In cyclic females, FSH stimulates ovarian estradiol (E2) production and follicular growth up to the terminal stage. A transient elevation in circulating FSH and E2 levels occurs shortly after birth. But what could be the action of FSH on the ovary during this period, and in particular how it stimulates ovarian steroidogenesis without supporting terminal follicular maturation is intriguing. By experimentally manipulating FSH levels, we demonstrate in mice that the mid-infantile elevation in FSH is mandatory for E2 production by the immature ovary, but that it does not stimulate follicle growth. Importantly, FSH increases aromatase expression to stimulate E2 synthesis, however it becomes unable to induce cyclin D2, a major driver of granulosa cell proliferation. Besides, although FSH prematurely induces luteinizing hormone (LH) receptor expression in granulosa cells, LH pathway is not functional in these cells to induce their terminal differentiation. In line with these results, supplying infantile mice with a superovulation regimen exacerbates E2 production, but it does not stimulate the growth of follicles and it does not induce ovulation. Overall, our findings unveil a regulation whereby high postnatal FSH concentrations ensure the supply of E2 required for programming adult reproductive function without inducing follicular maturation before puberty.
Postnatal gonadotrope axis activation has been poorly documented in mammal species. This period of transient elevation in circulating gonadotropins, i.e., luteinizing hormone (LH) and follicle-stimulating hormone (FSH) occurs in the first weeks (rodents, cattle) or months (chimpanzees, humans) after birth in both males and females. It follows a sex dimorphic pattern, with circulating FSH being more elevated than LH in females, while it is the opposite in males1,2,3,4,5,6,7. It is accompanied by sex-specific profiles of sex steroids (testosterone in males and estradiol [E2] in females) that contribute to postnatal male and female sexual development8,9,10,11,12. Gonadotropin and sex steroid levels become markedly elevated, and therefore this period has been named ‘mini-puberty of infancy’ in humans5,9. It is followed by a period of relative quiescence of pituitary gonadotrope and gonadal activities, and then by their re-activation shortly before puberty.
In cyclic females, FSH plays an important role in supporting follicular development up to the terminal stage of maturation13. A number of studies have documented the similarities of FSH actions in the ovary of sexually immature and mature females. Indeed, as in cyclic females, FSH acts via its receptor (FSHR) exclusively located on granulosa cells to convert thecal-derived androgens into estrogens in prepubertal females14,15,16. Besides, FSH also regulates follicular growth during this period as shown in infantile rodents by the arrest of folliculogenesis at the preantral/early antral stage in Fshr−/− and Fshb−/− mice and by its restoration induced by an FSHR agonist in hypophysectomized rats17,18,19. FSH regulation of early follicular growth in infantile mice has also been demonstrated in vitro20. On the other hand, despite the important elevation in circulating FSH in prepubertal females and the associated production of E2, follicles do not grow beyond the antral stage and no ovulation occurs21,22,23,24,25. These latter observations are intriguing given the well-documented stimulatory action of FSH on the growth of follicles13. Therefore, during this period, FSH action on the ovary cannot simply be extrapolated from our knowledge on adult physiology. Hence, in-depths studies are required to thoroughly analyze gonadotrope axis activation and to establish the effect of elevated FSH concentrations on the function of the immature ovary.
Here we used the mouse as an experimental model to determine how elevated postnatal FSH levels regulate key ovarian physiological processes, i.e., steroidogenesis, follicular growth and maturation during the infantile period. We used a pharmacological approach to suppress FSH specifically at its peak during mid-infantile life. The current study clearly shows that the marked elevation in FSH levels occurring during the postnatal period is mandatory for the significant production of E2 by the immature ovary. However, it does not stimulate preantral/early antral follicle growth and it does not stimulate terminal follicular maturation. Our studies provide some molecular cues to explain this unprecedented uncoupling in FSH-mediated regulation of ovarian steroidogenesis and follicular growth during the prepubertal period.
Postnatal FSH levels and ovarian steroidogenesis are dramatically elevated during the infantile period but follicles do not grow beyond the early antral stage
Since postnatal gonadotrope axis activation has been poorly documented in the mouse, we first analyzed the serum profiles of LH, FSH and E2 during the infantile period from 7 to 21 days postnatal (dpn). To better evaluate the magnitude of pituitary and ovary activity during this period, we also monitored these endocrine parameters in adult females at the time of ovulation (proestrus, PE) and at other stages of the estrous cycle. Both LH and FSH levels were elevated in immature females but FSH was largely predominant (Fig. 1A and B). Circulating LH barely reached LH preovulatory surge values even at its peak at 14 dpn, and it declined sharply afterwards (Fig. 1A). By contrast, circulating FSH was ~5 fold higher than in adults at 14 dpn, and it decreased after 17 dpn (Fig. 1B). Ovarian LH and FSH receptivity, as assessed by Lhcgr and Fshr transcript abundance, increased rapidly during this period (Supplementary Fig. 1), further emphasizing the fact that growing follicles (GFs) become sensitive to gonadotropins early after birth in rodents15,16. By using the gold standard method for steroid measurement, i.e., gas chromatography coupled with mass spectrometry (GC-MS), we found that E2 production increased concomitantly to the rise in gonadotropin levels to attain a peak at 14 dpn (Fig. 1C). We further observed an overall increase in the relative abundance of major components of the sex steroid biosynthesis pathway (Supplementary Fig. 1).
