Background
Leptin is a 16 kDa peptide product of the
ob gene and is secreted by the adipose tissue [
1]. It binds to leptin receptors (OB-R) to mediate several signaling pathways, including Janus kinase 2/signal transducers and activators of transcription (JAK2/STAT), extracellular signal-regulated kinase (ERK) and phosphoinositide 3-kinase (PI3K) [
2]. Leptin has a role in energy homeostasis, glucose and lipid metabolism, and immune and neuroendocrine function that has been shown in both humans and rodents [
3]. Leptin is able to restore fertility in
ob/
ob mice which are leptin deficient, obese and infertile, indicating that leptin serves as a permissive signal to the reproductive system [
4,
5]. Certainly, there is increasing evidence that leptin participates in many events in reproduction [
1].
Serum leptin levels are higher in most obese people and in rodents that have ingested the high-fat diet for a long-term [
6,
7]. Obese men also have higher seminal leptin levels which are associated with increased serum leptin levels [
8]. Body mass index (BMI) has positive correlations with serum leptin levels; both BMI and serum leptin levels correlate positively with abnormal sperm morphology, and correlate negatively with sperm concentration and motility [
9,
10]. This supports the concept that serum leptin mediates a link between obesity and male infertility [
10]. Moreover, serum leptin levels are also increased in azoospermic men compared with normozoospermic fertile men [
11]. This elevation is not gonadotropin dependent, indicating that leptin has a direct effect on testis function, especially on spermatogenesis [
11]. Animal studies have provided evidence that leptin negatively affects male reproduction. Hyperleptinemia has been found to inhibit testicular steroidogenesis and halt testicular maturation in rodents [
12,
13].
Administration of exogenous leptin decreased sperm count and increased the percentage of abnormal sperm in nonobese rodents, suggesting that leptin plays a role in the negative correlations between BMI and sperm quantity and quality [
14]. In nonobese rodents, some studies have also shown that exogenous leptin can increase the percentage of abnormal sperm and the DNA fragmentation level while decreasing sperm count and motility, histone to protamine transition during spermatogenesis, and the ability to generate offspring [
15‐
19]. Leptin may exhibit a direct effect on testicular tissues or spermatozoa leading to abnormal sperm parameters [
14]. It may also induce reactive oxygen species (ROS) production and hormone profile modulation to affect male fertility [
15]. However, additional research is needed to further clarify the mechanisms of leptin’s negative effects on male reproductive function.
Leptin secreted by visceral adipose tissue has been reported to increase the permeability of the intestinal epithelial barrier by reducing the expression of tight junction (TJ)-associated proteins such as zona occludens-1 (ZO-1), zona occludens-3 (ZO-3), claudin 5 and occludin [
20‐
22]. In addition to be the primary structure of the intestinal epithelial barrier, TJ is also a vital structure of the blood testis barrier (BTB). The BTB is comprised of coexisting TJ, basal ectoplasmic specialization, gap junction and desmosome [
23]. TJ in the BTB has two main functions, restricting the passage of molecules and dividing the seminiferous epithelium into basal and apical compartments [
24]. In mice, the contribution of occludin and claudins to BTB integrity are determined by deletion of occludin gene or genes for transcription factors that are upstream regulators of claudins [
25]. The BTB creates a specialized microenvironment that is necessary for germ cells development and movement [
24]. Damage to the BTB can cause germ cell loss, reduced sperm count, male infertility or subfertility [
23,
26‐
28]. As leptin impairs TJ integrity in the intestinal epithelium, and because the impact of leptin on BTB integrity has not been addressed in previous studies, we supposed that leptin might affect male reproduction by impairing BTB integrity.
In this study, we administered different doses of leptin or same volume of saline as a control to adult male mice for 2 weeks. We examined the effects of exogenous leptin on serum leptin levels, serum testosterone levels, sperm parameters and testicular cell apoptosis, as well as BTB integrity and TJ-associated proteins. To evaluate whether leptin had a direct effect on TJ-associated proteins, we treated TM4 cells (a mouse Sertoli cell line) with leptin and further investigated the possible leptin-mediated signaling pathways involved in this process.
Methods
Animals and treatments
Seven-week-old male C57BL/6 mice were purchased from Hubei Research Center of Laboratory Animals. Mice were kept under a 12 h light and 12 h darkness cycle at 24 °C and allowed to adapt for 1 week before the experiments. At the age of 8 weeks, mice received daily intraperitoneal injections with 0.1, 0.5 or 3 mg/kg leptin (recombinant mouse leptin, Prospec, Israel) dissolved in saline or same volume of saline as a control for 2 weeks. The weights of mice and food in each cage were measured every 2 days.
