells based on their affinities to basic dyes and granule contents (Montagna et al., 1953; Munger, 1961). The clear cells are without secretory granules but have many mitochondria and membrane villi, which contribute to generate water, electrolytes, and inorganic substances in the sweat. By contrast, the dark cells contain many Schiff-reactive granules, which are mainly in charge of generating macromolecules such as glycoproteins (LobitzJr., and Dobson, 1961; Munger, 1961; Yanagawa et al., 1986). Furthermore, sweat also contains various proteolytic enzymes (Horie et al., 1986), IgA (Okada et al., 1988), active interleukin-1 (Sato and Sato, 1994) and several antimicrobial peptides (Schittek et al., 2001; Niyonsaba et al., 2009), which likely to be conducive to the barrier function of the skin.
The development of electron microscopy (EM) and the ultrastructure that it revealed accelerated the studies of ESGs. Ultrastructural observations on the development of ESG in human embryos have been reported since the 1960s (Hashimoto et al., 1965). From the perspective of embryonic development, at 3 about months, the epidermal ridges on the palms begin to form epithelial cell cords, which are the starting point for the development of ESGs, and at 5 about months, ESGs in other parts of the body begin to develop (Sato et al., 1989). By the eighth month of the fetus, ESGs are morphologically mature (Sato et al., 1989). In mice, ESG germs were spotted at E17.5 and the coiling of secretory portions was at P1, and ESG formation was in essence completed by P5 (Kunisada et al., 2009; Figure 1). In rats, ESG germs were first detected at E19.5, straight ducts first appeared at E21.5, and secretory coils began to form at P1 (Li et al., 2017). During the ESG morphogenesis, the progenitor properties change from multipotency to unipotency, and ultimately, they form four unipotent adult stem cell populations: basal duct, suprabasal duct, myoepithelial, and glandular luminal stem cells (Lu et al., 2012). Proliferation is almost undetectable in the mature glands and remain active only in the basal cells of the sweat duct and the epidermis of the paw skin (Lu et al., 2012).
Feasibility of Regeneration of ESG
Engineered skin is certainly developing rapidly today, while it still lacks skin appendages. As skin appendages, ESGs play important roles in the temperature regulation and maintenance of homeostasis (Huang et al., 2010). So far, patients with irreversible loss of functional ESGs still cannot receive effective treatment. Current strategies for repair and regeneration of ESGs are mainly based on stem cells, scaffolds, bioactive cytokine and growth factors, and involved signaling pathways (Figures 2, 3).
Figure 2. Schematic representation of regeneration of ESGs. With the 3D scaffolds, specific cells can be induced by specific cytokines and growth factors to differeniate into sweat gland-like cells. There are three main types of cells that may be used to repair and regenerate ESGs: ESG-derived stem cells, non-sweat gland-derived stem cells, and induced pluripotent stem cells. This process can take place in vivo or in vitro.
Figure 3. Cells and factors involved in ESG regeneration and their relationships. Stem cells are often used in the study of wound repair and regeneration of various tissues due to their ability to self-renew and differentiate into multiple lineages. To date, eight types of cells have been reported to have the potential to regenerate ESGs (Shikiji et al., 2003; Li et al., 2006, 2015b; Nolte et al., 2008; Sheng et al., 2009; Vierbuchen et al., 2010; Lu et al., 2012; Xu et al., 2012, 2016; Wang et al., 2013, 2019; Hassan et al., 2014; Tao et al., 2014; Liang et al., 2016; Kolakshyapati et al., 2017; Sun et al., 2018; Yao et al., 2018, 2019, 2020; Chen et al., 2019; Hu et al., 2019). Cytokines and growth factors play a role in inducing cells directed to differentiate into sweat gland-like cells during the process of ESG regeneration, and the discovery of these factors involves research on the determination and development of ESGs (Shikiji et al., 2003; Cai et al., 2011; Zhao et al., 2015; Liang et al., 2016; Xu et al., 2016; Kolakshyapati et al., 2017; Sun et al., 2018; Yao et al., 2018, 2019, 2020; Chen et al., 2019; Hu et al., 2019; Wang et al., 2019). Selecting appropriate cells and appropriate factors to induce the differentiation of sweat gland-like cells makes the regeneration of ESGs possible.