At the time of postnatal FSH and LH elevation, numerous GFs up to the preantral/early antral stage with a diameter of ~120–150 μm (mean surface of follicles: ~6 × 103 μm2) were present in the central part of the murine ovary (data not shown), as reported26. They correspond to the first follicular wave of follicles developing immediately after their formation27. They expressed AMH (anti-Müllerian hormone), used as a marker of healthy GFs (Fig. 1D). We observed a somehow similar pattern of follicular growth in ovaries from human infants at an equivalent period of development (2–6 months old; n = 4 ovaries) with numerous AMH positive GFs up to the antral follicle stage (≤2 mm in diameter) (shown at 2 months in Fig. 1D). Those GFs in both mouse and human ovaries also expressed the enzyme that is responsible for the conversion of androgens into estrogens, i.e., aromatase (Fig. 1E), which normally appears in granulosa cells from late antral/preovulatory follicles in sexually mature females (data not shown), as reported28. In addition, human infant ovaries exhibited follicular cysts (9–10 mm in diameter) consisting of a large cavity surrounded by a thick layer of thecal cells that displayed neither AMH nor aromatase expression (Fig. 1E). Follicular cysts are observed throughout childhood in human ovaries29.
Elevated postnatal FSH concentrations are necessary to promote E2 biosynthesis but not for follicular growth
To determine the role of the postnatal elevation in FSH concentrations on both E2 production and follicular growth, female mice were treated by the GnRH receptor antagonist Ganirelix to decrease the FSH peak (12–14 dpn), and some of them were supplemented with the exogenous gonadotropin eCG to substantially re-activate FSH signaling pathway (Fig. 2A). Ganirelix treatment suppressed LH levels and induced an 80% reduction in FSH levels (Fig. 2B and C). It was accompanied by a 2-fold decrease in circulating E2 levels, but these levels remained normal after co-treatment with eCG (Fig. 2D). Notably, in spite of these dramatic effects on ovarian steroidogenesis caused by reduced FSH action, the growth of preantral/early antral follicles of the first wave remained unaltered as shown by their normal number and size (Fig. 2E and F). As a complementary experiment, we administered a superovulation regimen consisting of eCG at 14 dpn for boosting follicular growth and then of hCG at 16 dpn for inducing ovulation through activation of LH signaling. Animals were sacrificed at 17 dpn to assess the effect of the treatment on ovarian steroidogenesis and follicular growth (Fig. 2G). Compared with 14 dpn ovaries, folliculogenesis had slightly progressed in 17 dpn control females, with antral follicles in the central part of the ovary exhibiting a diameter >200 μm (mean surface of follicles: ~1.1 × 104 μm2). Interestingly, the treatment led to the increase by ~ two fold in circulating E2 levels as compared with those in control females (Fig. 2H). However, there was no alteration in follicular growth and no ovulation in mice under surperovulation regimen (Fig. 2I and J).
The refractoriness of follicular growth to high FSH levels may result from the loss of FSH-mediated Ccnd2 expression
In the ovary, FSH up-regulates the expression of aromatase (Cyp19a1) and cyclin D2 (Ccnd2), which are involved in E2 production and follicular growth, respectively13,30,31. CCND2 is specifically expressed in granulosa cells of GFs at the difference of the other D-type cyclins30,31. To understand how FSH stimulates steroidogenesis but not follicular growth in infantile ovaries, we analyzed its action on the expression of these two genes. Study of the ontogeny of both Cyp19a1 and Ccnd2 expression revealed that their relative abundance markedly varied during the infantile period (Fig. 3A). While Cyp19a1 transcript and protein levels grossly followed the same pattern as circulating FSH levels, interestingly Ccnd2 mRNA and protein levels displayed an opposite pattern (Figs 1B and 3A). To better understand the action of FSH on Cyp19a1 and Ccnd2 expression in immature ovaries, we examined the effect of Ganirelix treatment, with or without co-administration of eCG, on the regulation of these two genes. Ganirelix treatment significantly decreased Cyp19a1 mRNA and protein expression in preantral/early antral follicles (Fig. 3B and C), in line with the observed reduction in E2 levels (Fig. 2D). However, it increased Ccnd2 mRNA and protein levels in these follicles (Fig. 3B and C). Supplying eCG prevented the effects of the Ganirelix treatment on both Cyp19a1 and Ccnd2 expression (Fig. 3B and C).
To determine whether these alterations in FSH-regulated Ccnd2 expression had an impact on granulosa cell proliferation in preantral/early antral follicles, we examined by immunohistochemistry the expression of a mitosis marker, i.e., phosphorylated histone H3 (p-HH3)32 and the incorporation of BrdU under these experimental conditions (Fig. 3D). Importantly, Ganirelix treatment increased by ~2 fold the number of granulosa cells expressing p-HH3 or with BrdU incorporation as compared with controls (Fig. 3D), and this effect was prevented by co-administration of eCG (Fig. 3D). To gain further insights into this observed differential regulation of Cyp19a1 and Ccnd2 by FSH in immature ovaries, we analyzed the effect of increasing concentrations of FSH on their expression using an in vitro culture system (Fig. 3E). Ovaries from 12-dpn mice were cultured in serum-free medium, and then treated with different concentrations of purified FSH (50, 200 and 500 ng/ml). At the highest dose, FSH up-regulated the expression of Cyp19a1, but it did not alter that of Ccnd2 (Fig. 3F). In contrast, at the lowest dose, FSH significantly augmented Ccnd2 mRNA levels but not those of Cyp19a1 mRNAs (Fig. 3F).