Mice were sacrificed by exsanguination under anesthesia the day after treatment ended. Reproductive organs including testes and epididymides were weighed immediately and used for further experiments. Blood samples were collected and stored at room temperature for 1 h to clot, before centrifuging at 3000 rpm for 15 min to obtain serum for ELISA.
All animal experiments were approved by the Tongji Medical College Committee on the Use and Care of Animals and were conducted according to the Committee’s guidelines.
Cell culture and treatment
TM4 cells were obtained from ATCC and stored in Family Planning Research Institute of Tongji Medical College. TM4 cells were cultured in DMEM/F12 supplemented with 2.5% fetal bovine serum and 5% equine serum at 37 °C and 5% CO2.
To detect the direct effects of leptin on TJ-associated proteins in TM4 cells, cells were seeded at a density of 1 × 10
5/ml in 6-well dishes, cultured with low-serum medium containing 0, 10 or 100 nM leptin for 48 h and then harvested for further experiments. Inhibitors of leptin signaling mediators were employed to determine the possible leptin-mediated signaling pathways in vitro. Cells were pretreated with low-serum medium containing 10 μM AG490, LY294002 or U0126 (the inhibitors of JAK2, PI3K and ERK, respectively) (MCE, USA) dissolved in dimethyl sulfoxide (DMSO) for 4 h (the final concentration of DMSO was 0.1%). The inhibitors were removed, and cells were washed with pre-warmed phosphate buffered saline (PBS). Low-serum medium containing 100 nM leptin was then added to cells. After cultivation for 48 h, cells were harvested for further experiments. The concentration of AG490, LY294002 and U0126 was chosen according to earlier studies [
29‐
31].
Measurement of serum leptin and testosterone levels
Mouse serum leptin and testosterone levels were measured using commercial ELISA kits from Boster Biological Technology (Wuhan, China) and Cusabio (Wuhan, China), respectively. The measurements were processed according to the manufacturer’s protocols.
Assessment of sperm parameters
Cauda epididymides from each mouse were dissected in 1 ml pre-warmed Ham’ s F10 buffer (Sigma-Aldrich, USA) and incubated at 37 °C for 15 min to allow spermatozoa to swim out. Sperm concentration, motility and progressive motility were determined according to the 5th WHO laboratory manual guidelines [
32]. For the detection of sperm with abnormal morphology, sperm suspensions were smeared on glass slides, allowed to dry, and then fixed and stained using a Diff-Quick kit (Phygene, Fuzhou, China) according to the manufacturer’s protocol. The slides were viewed under a light microscope. At least 200 spermatozoa from each sample were assessed. Abnormalities in sperm morphology including head, tail and head-neck connection abnormalities were determined according to Ward et al. [
33].
Apoptosis of testicular cells
TUNEL assay was conducted to detect testicular cell apoptosis. Sections (5 μm) from frozen testes were deproteinized using proteinase K for 25 min at 37 °C. After blocking with 0.1% Triton X-100 for 20 min at room temperature, sections were incubated with TUNEL working solutions (Roche, Germany) in the dark at 37 °C for 1 h and then stained with DAPI and mounted in glycerin. Sections were observed using a fluorescent microscope, and TUNEL positive nuclei which indicated apoptosis were counted in at least 40 seminiferous tubules from three non-consecutive testis sections from each mouse.
Biotin tracer experiment
The biotin tracer experiment was used to determine BTB integrity according to the method of Meng et al. [
34], with a minor modification. EZ-Link Sulfo-NHS-LC-Biotin (Thermo Scientific, USA) was freshly diluted in PBS containing 1 mM CaCl
2 at a final concentration of 10 mg/ml. Mice were anesthetized, and their testes were exposed. A 30G needle was used to gently inject 30 μl of biotin solution into the testes. After 30 min, mice were euthanized, and their testes were immediately removed and frozen. Sections (5 μm) from frozen testes were blocked with 5% albumin from bovine serum in PBS containing 0.1% Triton X-100 for 1 h, and then incubated with streptavidin conjugate-Alexa Fluor 568 (1:3000, Invitrogen, USA) for 30 min at room temperature. Finally, sections were stained with DAPI, mounted in glycerin and observed using a fluorescent microscope. At least 30 seminiferous tubules from three non-consecutive testis sections from each mouse were examined.