ESG Regeneration by Stem Cells
Adult tissue-specific stem cells are distributed in various tissues and organs. In the skin, stem cells have long been found in the epidermis and hair follicles, but it was not known until recently that ESGs are also rich in stem cells (Lu et al., 2012). As judged from immunohistochemical staining of nucleotide analog incorporation and cell proliferation markers, proliferation occurs rarely in the secretory coil cells, but frequently in the basal cells of sweat ducts during homeostasis of adult ESGs (Morimoto and Saga, 1995; Li et al., 2008, 2016b; Chen et al., 2014). With the use of lineage tracing and pulse-chase studies, ESG stem cells have been identified from both developing and mature mouse ESGs by Lu et al. (2012). The multipotent K14+ bud progenitors in the basal layer of embryonic ectoderm is the starting point of ESG formation, which then develops into transient multipotent K14+ basal progenitors and K18+/lowK14 suprabasal progenitors (Lu et al., 2012). Finally, in mature ESGs, the progenitor properties change from multipotency to unipotency in the form of four unipotent adult stem cell populations: basal duct, suprabasal duct, myoepithelial, and glandular luminal stem cells (Lu et al., 2012).
Basal cells in paw epidermis and sweat ducts proliferate can renew and replenish cells of scuffed suprabasal epidermis and intraepidermal duct during homeostasis (Lu et al., 2012; Chen et al., 2014; Li et al., 2016b). When epidermis is severely damaged or excised, neighboring basal cells of epidermis and sweat duct, not including secretory coil cells, rapidly proliferate to repair the injured area (Lu et al., 2012; Chen et al., 2014; Li et al., 2016b). The basal and suprabasal duct stem cells also contribute to repair the skin epidermis and epidermal sweat ducts wound (Lu et al., 2012; Chen et al., 2014; Li et al., 2016b).
There have been many studies that have shown the quiescent nature of both luminal and myoepithelial cells of the secretory coil in adult ESGs (Li et al., 2008, 2016b; Lu et al., 2012). Only when localized injury occurs, do myoepithelial and glandular luminal progenitors replenish their own descendants, and the remarkable thing is that they act as unipotent progenitors during repair (Lu et al., 2012). Luminal cells can proliferate to repair neighboring injured luminal cells, and myoepithelial cells can proliferate to repair neighboring injured myoepithelial cells (Lu et al., 2012). Many studies have shown that the myoepithelial cells of adult ESGs are quiescent (Li et al., 2008, 2016b; Lu et al., 2012).
There are also studies showing that ESG secretory cells not only participate in their own repair, but also participate in the repair of the epidermis, and their regeneration and repair ability is stronger than that of sweat duct luminal cells (Rittie et al., 2013; Pontiggia et al., 2014; Diao et al., 2019). As for myoepithelial cells, it is not clear whether they are involved in epidermal repair under physiological conditions. However, studies have shown that engrafting purified myoepithelial cells to back skin can generate epidermis (Lu et al., 2012). Investigators also isolated cells with typical characteristics of mesenchymal stem cells, from myoepithelial cells of secretory coils in adult human ESGs, which may contribute to the study of wound repair and ESG regeneration (Kurata et al., 2014; Ma Y. et al., 2018).
As is mentioned above, the stem cell populations in mature ESGs are unipotent. However, some unipotent stem cells tend to regain multipotency when leaving the original environment. Based on cell-surface markers, Lu et al. (2012) exploited fluorescent activating cell sorting (FACS), purified different cell populations from mouse secretory coils and sweat ducts, and studied their individual regenerative capacities in engraftment experiments. Grafting the myoepithelial or basal duct stem cells, but not luminal or suprabasal duct stem cells, into cleared mammary fat pads or shoulder fat pads can regenerate de novo ESGs (Lu et al., 2012). Notably, there have been many studies that have shown the quiescent nature of myoepithelial cells in adult ESGs (Li et al., 2008, 2016b; Lu et al., 2012; Leung et al., 2013). Based on these findings, it is interesting that adult progenitors show single-function nature in their native environmemt. Therefore, further experiments will be needed to analyze the molecular causes.