Lack of FSH-induced terminal follicular maturation is associated with the inefficiency of LH signaling in granulosa cells
When GFs reach the terminal follicular stage in cyclic females, FSH induces LHCGR expression in addition to up-regulating Cyp19a1 expression in granulosa cells; the preovulatory surge in LH then further increases E2 production and leads to the release of EGFR ligands to activate the ovulatory cascade13,33. The dramatic elevation in FSH levels together with the premature maturation of GFs demonstrated by Cyp19a1 expression in preantral/early antral follicles of infantile ovaries led us to seek the effect of FSH on LHCGR expression and functionality during the infantile period. Strikingly, Lhcgr transcripts were not only observed in thecal cells of GFs as expected, but also in granulosa cells from antral follicles (Fig. 4A). Lhcgr expression in granulosa cells disappeared following Ganirelix treatment and was partially restored after eCG supply (Fig. 4A and B). This stimulation of Lhcgr expression by high FSH levels was further demonstrated in vitro in infantile ovaries wherein a high, but not a low, FSH concentration efficiently increased Lhcgr mRNA abundance (Fig. 4C). To assess whether LH signaling was functional in granulosa cells, we examined the effect of hCG on both Cyp19a1 expression and circulating E2 levels in infantile Ganirelix-treated females supplemented or not with eCG. There was no induction in Cyp19a1 expression and no increase in E2 levels in hCG-treated females (Fig. 4D and E). Besides, the expression of Ccnd2, which is negatively regulated by LH in granulosa cells of preovulatory follicles31, was not altered by hCG in Ganirelix-treated females supplemented or not by eCG (Supplementary Fig. 2A). LHCGR signaling was efficient, however, in increasing both the expression of thecal-specific steroidogenic factors and testosterone levels (Supplementary Fig. 2B and C). Overall, these findings suggest that the high FSH levels of the infantile period stimulate granulosa cell differentiation to some extent, but not sufficiently for the follicle to reach the terminal stage of maturation.
Mini-puberty of infancy, which is characterized by the postnatal activation of the hypothalamo-pituitary ovarian (HPO) axis, is a phenomenon common to mouse, rat, monkey, sheep, cow and human1,2,3,5,7,34. The mechanisms underlying the postnatal gonadotropin increments remain unclear; it has been advanced, however, that this postnatal activation results from the abrupt withdrawal of maternal placental estrogens, which exert an inhibitory effect on the HPO axis5. What effect this hypergonadotropic environment has on early ovarian activity had not been clearly analyzed. Using qualitative and quantitative methods in addition to the most reliable approach to measure steroids, i.e., GC-MS, this study is the first to thoroughly analyze the role of FSH in ovarian physiology during the infantile period. Importantly, it demonstrates that high FSH levels permit ovarian steroidogenesis without stimulating follicular growth and allowing terminal follicular maturation. We discovered that it involves a regulatory mechanism whereby high FSH concentrations do not similarly impact the expression or activity of its targets involved in steroid production, follicular growth and maturation.
Our data emphasize previous observations that gonadotropins are already involved in the regulation of ovarian steroidogenesis in postnatal life, prior ‘true’ puberty14,24,35. Besides showing a concomitant increase in pituitary gonadotrope activity and ovarian steroidogenesis, we provide experimental evidence in vitro and in vivo that FSH is responsible for this process. Indeed, high levels of FSH are required to induce Cyp19a1 in granulosa cells of preantral/early follicles from the first follicular waves. The observation of aromatase expression in relatively small GFs in human infant ovaries when FSH levels are elevated suggests that postnatal activation of the pituitary also enhances ovarian steroidogenesis through relatively small GFs in humans. Several studies have suggested that infantile GFs differ from those in adults, their granulosa cells arising from a population of somatic cell precursors that differentiate earlier during fetal life; besides, infantile GFs come from a population of follicles that start growing as soon as they form, at least in rodents27,36,37,38. Given the large number of studies using the infantile ovary as a relevant model of adult ovarian physiology, addressing whether this early FSH responsiveness is unique to infantile GFs or if it could also occur in size-matched follicles in the adult ovary needs to be clarified.