Western blot
Western blot was used to detect the expression of TJ-associated proteins both in testes and in TM4 cells, and was performed according to the standard procedure. Antibodies against claudin 5 (Invitrogen, USA), occludin (Proteintech, USA), ZO-1 (Proteintech, USA) and β-Actin (Proteintech, USA) were used with the details given in Additional file
1: Table S1. Immunopositive bands were detected using the enhanced chemiluminescence (ECL) (Beyotime, Beijing, China). β-Actin served as the loading control. The densitometric analysis was performed using ImageJ software.
Immunofluorescence
Immunofluorescence was used to detect the expression and localization of TJ-associated proteins in sections (5 μm) from frozen testes, and was conducted according to the standard procedure. Antibodies against claudin 5 (Invitrogen, USA), occludin (Proteintech, USA) and ZO-1 (Proteintech, USA) were used with the details given in Additional file
1: Table S1. After incubated with Alexa Fluor 488-conjugated secondary antibodies (1:200, Proteintech, USA), sections were stained with DAPI, mounted in glycerin and observed by a fluorescent microscope.
RNA isolation and PCR
Total RNA in TM4 cells and testes was extracted using TRIzol reagent (Invitrogen, USA), and was then reversed-transcribed into cDNA using a PrimeScript RT reagent kit (TAKARA, Japan). To detect leptin receptor mRNA in TM4 cells, synthesized cell cDNA was subjected to PCR using Premix Taq (TAKARA, Japan). PCR products were run in 1.5% agarose gel electrophoresis (120 V, 30 min) and visualized using an imaging system (Bio-Rad, USA). To determine the expression of steroidogenic genes (
Sf-1,
Star and
Cyp11a1) and androgen receptor in testes, synthesized testicular cDNA was subjected to real time quantitative PCR using SYBR ® Premix Ex Taq II (TAKARA, Japan). The primer sequences were listed in Additional file
2: Table S2. Primers for leptin receptor and
Sf-1 have been reported by El-Hefnawy et al. [
35] and Woods et al. [
36], respectively.
Statistical analysis
All data were analyzed using SPSS (ver.21) software. Differences between groups were determined using Kruskal-Wallis test, one-way ANOVA followed by Dunnett test, chi-square test or Student’s t test. Data were expressed as mean ± SD, and differences were considered significant when p < 0.05. Graphs were made using Graphpad Prism 7.
Discussion
Leptin is a well-known protein secreted by adipose tissue that maintains normal reproductive function. This is proven by administering leptin to
ob/
ob mice to restore fertility [
4,
5]. However, leptin seems to have adverse impacts on male fertility when serum leptin levels are higher than normal and in nonobese rodents given exogenous leptin. The present study highlighted the effects of exogenous leptin on sperm parameters and the role of leptin in damaging BTB integrity, which could be a mechanism for leptin-related male subfertility and infertility.
It is evident that leptin treatment restores reproductive function in
ob/
ob mice [
4,
5,
37]. However, the effects of leptin treatment on normal rodents are negative [
14‐
19]. In our study, sperm concentration, motility and progressive motility decreased whereas the percentage of abnormal sperm and the number of apoptotic testicular cells increased in 3 mg/kg leptin-treated mice. Using a biotin tracer, we showed that these mice also had impaired BTB integrity. Haron et al. suggested that decreased sperm count and increased abnormal spermatozoa in leptin-treated rodents were likely due to a direct effect of leptin on spermatozoa or testicular tissues [
14]; Abbasihormozi et al. proposed that exogenous leptin suppressed male fertility by sperm ROS production or hormone modulation [
15]. Here, we showed that altered sperm parameters in normal mice exposed to exogenous leptin had a relationship with impaired BTB integrity. The BTB acts as a physical and immunological barrier to protect spermatogenic cells from toxicants, and from being recognized and attacked by the immune system [
23]. Exposure to some environmental toxicants can induce injury to the BTB and elicit subsequent damage as germ cell loss, reduced sperm count, male infertility or subfertility [
23,
26‐
28]. Impaired BTB might alter the microenvironment for spermatogenesis in 3 mg/kg leptin-treated mice leading to germ cell apoptosis and compromised sperm quantity and quality. The biotin tracer assay also showed that biotin was more often observed in the adluminal compartments of seminiferous tubules at stage VIII. Although the BTB disassembles and reconstructs to facilitate the transit of preleptotene spermatocytes into the apical compartments at this stage, it still holds intact function due to its distinctive structure under normal condition [
23]. The results of biotin tracer assay suggested that leptin might interfere with the reconstruction process of the BTB at stage VIII, and thus the BTB was more often impaired at this stage.