In a previous in vitro study, Li et al. (2013) demonstrated that human ESG cells cultured in Matrigel not only build three-dimensional (3D) tubular-like structures with lumens, but also express α-SMA, epithelial membrane antigen (EMA), CK7, and CK19, and then, they did in vivo experiment on this basis, Matrigel-embedded ESG cells were subcutaneously implanted into nude mice (Li et al., 2015a). Compared with ESGs formed in vitro, ESGs formed in nude mice were more similar to natural ones (Li et al., 2015a). Reconstituted 3D ESGs recapitulated the polarization at the appropriate time points during spheroid differentiation, and secreted fluid similar to native human ESGs (Li et al., 2016a). In addition to the above, the authors also demonstrated that the 3D-reconstituted ESGs were nourished by blood vessels and mediated by both cholinergic and adrenergic innervation (Zhang et al., 2018). Thus, the 3D-reconstituted ESGs have the completeness of structural components, the prerequisite for full functionality, from which the authors inferred that the 3D-reconstituted ESGs may function as the native ones do. However, the secretory function of the 3D-reconstituted ESGs remains to be fully established. All in all, it is an intriguing development in the process of questing treatments burn patients.
The difficulty of using isolated ESG cells to reconstruct sweat gland-like (SGL) structures is that ESG cells are dispersive in the dermis and difficult to gather. Further, with extensive severe burns, the ESGs of patients are destroyed and autologous mature ESG cells and ESG stem cells are insufficient. The optimized cell culture of Diao et al. (2019) can provid the appropriate cells in sufficient quantity for mouse ESGs and skin regeneration, and offers a new strategy for regenerating SGL structures.
In skin tissues, epidermal stem cells (EpiSCs), as the specific stem cell type, can regenerate skin tissue, repair wound and re-modeling (Boehnke et al., 2012). During embryonic development, both ESGs and hair follicles (HFs) originate from EpiSCs, so EpiSCs are the common progenitor cells of both ESGs and HFs. Research has shown that young human keratinocytes, including EpiSCs, can invade collagen gels and differentiate into/toward ESG duct-like structures in vitro with fibroblasts, epidermal growth factor (EGF) and fetal bovine serum (FBS) (Shikiji et al., 2003). EGF, interferon regulatory factor 6 (IRF6) and bone morphogenetic protein 4 (BMP4) have also been shown to play a role in inducing EpiSCs to transform into ESG cells (Shikiji et al., 2003; Yao et al., 2018; Hu et al., 2019). Therefore, EpiSCs can be induced directly and differentiate into ESG cells, and is one of the most common means of ESG regeneration. However, in the adult body, the number of EpiSCs is limited, for merely 1–10 percent of basal stem cells (Cotsarelis et al., 1999). As a result, producing a large number of SGL cells (SGLCs) by epidermal cell reprogramming may be another method for ESG regeneration. Yao et al. (2019) showed that overexpressing the transcription factor FoxC1 can directly reprogram epidermal cells to induce functional SGLCs. Since the epidermis of patients with extensive severe traumatic burns is damaged and autologous mature epidermal cells and EpiSCs is scarce, this method of regeneration is more suitable for anhidrotic/hypohidrotic ectodermal dysplasia patients (Yao et al., 2019).
Bone marrow-derived MSCs (BM-MSCs) are characterized by lower immunogenicity and rarely destroyed in the event of skin damage, so they have great potential for development (Zhang et al., 2015). Although the mechanism of using BM-MSCs to regenerate ESGs remains unclear, multiple cytokines appear to play an important role in ESG regeneration and development. Li et al. (2006) directly co-culture BM-MSCs with heat-shocked ESG cells and found that it can differentiate BM-MSCs into SGLCs. Then, transplanting SGLCs into the wounds of nude mice showed a significantly promotion of damaged ESG repair and regeneration (Sheng et al., 2009). Li et al. (2015b) have also demonstrated that 3D co-culture of BM-MSCs and ESG cells in Matrigel can help the transdifferentiation of BM-MSCs into ESG cells, with the transdifferentiated BM-MSCs potentially able to function as ESG cells. There are other ways to directly induce BM-MSCs to differentiate into SGLCs, and involves various cytokines and scaffolds, which will be described in the following chapters. Even though there is a distinct advantage using BM-MSCs for ESG regeneration, the number of BM-MSCs is limited and it is difficult to maintain pluripotency after extensive passage (Zhang et al., 2015). Recently, investigators have reported that severely burned skin contains viable, undamaged cells that show characteristics of human MSCs, and can be used to promote wound healing without adverse side effects (Amini-Nik et al., 2018). These findings provide an ideal source of MSCs for treatment of severely burned patients.