Despite the premature endocrine maturation of GFs and elevated gonadotropin levels, no terminal follicular maturation and no ovulation occur during the infantile period21,26. In the present report, we bring experimental evidence that despite its tremendous increase, FSH does not drive the sequence of events required to achieve these processes, that is follicular growth where granulosa cells proliferate and the antral cavity develops, and then follicular maturation wherein mural granulosa cells become LH-responsive and activate EGFR signaling to trigger ovulation. Our study does not question the fact that FSH is required for basal follicular growth up to the preantral/early antral stage during the infantile period, as shown previously17,18,19,20. But it supports the idea that elevated concentrations of FSH are unable to support subsequent growth of those follicles. Indeed, the experimental decrease of the FSH peak does not impair their number and size, although it affects ovarian production of E2. Conversely, the addition of exogenous gonadotropins to infantile mice is inefficient in stimulating their growth, notwithstanding enhanced E2 production. This treatment becomes efficient in stimulating follicular growth in our mouse colony when circulating FSH has returned to moderate levels, after 21 dpn (data not shown). Our findings are consistent with observations showing that preantral/early antral follicles display a slower growth at 14 dpn than at older prepubertal ages in the mouse26, but in apparent contradiction with a study in mouse models of follicle tracing37. In addition, an inverse relationship has been observed between antral follicle count and FSH levels in ewe lambs during mini-puberty39. Our study may provide some cues to understand why the aberrant elevation of postnatal FSH concentrations for several months following birth in prematurely born infant girls is associated with enhanced E2 levels but with decreased number of antral follicles8,40. It also raises the intriguing possibility that elevated FSH levels in adult patients with premature ovarian failure might be detrimental for follicular growth41.
By investigating the mechanisms underlying the refractoriness of follicular growth to FSH, we discovered that at high levels FSH becomes unable to stimulate cyclin D2-dependent follicular growth. Indeed, our in vitro studies using an organotypic culture system indicate that FSH induces Ccnd2 expression in infantile ovaries only if present at a low, and not at a high concentration in the medium. In vivo, lowering the FSH peak to 20% of its normal value by Ganirelix efficiently restores FSH-induced Ccnd2 expression in the ovary. This is accompanied by an increase in granulosa cell proliferation as shown by higher numbers of phospho-histone H3 and BrdU-positive granulosa cells in preantral/early antral follicles; these two effects are abolished by co-treatment with eCG. The existence of such a regulation in vivo is also suggested by the fall in Ccnd2 expression when circulating FSH rises during the infantile period. We also report here that high FSH concentrations stimulate LHCGR expression in granulosa cells of immature GFs. However, LHCGR signaling is not functional in granulosa cells at this stage, at least in regulating both Cyp19a1 and Ccnd2 expression. Thus, the absence of terminal maturation of GFs would not solely result from the lack of FSH-mediated follicular growth, but also from the inability of granulosa cells to fully differentiate in response to gonadotropin hormones at this stage.
The present report unveils the existence of decoupling in common regulatory pathways of FSH during the infantile period. This is well illustrated by the differential action of high FSH concentrations on the regulation of the expression of Cyp19a1 (strongly induced) and Ccnd2 (no induction) to trigger steroidogenesis while not supporting subsequent follicle growth. The fact that these events can proceed independently is further emphasized by previous studies showing that FSH treatment up-regulates the expression of Cyp19a1 in the ovary of immature Ccnd2−/− mice despite the absence of granulosa cell proliferation31. Since FSH signals through different pathways in addition to that of protein kinase A to selectively regulate target genes in granulosa cells42,43, we hypothesize that high FSH concentrations may stimulate downstream pathways involved in steroidogenesis while shutting down those involved in cell proliferation. Since the oocyte plays a major role in the development of ovarian follicles through the secretion of paracrine factors that regulate proliferation, steroidogenic ability and differentiation of granulosa cells44,45, it would be of interest to determine the possible contribution of the oocyte in the function of the infantile ovary. Overall, our findings establish that elevated FSH levels during the postnatal period essentially induce substantial ovarian endocrine activity by stimulating steroidogenesis with a minimal impact on other processes (Fig. 5). Such a mechanism would ensure E2 supply for the subsequent establishment of reproductive function while preserving the ovary from premature follicular maturation.
All studies were conducted on C57BL/6JRj mice aged 7 to 21 dpn and in adult cycling females that were born at the animal facility from genitors purchased at Janvier Labs (Le Genest St Isle, France). Mice were maintained under controlled conditions (12 h light/dark cycle) with food (Scientific Animal Food and Engineering (SAFE), A03–10) and water available ad libitum. The day of birth was designed as 0 dpn. Vaginal cells from females aged 4 to 6 months were collected by daily saline washes and analyzed after hematoxylin and eosin staining. Stages of the estrous cycle were characterized by predominant nucleated cells, predominant cornified epithelial cells and predominant leukocytes for proestrus (PE), estrus (E) and diestrus 2 (D) stages, respectively. Mice were anesthetized with a mix of ketamine (Imalgene® 1000) and xylazine (Rompun® 2%) to collect the blood by cardiac puncture. Blood was allowed to clot at room temperature for at least 15 minutes, and then centrifuged at 5000 g for 5 minutes to obtain the serum. After cervical dislocation, ovaries were collected, frozen in liquid nitrogen and stored at −80 °C for RNA and protein extraction, or fixed in 4% paraformaldehyde (PFA) for in situ hybridization, or immediately used for organotypic cultures. Experiments were performed in accordance with the ethics guidelines of the French Ministry of Agriculture and were approved by the ethics committee of University Paris 7.