The BTB is formed largely by TJ between Sertoli cells, which serves as a barrier and boundary in the seminiferous epithelium. We hypothesized that impaired BTB integrity was associated with decreased expression of TJ-associated proteins. As expected, in 3 mg/kg leptin-treated mice, which had impaired BTB integrity, the expression of claudin 5, occludin and ZO-1 decreased significantly and the immunofluorescent stains of these proteins became thin and irregular at BTB area. Further studies are needed to fully understand the mechanisms underlying leptin’s disruption to the BTB as other junctions in the BTB have not yet been evaluated. Fan et al. determined AR expression using testicular proteins in diet-induced obese mice and suggested AR as an upstream factor affecting BTB integrity [
38]. The decreased testicular AR gene expression in 3 mg/kg leptin-treated mice suggested that it could contribute to inducing BTB impairment. On the other hand, we could not rule out the possibility that leptin directly reduced TJ-associated proteins in Sertoli cells. Leptin carries out its biological effects through OB-R which is expressed in rat Sertoli cells and human Sertoli cells [
39,
40]. Since leptin can modulate the nutritional support for spermatogenesis by altering the metabolic behavior of human Sertoli cells [
40], we treated TM4 cells with low (10 nM) and high concentration (100 nM) of leptin to test the direct effect of leptin on TJ-associated proteins. We first confirmed the presence of OB-R, which allows leptin to interact with TM4 cells. We then found that 100 nM leptin reduced the expression of claudin 5, occludin and ZO-1 in TM4 cells. Taken together, our in vitro experiments confirmed that leptin alone directly reduced TJ-associated proteins, which could contribute to BTB impairment in vivo.
Leptin uses JAK2/STAT3 as its principle signaling pathway [
41], and it also activates ERK and PI3K pathways [
2]. Inhibition of JAK2, ERK and PI3K reversed leptin-induced decline in TJ-associated proteins in TM4 cells to different extents (Fig.
4e). However, AG490, an inhibitor of JAK2, was not the most effective inhibitor to rescue the decrease of TJ-associated proteins in TM4 cells. Activation of JAK2/STAT3, along with the activation of PI3K and ERK, is involved in leptin-induced TJ dysfunction in intestinal cells [
20]. When SUMO-2/3 specific protease (SENP3) is knocked down, it compromises the activation of STAT3, resulting in TJ dysfunction in Sertoli cells [
42]. In addition, a high level of leptin has also been found to upregulate the expression of suppressor of cytokine signaling 3 (SOCS3), which can inhibit STAT3 phosphorylation [
12]. The role of the JAK2/STAT3 pathway in leptin-induced decline in TJ-associated proteins required further investigation. In this study, JAK2/STAT, PI3K and ERK pathways were suggested to be involved in leptin-induced decline in TJ-associated proteins.
Leptin treatment causes body weight loss and increases reproductive organ weights in
ob/
ob mice [
4]. However, leptin treatment hardly alters body weights or reproductive organ weights in normal rodents [
14,
16‐
19,
43], also shown in this study, indicating that the effect on sperm parameters after leptin administration is unlikely due to leptin resistance [
14]. Previous studies have reported that leptin treatment has no influence on serum leptin levels in normal rodents [
14,
18]. Although circulating leptin levels at 1 h after administration of 3 mg/kg leptin show a 170-fold increase in fasted mice and a 13-fold increase in fed mice, the half-life of mouse leptin is found to be 40.2 min [
44]. This could explain why serum leptin levels in our leptin-treated mice were not significantly different compared with control mice.
The relationship between leptin treatment and testosterone has been investigated in many studies. In
ob/
ob mice, leptin treatment increases intratesticular testosterone via improved Leydig cell function [
37]. However, serum testosterone is negatively correlated with serum leptin in humans and rodents [
45‐
47]. In vitro experiments also show that leptin can directly reduce testosterone secretion and the expression of steroidogenic genes [
12,
39,
48]. In normal rats, leptin treatment does not change serum testosterone significantly [
14,
18], although parenchymal testosterone decreases by about 49% compared with control rats [
18]. Our study showed that 3 mg/kg leptin treatment repressed testicular steroidogenesis genes expression in vivo but did not produce a significant decrease in serum testosterone levels. The conflicting findings observed in various studies are most likely due to different experimental objectives and variable study designs such as the different doses of leptin used and experiment durations. In our study, altered sperm parameters and impaired BTB integrity observed in leptin-treated mice were unlikely to be related to the alterations in serum testosterone levels since the decreases were not statistically different. Instead, it seemed to be leptin that exerted critical and direct effects on male reproductive tissues.
Acknowledgments
We would like to thank Liling Wang, Na Fang, and Yuanyuan Li of the Family Planning Research Institute/Center of Reproductive Medicine, Tongji Medical College, HUST, for their excellent technical assistance.