3D Reconstitution Model of ESG in vitro/vivo
The extracellular matrix (ECM), often used to refer to all the substances surrounding cells in a multicellular organism except for circulating fluids, is a 3D structural scaffold made of non-cellular, fibrous, and non-fibrin proteins that exists in all tissues and is a major component of the cellular microenvironment (Theocharis et al., 2016). The ECM does more than provide physical support for organizational integrity and resilience: it is a dynamic structure that is constantly reshaped to control organizational homeostasis and organ development, as well as tissue repair and regeneration (Bonnans et al., 2014). A highly dynamic 3D ECM provides environmental signals that influence basic cell behaviors, such as cell proliferation, adhesion, migration and differentiation, impact cell mechanics, and regulate the fate of stem cells (Watt and Huck, 2013). Therefore, the ECM plays essential roles not only in embryonic development and homeostasis, but also in tissue engineering and regenerative medicine (Blankenship, 1990; Watt and Huck, 2013; Bonnans et al., 2014). 3D scaffolds are manufactured by removing cellular content from source tissues while retaining the original structural and functional molecular units of the ECM, and it has been widely applied to the field of tissue engineering and regenerative medicine (Costa et al., 2017).
So far, the studies on isolated sweat gland stem cells/progenitor cells cultured in traditional monolayers have always rapidly differentiated into keratinocytes and lost their specific phenotypic characteristics (Rittie et al., 2013; Pontiggia et al., 2014). Compared with the traditional 2D culture models, 3D culture models recapitulate the function and physiological architecture of the body (Kleinman and Martin, 2005; Kozowski et al., 2011). Under 2D culture conditions, cells undergo proliferation but have difficulty in inducing directional differentiation, but under 3D culture conditions, they could be induced directional differentiation (Petrakova et al., 2012; Li et al., 2015b). Therefore, culturing cells under 3D conditions is a useful model for studying cell proliferation and differentiation. To date, researchers have developed several kinds of 3D organoid culture matrices for ESG regeneration, aiming to achieve the enrichment and amplification of cells while maintaining the specific characteristics of ESG cells.
The Matrigel basement membrane matrix (abbreviated as Matrigel) is a dissolved basement membrane preparation that contains fetal collagens, laminin, entactin, heparan sulfate proteoglycans, and several matrix-bound growth factors, which help cell growth as organoids (Kleinman and Martin, 2005; Li et al., 2015a). Using 3D culture method to culture cells in a gel basement membrane matrix, many cells will differentiate into tissue-specific structures, and vascular endothelial cells are one of the earliest cell types showing morphological differentiation (Kleinman and Martin, 2005; Arnaoutova et al., 2009). The differentiation of endothelial cells in Matrigel mimics the process of angiogenesis in vivo, which indicates that Matrigel can be used to obtain a large amount of information about angiogenesis regulators, genes that play an important role in angiogenesis in endothelial cells, and the characterization/identification of endothelial progenitor cells (Auerbach et al., 2003). Besides this, Matrigel has been widely used to study tumor cell invasion, and an altered ECM has been shown to promote tumorigenesis (Bissell and Labarge, 2005). Salivary gland cell lines cultured on Matrigel are widely used to study cell differentiation, such as glandular-like morphogenesis, acinus formation and branching morphogenesis (Barka et al., 2005). Maria et al. (2011) obtained cells from parotid and submandibular glands, expanded in vitro, and then cultured on Matrigel. On Matrigel-coated substrates, cells formed 3D acinar-like units, adopting a large number of secreted granular acinar phenotypes, expressing α-amylase and the water channel protein, aquaporin-5. Experiments by Kozowski et al. (2011) show that the bovine mammary epithelial cell line BME-UV1 cultured on Matrigel could form 3D acinar structures with a hollow lumen in the center, which is similar to the mammary gland alveoli in a functionally active mammary gland. To study ESG progenitor/stem cells, Lu et al. (2012) suspended four sorted ESG cells in Matrigel and injected them individually into cleared mammary or shoulder fat pads from female Nu/Nu mice. In rare cases, purified adult ductal basal cells produce glands and ducts, while purified myoepithelial cells continue to form ESGs, and luminal or suprabasal duct cells did not show this diverse behavior (Lu et al., 2012). Subsequently, Matrigel was applied to the regeneration of ESGs. Li et al. (2013, 2015a) inoculated ESG cells into the tissue structure formed by a Matrigel basement membrane matrix in vitro or in nude mice to simulate the growth microenvironment of natural ESGs, and successfully reconstructed SGL structures using the isolated ESG cells. These studies indicate that the interactions between Matrigel and ESG cells play important roles in the 3D reconstruction of SGL structures. On this basis, Diao et al. (2019) added some growth factors and small molecules, such as EGF, bFGF, and EDA, in order to increase the differentiation efficiency. Although there are some differences between the reconstructed SGL structures and the original ESGs, these studies demonstrated that Matrigel can induce ESG cells to reconstitute SGL structures. Maybe subsequent work could implant Matrigel-embedded ESG cells subcutaneously into burn victims to reconstitute ESGs. However, in practice, the implanted ESG cells do not reconstruct ESGs with complete structure and function as we had hoped. Therefore, in the following scientific research work, there are still many problems for us to explore and solve.