Ten μg of Ganirelix acetate (Orgalutran®, N.V. Organon, Puteaux, France) or saline was subcutaneously injected twice on prepubertal female mice, at 12 and 13 dpn. In addition to Ganirelix, 13 dpn mice received an intraperitoneal injection of either 5 IU of human Chorionic Gonadotropin (hCG) (N.V. Organon), or 5 IU of equine Chorionic gonadotropin (eCG) (N.V.Organon), or saline. Injections (less than 12.5 μl) were performed with Hamilton syringes connected with catheters and needles (Phymep, Paris, France). Mice were then dissected at 14 dpn to collect blood and ovaries. For the superovulation procedure, mice received 5 IU of equine chorionic gonadotropin (eCG) followed 48 hours later by a 5-IU injection of hCG. Females were killed 20 hours later. Their oviducts were retrieved and placed in hyaluronidase in order to visualize any oocyte removed from the ampulla. For BrdU incorporation studies, females received a single injection of 100 mg/kg BrdU the day before dissection.
Determination of serum estradiol levels
Gas chromatography coupled with mass spectrometry (GC-MS) procedure was used to determine the levels of E2 in the serum, as described previously46. After clotting, sera were kept at −80 °C until hormone assays. Randomized serum samples from two to three prepubertal animals were pooled. E2 was assayed in two steps. Additional information can be found in SI Materials and Methods and Table S1.
LH and FSH were simultaneously assayed in 10 μl of serum simplicate from the same serum samples, using the Luminex technology with the rat pituitary magnetic bead panel Milliplex Map kit (Merck-Millipore, Nottingham, UK) in accordance with the manufacturer’s instructions. Samples were run on a Bioplex-200 instrument (Bio-Rad, Marnes-La-Coquette, France) and concentrations were calculated using a five parameter logistic fit curve (5PL) generated from the standards by the Bio-Plex Manager 6.1 software (Bio-Rad, Marnes-La-Coquette, France). The sensitivity of the assays was 32 pg/ml for FSH and 3.2 pg/ml for LH. The inter-assay coefficient of variation was 5.4% for FSH and 3.2% for LH. The intra-assay coefficient of variation was 7.6% for FSH and 5.9% for LH.
Cultures of postnatal ovaries
Ovaries from 12 dpn female mice were placed on cell culture inserts (Millicell #PICM01250, Millipore, Guyancourt, France) on the top of 400 μl of culture media containing RPMI without red phenol, fetuin (Sigma, #F2379), insulin (Sigma, #I0516), transferrin (Sigma, #T8158), sodium selenite (Sigma, #S5261) and BSA (Euromedex, Souffelweyersheim, France) in 24-well plates for 24 hours. Then, the culture medium was replaced with 400 μl of fresh medium containing purified ovine pituitary FSH (50, 200 or 500 ng/ml) provided by Dr R. Counis (University Paris-Diderot, France). After 8 hours of gonadotropin treatment, ovaries were snap-frozen in liquid nitrogen and stored at −80 °C for RNA extraction.
RNA extraction, reverse transcription and quantitative real-time PCR
Single frozen ovaries were lysed with TissueLyser (Qiagen, Courtaboeuf, France) in RLT buffer from RNeasy mini kit (#74106, Qiagen), following manufacturer’s protocol. The extraction of total RNA was performed on columns and eluted with 30 μl of sterile water. The concentration and the quality of RNAs were assessed by the ratio of 260/230 nm and 260/280 nm with the Nanodrop device (Thermo Scientific, France). Total RNA (100 to 200 ng) was reverse transcribed with Superscript II (Invitrogen, Cergy Pontoise, France) and random primers (Invitrogen) following manufacturer’s instructions. Primers used for quantitative real-time PCR are listed in Table S2. Hprt was used as a reference gene to normalize the data. Real-time PCR was performed with Lightcycler® 480 SYBR Green I Master (Roche Molecular Biochemicals, La Rochelle, France) and Light Cycler instrument (Roche) as previously described47.
In situ hybridization
Ovaries were collected and fixed for 1–2 hours in 4% PFA, rinsed in PBS and placed in 18% sucrose before being embedded in Optimal Cutting Temperature (OCT) (Cellpath, Newtown, UK). In situ hybridization was performed on frozen sections with digoxigenin-11-UTP labelled RNA probes, as previously described25,47.
Tissue processing and immunohistochemistry
For histological examination of mouse ovarian morphology and follicle counts, ovaries were fixed in 4% paraformaldehyde for at least 1 h, dehydrated in alcohol, and paraffin-embedded using standard protocols. Sections of 7-μm thickness were mounted on glass slides and stained with hematoxylin and eosin. Only follicles at the preantral/early antral stage (several layers of granulosa cells and diffuse or small antral cavities) located in the central part of the ovary were considered. Their number and surface was analyzed in every fifth histological section by ImageJ (ImageJ 1.64; Wayne Rasband, NIH). Immunostaining of Serine 10 phosphorylated histone H3 (Cell Signaling Technology, #9701) and BrdU (#ab152095, Abcam) was performed as described48,49. Counting of BrdU and P-HH3-positive granulosa cells in preantral/early antral follicles was performed using ImageJ. Immunostaining for fibronectin (Sigma, #086K4803) and cyclin D2 (Santa-Cruz biotechnologies, sc-593) was performed on frozen mouse ovarian sections, as previously reported47.