Three-dimensional bioprinting has become a promising technology for manufacturing complex tissue structures with tailor-made biological components and mechanical properties (Murphy and Atala, 2014). By using this revolutionary technology, bio-inks, including growth factors, cells, and hydrogels, can be precisely positioned to create 3D in vitro culture environments (Ma X. et al., 2018). Pati et al. (2014) decellularized adipose, cartilage and heart tissue to make bioink, and adopted a 3D bioprinting technique to construct a 3D structure in vitro, successfully inducing adipose-derived MSCs to express specific markers of cardiomyocytes and chondrocytes. By building 3D printing scaffolds that continuously release a variety of growth factors, Lee et al. (2014) successfully treated sheep with damaged menisci by inducing endogenous MSCs to differentiate into menisci in vivo. The findings strongly suggest that 3D bioprinting has great potential in simulating the microenvironment to induce stem cell differentiation and promote tissue regeneration. Through 3D bioprinting, Fu’s research team successfully induced EpiSCs to differentiate into ESG cells using gelatin-alginate hydrogels and mouse ESG-ECM protein components (Huang et al., 2016; Liu et al., 2016; Li et al., 2018). They subsequently adopted 3D bioprinting to mimic the regenerative microenvironment to direct of MPCs or MSCs to specifically differentiate into ESGs, and ultimately guide the formation and function of glandular tissue (Wang et al., 2019; Yao et al., 2020). Alginate/gelatin hydrogel can serve as bio-ink due to its good cell compatibility, printability, and stable structure during long-term culture (Huang et al., 2009). Wang et al. (2019) used gelatin-alginate hydrogels to combine with ESG-ECM protein to form a characteristic bio-ink, which made it possible to induce the transformation of mammary progenitor cells to ESG cells (Yao et al., 2020). Although its mechanism still needs further exploration, it may be used as an effective tool to induce ideal cells or tissues in vitro through an engineered microenvironment in the future.
Gelatin is not only an irreversible form of denatured collagen, it has the ability to form a scaffold suitable for dermal regeneration without adding any other polymers, but also has the ability to control the release of growth factors for a long time (Shevchenko et al., 2014). Therefore, Huang et al. (2009, 2010) developed gelatin microspheres containing EGF as multifunctional vehicles on which ESG cells could be cultured, and delivered these ESG cell-microsphere complexes into an engineered skin for wound repair. Later, they delivered BM-MSCs by an EGF microsphere-based engineered skin model to repair ESGs and improve cutaneous wound healing (Huang et al., 2012). Analogously, Kolakshyapati et al. (2017) combined the collagen-chitosan porous scaffold with Lipofectamine 2000/pDNA-EGF complexes to yield a gene-activated scaffold (GAS) on which BM-MSCs are cultured. Such GAS/BM-MSCs could accelerate the wound healing and induce full-thickness skin regeneration with SGL structure in situ (Kolakshyapati et al., 2017). These engineered skin constructs are promising tools for ESG regeneration in skin repair and are a valuable engineering strategy for constructing engineered skin models containing appendages.
Mechanism of ESG Development and Regeneration
Up to now, studies have revealed involvement of Wnt, EDA, Shh, BMP, and ERK signaling pathways in ESG determination and development (Figure 4). These findings lead to a series of explorations into the regeneration of ESG.
Figure 4. The signaling pathways involved in ESG development and regeneration. From left to right are the Wnt, EDA-A1, Shh, BMP, and ERK signaling pathways. Wnt signaling pathway (Nusse and Clevers, 2017; Routledge and Scholpp, 2019): in the absence of Wnt signals, GSK-3β/Axin/APC/β-catenin/CK1 is a destruction complex. GSK-3β phosphorylates β-catenin, thereby inhibiting its activity and then β-catenin is degraded by ubiquitination. When Wnt proteins bind to a receptor complex, it induces the association of Axin and Dvl with LRP5/6 and Frizzled. Dvl inhibits GSK-3β and the destruction complex falls apart, and thus prevents the degradation of β-catenin, permitting β-catenin accumulation, leading to binding TCF/LEF in the nucleus to upregulate target genes. EDA signaling pathway (Oeckinghaus et al., 2011; Sisto et al., 2016): in the absence of EDA-A1 signals, NF-κB dimers (P50–P65) are bound to inhibitory IκB proteins, which sequester inactive NF-κB complexes in the cytoplasm. When EDA-A1 binds to EDAR, stimulation of EDAR leads to the binding of EDARADD, for IKK activation. Shh signaling pathway (Fattahi et al., 2018; Xin et al., 2018): in the absence of Shh signals, Ptc inhibits the activity of Smo by affecting its localization to the cell surface, and protein kinases (PKA, CK1, and GSK3β) constitutively phosphorylate Gli proteins to inhibit the Gli. The secreted active Shh ligand binds to Ptc and relieves the repressive effect of the Ptc on Smo, activating the Smo, which then translocates to the cell membrane to inhibit PKA, CK1, and GSK3, providing an assembly platform for the recruitment of Kif7, Sufu and Gli, thus activating the Gli. Subsequently, the activated Gli forms (GliAs) translocate into the nucleus and activate Shh target genes. BMP signaling pathway (Gonzalez and Medici, 2014): when BMPs bind to BMPRs, intracellular Smad1 becomes phosphorylated. The phosphorylated Smad1 binds to Smad4 and then translocates into the nucleus and activates BMP target genes. ERK signaling pathway (Calvo et al., 2010; Gallo et al., 2019): Phosphorylated RTK binds to GRB2, and GRB2 binds to SOS, which stimulates RAS. RAS initiates activation of the MEK-ERK cascade by converting a molecule from GDP to GTP.
Wnt/β-Catenin Signaling Pathway
Wnt/β-catenin signaling pathway is a relatively conservative cell-cell communication system in evolution, which is very important for embryogenesis, stem cell renewal, cell proliferation and cell differentiation (Steinhart and Angers, 2018). When cytokines activate the Wnt signaling pathway, β-catenin accumulates and enters the nucleus, associates with DNA binding factors of the TCF/LEF family, and activates the expression of target genes (Xu et al., 2017). The Wnt/β-catenin signaling pathway is active in the appendages of embryonic ectoderm and is necessary for their formation. Whether the Wnt signaling is upstream or downstream of the EDA signaling is controversial in the basal formation process of the ectodermal appendage, but now, there is mounting evidence that Wnt signaling is an upstream regulator of EDA signaling (Cui et al., 2014). As ESG germs start to form, Wnt activity declines quickly in the dermis and rises strongly in the basal layer of epidermis, and then stays active at the tip of the growing ducts until it disappears when the sweat ducts starts to coil (Cui et al., 2014). According to reports, Wnt10a mutations account for 16% of human hyperhidrosis ectodermal dysplasia (HED) patients (Cluzeau et al., 2011). After further study, researchers have found that Wnt10a/β-catenin signaling is necessary for ESG germ development and postnatal ESG duct development (Xu et al., 2017). It will be interesting in the future to apply Wnt10a to ESG regeneration.