Formalin-fixed paraffin-embedded ovaries from girls aged from 2 to 6 postnatal months dying suddenly and unexpectedly in the hospital-university of Rennes were accrued under the French autopsy law that allows the use of such tissues for in-depth anatomopathological examination (Law 94–654 published on 29 July 1994). Autopsy was performed with informed consent of the parents in all cases. Adult human ovaries were provided by the Laboratory of Pathology of Gustave Roussy Institute (Villejuif, France) following prophylactic removal due to breast cancer between 1975 and 1980 with informed consent was obtained by the patients. These methods were carried out in accordance with relevant guidelines and regulations. All the experiments and experimental protocols on human subjects were approved by the institutional committee of the French agency for biomedical research (Agence de la Biomédecine, Saint-Denis la Plaine, France). Adult ovaries did not present any pathological aspect, showing corpora lutea at various stages of regression compatible with at least three successive ovulatory cycles. Immunohistochemistry was performed as previously described48. Slides were incubated overnight with primary antibodies for AMH (generously provided by Dr JY Picard) and aromatase (Sigma, #A7981). They were counterstained in hematoxylin, dehydrated and mounted in Permount (Fisher Scientific).
Pooled (n = 2 ovaries at 7 dpn) or single frozen ovaries were lysed with TissueLyser (Qiagen) in Frackelton buffer (10 mM Tris HCl, 50 mM NaCl, 1% Triton, 30 mM NaPPi, 50 mM NaF, 5 μM ZnCl2, 100 μM Na3VO4, 1 mM DTT, 1X protease inhibitor (Roche), 1X phosphatase inhibitor [Thermo Scientific]). After a 30-minute incubation on ice, lysates were centrifuged at maximal speed for 30 minutes, and supernatants were collected. Thirty μg of lysates were used for the determination of aromatase (Sigma, #A7981), cyclin D2 (Santa-Cruz, #sc-181) and GAPDH (Santa-Cruz, #sc-25778). Membranes were incubated in 10% milk for 60 minutes and incubated overnight with primary antibodies at 4 °C. The following day, the membrane was incubated with an anti-rabbit HRP-linked IgG antibody (dilution: 1/3000) for 2 h. Proteins were detected by chemiluminescence with ECL using CCD camera (LAS 4000, FujiFilm).
All data were analyzed by Prism 6 (version 6.0, GraphPad Software). Statistical analyses were performed with the use of Student t-test or one-way ANOVA depending on the experimental setting. Data are shown as means ± SEM. A P value < 0.05 was considered as significant.
How to cite this article: François, C. M. et al. A novel action of follicle-stimulating hormone in the ovary promotes estradiol production without inducing excessive follicular growth before puberty. Sci. Rep. 7, 46222; doi: 10.1038/srep46222 (2017).
Publisher's note: Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.
Döhler, K. D. & Wuttke, W. Changes with age in levels of serum gonadotropins, prolactin and gonadal steroids in prepubertal male and female rats. Endocrinology 97, 898–907 (1975).
Winter, J. S., Faiman, C., Hobson, W. C., Prasad, A. V. & Reyes, F. I. Pituitary-gonadal relations in infancy. I. Patterns of serum gonadotropin concentrations from birth to four years of age in man and chimpanzee. J. Clin. Endocrinol. Metab. 40, 545–551 (1975).
Dullaart, J., Kent, J. & Ryle, M. Serum gonadotrophin concentrations in infantile female mice. J. Reprod. Fertil. 43, 189–192 (1975).
Chellakooty, M. et al. Inhibin A, inhibin B, follicle-stimulating hormone, luteinizing hormone, estradiol, and sex hormone-binding globulin levels in 473 healthy infant girls. J. Clin. Endocrinol. Metab. 88, 3515–3520 (2003).
Kuiri-Hänninen, T., Sankilampi, U. & Dunkel, L. Activation of the hypothalamic-pituitary-gonadal axis in infancy: minipuberty. Horm. Res. Pædiatrics 82, 73–80 (2014).
Bergadá, I. et al. Time course of the serum gonadotropin surge, inhibins, and anti-Müllerian hormone in normal newborn males during the first month of life. J. Clin. Endocrinol. Metab. 91, 4092–4098 (2006).
Rawlings, N. C., Evans, A. C. O., Honaramooz, A. & Bartlewski, P. M. Antral follicle growth and endocrine changes in prepubertal cattle, sheep and goats. Anim. Reprod. Sci. 78, 259–270 (2003).
Kuiri-Hänninen, T. et al. Postnatal ovarian activation has effects in estrogen target tissues in infant girls. J. Clin. Endocrinol. Metab. 98, 4709–4716 (2013).
Rey, R. A. Mini-puberty and true puberty: differences in testicular function. Ann. Endocrinol. 75, 58–63 (2014).
Brock, O., Baum, M. J. & Bakker, J. The development of female sexual behavior requires prepubertal estradiol. J. Neurosci. Off. J. Soc. Neurosci. 31, 5574–5578 (2011).