EDA/EDAR/NF-κB Signaling Pathway
Hypohidrotic ectodermal dysplasia is a well-characterized human disease characterized by absent or malformed HFs, teeth, and ESGs (Cui and Schlessinger, 2006; Mikkola, 2009). Much of the information known about ESG determination and development related to signaling pathways originated from research on HED patients. As a member of the TNF family of signaling molecules, ectodysplasin-A (EDA) exists as two highly homologous isoforms, EDA1 and EDA2, and the EDA-A1 gene, specific for the type I transmembrane protein EDA receptor (EDAR), is one of the genes that regulates the determination and development of ESGs (Srivastava et al., 2001). The main axis of the pathway comprises EDA (encoded in mice by tabby), EDAR (encoded by downless), and EDAR-associated death domain (EDARADD, encoded by crinkled) (Srivastava et al., 1997; Monreal et al., 1999). Any mutation in the components of these pathways will cause HED, which is phenocopied in mice (Headon et al., 2001; Cui and Schlessinger, 2006). In addition, mice deficient for nuclear factor-κB (NF-κB) activity also showed a phenotype identical to HED, leading researchers to realize that EDA/EDAR sends signals through the NF-κB pathway during skin appendage development (Doffinger et al., 2001; Kumar et al., 2001; Schmidt-Ullrich et al., 2001). Studies have found that EDA mainly regulates ESG maturation through activating NF-κB after binding to EDAR in the early stages of embryonic development (Doffinger et al., 2001; Kumar et al., 2001).
The almost complete restoration of ectodermal appendages (including ESG) is caused by the transgenic expression of the mouse EDA-A1 isoform in Tabby (EDA-less) (Srivastava et al., 2001), but wild-type mice overexpressing EDA-A1 showed larger ESGs with greater activity (Mustonen et al., 2003). Furthermore, Gaide et al., found that treating pregnant Tabby mice with EDA-A1 recombinant protein can permanently rescue the tabby defect in the offspring (Gaide and Schneider, 2003). Thus, researchers have hypothesized that activation of the EDA gene could induce the regeneration of ESGs. In support of this, the reprogramming of BM-MSCs to SGLCs was successfully induced by the high expression of EDA gene in BM-MSC (Cai et al., 2011). In addition, the findings of Sun et al. (2018) demonstrate that induction of EDA gene overexpression via transfection with an RNA-guided dCas9-effector could promote the transformation of BM-MSCs into SGLCs. These results indicate that the potential of EDA-modified MSCs for the repair and regeneration of ESGs.
As downstream effectors of EDA and EDAR signaling, IKK pathway activates the NF-κB transcription factors for development of skin appendages, and the activated NF-κB transcription factors can enter the nucleus to promote the expression of NF-κB target genes, such as keratins, cyclin D1, Shh and fox family genes (Schmidt-Ullrich et al., 2006). In different stages of ESG development, these genes are essential (Kunisada et al., 2009). Thus, researchers have sought to determine whether NF-κB could induce the regeneration of ESGs in vitro. Zhao et al. (2015) found that human fibroblasts could be directly reprogrammed into SGLCs by introducing NF-κB and Lef-1 (a downstream transcription factor of β-catenin signaling) genes into human fibroblasts. Chen et al. (2019) also noted increased expression of NF-κB during the reprogramming of BM-MSCs into SGLCs by determining the differential expression of miRNAs between BM-MSCs and SGLCs. These results indicate that EDA/EDAR/NF-κB signaling is not only associated with the occurrence and development of ESGs but also plays a vital role in ESG regeneration. However, many other aspects of the EDA/EDAR/NF-κB pathway for ESG regeneration still need to be thoroughly explored, such as receptor activation, ligand binding sites, desensitization, and transportation. It indicates that EDA/EDAR/NF-κB signaling are not only related to the determination and development of ESGs, but also important in ESGs regeneration.
Shh Signaling Pathway
The Shh signaling pathway plays a vital role in embryonic development and tissue regeneration (Xu et al., 2015). The Shh signaling pathway is downstream of the EDA/EDAR/NF-κB signaling pathway. Some studies have shown that Shh signaling is involved in the development of ESG, especially in the process of ESG induction and/or early development, but not in the process of maturation and/or maintenance (Kunisada et al., 2009; Lu and Fuchs, 2014; Lu et al., 2016). Conversely, many studies have also shown that Shh signaling inactivation does not affect the formation of ESG germ or subsequent ducts, but the secretory coil formation is still blocked in the primary stage (Cui et al., 2014; Cui and Schlessinger, 2015). In the process of ESG cells regeneration, it is unclear whether there is a specific connection between the two experimental results. Liang et al. (2016) reported that Shh is an important factor in conditioned medium that influences the differentiation and the formation of ESG tubule-like structures during the differentiation of amniotic fluid stem cells into SGLCs. However, the underlying mechanism is unknown and the exact role of Shh signaling in ESG morphogenesis remains to be clarified.
BMP Signaling Pathway
Bone morphogenetic proteins (BMPs) are multi-functional growth factors belonging to the transforming growth factor (TGF)-β superfamily (Botchkarev and Sharov, 2004). Previous experiments have shown that the ESGs in the mouse paws can be converted into HFs by suppressing the BMP signaling (Plikus et al., 2004). Lu et al. (2016) investigated it further and found that the selection of appendages depends on the antagonism between Shh signaling and BMP signaling in different skin areas in the mesenchyme after epidermal bud formation. When the BMP signaling is in the active state, it determines the formation of ESGs. When BMP signaling is weaker than Shh, it determines the formation of HFs. Hu et al. (2019) cocultured EpiSCs with embryonic paw pad tissue, which demonstrated glandular structure. Moreover, BMP4 concentration was detected in the medium and a BMP receptor inhibitor could effectively block the EpiSC differentiation to ESGs (Hu et al., 2019), implying the possibility of BMP4 application in the regeneration of ESGs.
ERK Signaling Pathway
Epidermal growth factor and FGF, as cytokines, can activate the ERK signaling pathway. EGF can specifically trigger proliferation or differentiation by leading to population-averaged transient or sustained ERK (Marshall, 1995; Santos et al., 2007). By activating ERK through FGFRs, FGF can regulate development, wound healing, and angiogenesis (Ornitz and Itoh, 2015). Some studies have shown that EGF or KGF (also called FGF7) could induce stem cell differentiation into SGLCs (Xu et al., 2016; Kolakshyapati et al., 2017). All of these show that the ERK pathway is important in ESG regeneration.
Conclusion and Future Perspectives
Recently, skin tissue engineering research has been greatly developed. However, current skin substitutes do not contain skin appendages. Therefore, current skin substitutes can only be used to cover the wound, but cannot play physiological functions of normal skin, which is far from enough for patients with severe burns. Studies on the development, structure and function of ESGs have been intensively conducted. On this basis, ESG regeneration has been studied and great advances have been made. The study of skin tissue engineering is often divided into several aspects of cells, scaffolds and biomolecules, and ESG regeneration research is also similar. In this review, ESG and its regeneration have been systematically reviewed. There are three main categories must be considered in ESG regeneration: stem cells, scaffolds, and possible signaling pathways involved.
It is clear from the works herein reviewed that ESG regeneration research involves combination of different types of stem cells, scaffolds, and signaling pathways. So far, researchers successfully reconstructed SGL structures via a variety of methods. However, whether the 3D-reconstituted ESGs can perform physiological functions needs further verification. In addition, the detailed mechanism of how a variety of biomolecules induces ESG differentiation remains to be further studied. Current methods of regenerating ESGs are inefficient, mainly due to the limited number of stem cells, low cell differentiation efficiency and other unpredictable factors. In conclusion, ESG regeneration research is still at a very early stage. We expect to be able to regenerate ESGs to compensate for the inability of tissue-engineered skin to secrete sweat. With the development of stem cells study, molecular biology and biomaterials, ESG regeneration will be achieved in future.
Author Contributions
HL conceived and presented the outline of the review. YL collected literature as well as wrote the review. LC, MZ, SX, LD, and XZ revised the manuscript, provided some relevant insights, and made some edits. All authors read and approved the final version of the manuscript.
Funding
This study was supported in part by the National Natural Science Foundation of China (81772102 and 81471882).
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
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.
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Keywords: eccrine sweat gland, regeneration, stem cells, scaffolds, signaling pathways, methods
Citation: Lin Y, Chen L, Zhang M, Xie S, Du L, Zhang X and Li H (2021) Eccrine Sweat Gland and Its Regeneration: Current Status and Future Directions. Front. Cell Dev. Biol. 9:667765. doi: 10.3389/fcell.2021.667765
Received: 14 February 2021; Accepted: 09 July 2021;
Published: 28 July 2021.
Edited by:
Philip Iannaccone, Northwestern University, United StatesReviewed by:
Vasiliy Galat, Ann & Robert H. Lurie Children’s Hospital of Chicago, United StatesYongan Xu, Zhejiang University, China
Copyright © 2021 Lin, Chen, Zhang, Xie, Du, Zhang and Li. 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: Haihong Li, lihaihong1051@126.com