Clarkson, J., Boon, W. C., Simpson, E. R. & Herbison, A. E. Postnatal development of an estradiol-kisspeptin positive feedback mechanism implicated in puberty onset. Endocrinology 150, 3214–3220 (2009).
Stewart, J. & Cygan, D. Ovarian hormones act early in development to feminize adult open-field behavior in the rat. Horm. Behav. 14, 20–32 (1980).
Richards, J. S. & Pangas, S. A. The ovary: basic biology and clinical implications. J. Clin. Invest. 120, 963–972 (2010).
Fortune, J. E. & Eppig, J. J. Effects of gonadotropins on steroid secretion by infantile and juvenile mouse ovaries in vitro . Endocrinology 105, 760–768 (1979).
White, S. S. & Ojeda, S. R. Changes in ovarian luteinizing hormone and follicle-stimulating hormone receptor content and in gonadotropin-induced ornithine decarboxylase activity during prepubertal and pubertal development of the female rat. Endocrinology 109, 152–161 (1981).
O’Shaughnessy, P. J., McLelland, D. & McBride, M. W. Regulation of luteinizing hormone-receptor and follicle-stimulating hormone-receptor messenger ribonucleic acid levels during development in the neonatal mouse ovary. Biol. Reprod. 57, 602–608 (1997).
Kumar, T. R., Wang, Y., Lu, N. & Matzuk, M. M. Follicle stimulating hormone is required for ovarian follicle maturation but not male fertility. Nat. Genet. 15, 201–204 (1997).
McGee, E. A., Perlas, E., LaPolt, P. S., Tsafriri, A. & Hsueh, A. J. Follicle-stimulating hormone enhances the development of preantral follicles in juvenile rats. Biol. Reprod. 57, 990–998 (1997).
Balla, A., Danilovich, N., Yang, Y. & Sairam, M. R. Dynamics of ovarian development in the FORKO immature mouse: structural and functional implications for ovarian reserve. Biol. Reprod. 69, 1281–1293 (2003).
Hardy, K. et al. Onset and Heterogeneity of Responsiveness to FSH in Mouse Preantral Follicles in Culture. Endocrinology en20161435, doi: 10.1210/en.2016-1435 (2016).
Lintern-Moore, S., Peters, H., Moore, G. P. & Faber, M. Follicular development in the infant human ovary. J. Reprod. Fertil. 39, 53–64 (1974).
Peters, H., Byskov, A. G., Himelstein-Braw, R. & Faber, M. Follicular growth: the basic event in the mouse and human ovary. J. Reprod. Fertil. 45, 559–566 (1975).
Mahdi, D. & Khallili, K. Relationship between follicle growth and circulating gonadotrophin levels during postnatal development of sheep. Anim. Reprod. Sci. 106, 100–112 (2008).
Weniger, J. P., Zeis, A. & Chouraqui, J. Estrogen production by fetal and infantile rat ovaries. Reprod. Nutr. Dev. 33, 129–136 (1993).
Guigon, C. J. et al. Unaltered development of the initial follicular waves and normal pubertal onset in female rats after neonatal deletion of the follicular reserve. Endocrinology 144, 3651–3662 (2003).
Pedersen, T. Follicle growth in the immature mouse ovary. Acta Endocrinol. (Copenh.) 62, 117–132 (1969).
Hirshfield, A. N. & DeSanti, A. M. Patterns of ovarian cell proliferation in rats during the embryonic period and the first three weeks postpartum. Biol. Reprod. 53, 1208–1221 (1995).
Suzuki, T., Sasano, H., Sasaki, H., Fukaya, T. & Nagura, H. Quantitation of P450 aromatase immunoreactivity in human ovary during the menstrual cycle: relationship between the enzyme activity and immunointensity. J. Histochem. Cytochem. Off. J. Histochem. Soc. 42, 1565–1573 (1994).
Cohen, H. L., Eisenberg, P., Mandel, F. & Haller, J. O. Ovarian cysts are common in premenarchal girls: a sonographic study of 101 children 2-12 years old. AJR Am. J. Roentgenol. 159, 89–91 (1992).
Sicinski, P. et al. Cyclin D2 is an FSH-responsive gene involved in gonadal cell proliferation and oncogenesis. Nature 384, 470–474 (1996).
Robker, R. L. & Richards, J. S. Hormone-induced proliferation and differentiation of granulosa cells: a coordinated balance of the cell cycle regulators cyclin D2 and p27Kip1. Mol. Endocrinol. Baltim. Md 12, 924–940 (1998).
Hendzel, M. J. et al. Mitosis-specific phosphorylation of histone H3 initiates primarily within pericentromeric heterochromatin during G2 and spreads in an ordered fashion coincident with mitotic chromosome condensation. Chromosoma 106, 348–360 (1997).
El-Hayek, S., Demeestere, I. & Clarke, H. J. Follicle-stimulating hormone regulates expression and activity of epidermal growth factor receptor in the murine ovarian follicle. Proc. Natl. Acad. Sci. USA 111, 16778–16783 (2014).
Meijs-Roelofs, H. M., Uilenbroek, J. T., de Jong, F. H. & Welschen, R. Plasma oestradiol-17beta and its relationship to serum follicle-stimulating hormone in immature female rats. J. Endocrinol. 59, 295–304 (1973).
Gray, S. A., Mannan, M. A. & O’Shaughnessy, P. J. Development of cytochrome P450 aromatase mRNA levels and enzyme activity in ovaries of normal and hypogonadal (hpg) mice. J. Mol. Endocrinol. 14, 295–301 (1995).
Mork, L. et al. Temporal differences in granulosa cell specification in the ovary reflect distinct follicle fates in mice. Biol. Reprod. 86, 37 (2012).
Zheng, W. et al. Two classes of ovarian primordial follicles exhibit distinct developmental dynamics and physiological functions. Hum. Mol. Genet. 23, 920–928 (2014).
Anderson, R. A., McLaughlin, M., Wallace, W. H. B., Albertini, D. F. & Telfer, E. E. The immature human ovary shows loss of abnormal follicles and increasing follicle developmental competence through childhood and adolescence. Hum. Reprod. Oxf. Engl. 29, 97–106 (2014).
Torres-Rovira, L. et al. Postnatal pituitary and follicular activation: a revisited hypothesis in a sheep model. Reprod. Camb. Engl. 151, 215–225 (2016).
Kuiri-Hänninen, T. et al. Postnatal developmental changes in the pituitary-ovarian axis in preterm and term infant girls. J. Clin. Endocrinol. Metab. 96, 3432–3439 (2011).
Tartagni, M. et al. Effects of pretreatment with estrogens on ovarian stimulation with gonadotropins in women with premature ovarian failure: a randomized, placebo-controlled trial. Fertil. Steril. 87, 858–861 (2007).
Hunzicker-Dunn, M. & Maizels, E. T. FSH signaling pathways in immature granulosa cells that regulate target gene expression: branching out from protein kinase A. Cell. Signal. 18, 1351–1359 (2006).
Gloaguen, P., Crépieux, P., Heitzler, D., Poupon, A. & Reiter, E. Mapping the follicle-stimulating hormone-induced signaling networks. Front. Endocrinol. 2, 45 (2011).
Eppig, J. J. Oocyte control of ovarian follicular development and function in mammals. Reprod. Camb. Engl. 122, 829–838 (2001).
Guigon, C. J. & Magre, S. Contribution of germ cells to the differentiation and maturation of the ovary: insights from models of germ cell depletion. Biol. Reprod. 74, 450–458 (2006).
Giton, F. et al. Evidence of estrone-sulfate uptake modification in young and middle-aged rat prostate. J. Steroid Biochem. Mol. Biol. 152, 89–100 (2015).
Vandormael-Pournin, S. et al. Oocyte-specific inactivation of Omcg1 leads to DNA damage and c-Abl/TAp63-dependent oocyte death associated with dramatic remodeling of ovarian somatic cells. Cell Death Differ. 22, 108–117 (2015).
Guigon, C. J., Fozzatti, L., Lu, C., Willingham, M. C. & Cheng, S.-Y. Inhibition of mTORC1 signaling reduces tumor growth but does not prevent cancer progression in a mouse model of thyroid cancer. Carcinogenesis 31, 1284–1291 (2010).
Léguillier, T. et al. Omcg1 is critically required for mitosis in rapidly dividing mouse intestinal progenitors and embryonic stem cells. Biol. Open 1, 648–657 (2012).
The authors wish to thank the following investigators for providing reagents: Dr S. Mazaud-Guittot (IRSET, Rennes), Dr P. Loget (Service d’anatomopathologie, CHU de Rennes), Drs N. Di Clemente, J.Y. Picard and R. Counis (University Paris 7). They acknowledge the technical assistance of M. Surenaud for gonadotropin assays (Hopital Henri Mondor, France), S. Vandormael-Pournin for the superovulation procedure (Institut Pasteur, France), N. Coudouel for tissue sectioning and all the technicians of the Buffon animal facility (University Paris Diderot, France) who contributed to this work. The authors also thank Dr S. Bouret (Institut du Cerveau et de la Moelle, France) and Dr V. Simon (University Paris Diderot) for valuable discussions on this project. This work was funded by ‘Institut National de la Santé et de la Recherche Medicale’ (Inserm), by the ‘Centre National de la Recherche Scientifique’ (CNRS), and by University Paris Diderot. CMF was the recipient of a fellowship from Ecole Doctorale Bio-SPC (University Paris Diderot).
The authors declare no competing financial interests.
About this article
Cite this article
François, C., Petit, F., Giton, F. et al. A novel action of follicle-stimulating hormone in the ovary promotes estradiol production without inducing excessive follicular growth before puberty. Sci Rep 7, 46222 (2017). https://doi.org/10.1038/srep46222
Paediatric and Perinatal Epidemiology (2021)
Multistep analysis reveals the relationship between blood indices at the time of ovum pick-up and in vitro embryo production in heifers
Molecular and Cellular Endocrinology (2021)
Effects of human chorionic gonadotropin and gonadotropin releasing hormone analogue on plasma steroid hormones and spawning performances in golden rabbitfish Siganus guttatus
Journal of Applied Ichthyology (2020)
New markers for regulation of transcription and macromolecule metabolic process in porcine oocytes during in vitro maturation
Molecular Medicine Reports (2020)