In rodents, in utero exposure to exogenous estrogens including diethylstilboestrol (DES) results in major suppression of steroidogenesis in fetal testes. Whether similar effects occur in the human fetal testis is equivocal. Based on the results of the rodent studies, we hypothesised that exposure of human fetal testes to DES would result in a reduction in testosterone production. We show, using a xenograft approach, that testosterone production is not reduced in human fetal testis following DES exposure. Human fetal testes (15–19 weeks’ gestation, n = 6) were xenografted into castrate male nude mice which were then treated for 35 days with vehicle or 100 µg/kg DES three times a week. For comparison, similar treatment was applied to pregnant rats from e13.5–e20.5 and effects on fetal testes evaluated at e21.5. Xenograft testosterone production was assessed by measuring host seminal vesicle (SV) weights as an indirect measure over the entire grafting period, and single measurement of serum testosterone at termination. Human fetal testis xenografts showed similar survival in DES and vehicle-exposed hosts. SV weight (44.3 v 26.6 mg, p = 0.01) was significantly increased in DES compared to vehicle-exposed hosts, respectively, indicating an overall increase in xenograft testosterone production over the grafting period, whilst serum testosterone at termination was unchanged. In contrast intra-testicular testosterone levels were reduced by 89%, in fetal rats exposed to DES. In rats, DES effects are mediated via Estrogen Receptor α (ESR1). We determined ESR1 protein and mRNA expression in human and rat fetal testis. ESR1 was expressed in rat, but not in human, fetal Leydig cells. We conclude that human fetal testis exposure to DES does not impair testosterone production as it does in rats, probably because ESR1 is not expressed in human fetal Leydig cells. This indicates that DES exposure is likely to pose minimal risk to masculinization of the human fetus.
Citation: Mitchell RT, Sharpe RM, Anderson RA, McKinnell C, Macpherson S, Smith LB, et al. (2013) Diethylstilboestrol Exposure Does Not Reduce Testosterone Production in Human Fetal Testis Xenografts. PLoS ONE 8(4): e61726. doi:10.1371/journal.pone.0061726
Editor: Jean-Marc A. Lobaccaro, Clermont Université, France
Received: January 16, 2013; Accepted: March 11, 2013; Published: April 19, 2013
Copyright: © 2013 Mitchell et al. This is an open-access article distributed under the terms of the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original author and source are credited.
Funding: This work was supported in part by Grants G1100358 (RMS) and G1100357 (RAA) from the Medical Research Council and research awards from the British Society for Paediatric Endocrinology and Diabetes, and from the Academy of Medical Sciences (both RTM). The funders had no role in study design, data collection and analysis, decision to publish, or preparation of the manuscript.
Competing interests: The authors have declared that no competing interests exist.
Male reproductive disorders (cryptorchidism, hypospadias, testicular germ cell cancer, low sperm counts) are common and some have increased significantly in incidence in recent decades, raising concern about the role that lifestyle/environmental factors play in their etiology . It has been proposed that these disorders are components of a ‘Testicular Dysgenesis Syndrome’ (TDS) with a common origin in fetal life . Suppression of testosterone production resulting in abnormal testis development/function during fetal life has been implicated in the development of the TDS disorders , , , . What remains unclear is what lifestyle/environmental factors could affect human fetal testis development/function and give rise to these disorders.
Twenty years ago the so-called ‘estrogen hypothesis’ was proposed which suggested that the increasing incidence of reproductive abnormalities in the human male may be related to increased estrogen exposure in . This hypothesis was supported by a number of studies in pregnant rats exposed to the synthetic estrogen DES and by some epidemiological data in male offspring of mothers exposed in utero to DES . Male offspring of rats exposed in utero to DES demonstrated gross suppression of testosterone , . Studies in estrogen receptor-1 knockout (ERKO) mice have shown that the effects of DES are mostly mediated through classical estrogen signalling pathways involving ESR1 .
During the 1940’s–1970’s DES (~60–70 µg/kg/d) was administered to pregnant women to prevent miscarriage and was reported to result in an increased incidence of reproductive tract abnormalities in both male and female offspring , . However, other studies of the consequences of exogenous estrogen exposure in human pregnancy, including detailed meta-analyses, have largely failed to provide support for the estrogen hypothesis-TDS relationship in humans , , , . Moreover, some studies have indicated that ESR1 is not expressed in human fetal Leydig cells , .
In view of the previous lack of a human relevant system in which to investigate the effects of in utero exposure to estrogens, there remains uncertainty about the risk that environmental estrogens pose to masculinization of the human male . We hypothesised that exposure of human fetal testis to DES results in a reduction in testosterone production as it does in rats and mice. We have validated a xenograft system to determine the effects of exposure to environmental chemicals on the human fetal testis . The system involves grafting human fetal testis tissue into immune-compromised castrate mice, where it grows and develops normally for prolonged periods (6+ weeks) . Treatment with hCG during the grafting period to mimic normal in utero exposure, maintains Leydig cell steroidogenesis and thus stimulates growth of the host seminal vesicle, reflecting testosterone production from the xenografts over the duration of the grafting period . The xenograft model more effectively recapitulates the normal situation in pregnancy, without the reservations about in vitro and indirect approaches and as a result has the potential to provide a more ‘physiological’ system in which to evaluate the effects of exposure to estrogens on human fetal testis testosterone production. This was the aim of the present studies.
For all studies, animals were treated humanely and with regard for alleviation of suffering. Studies were performed according to the Animal (Scientific Procedures) Act 1986 following specific approval by the UK Home Office. Studies were conducted under an approved Project Licence (PPL 60/3914) following review by the University of Edinburgh Animal Research Ethics Committee. In order to obtain human fetal testes, women undergoing elective termination gave written consent in accordance with UK national guidelines , and ethical approval for this study was obtained from the Lothian Research Ethics Committee (LREC - 08/S1101/1).
Human Fetal Testes and the Xenografting Procedure
Second trimester (15–19 weeks, n = 6) human fetal testes were obtained following elective termination of pregnancy. No terminations were due to fetal abnormalities. A small portion of each testis was fixed as a pre-graft control, whilst the remainder was placed immediately into ice-cold media containing Liebowitz L-15 with glutamine, 10% fetal bovine serum, 1% penicillin/streptomycin and 1% non-essential amino acids (all Sigma, Poole, UK) for xenografting. Male CD1 nude mice (aged 4–6 weeks, n = 30; Charles River UK, Margate, England) were anesthetised by inhalation of isofluorane, and castrated. After a recovery period of 1–2 weeks, small pieces (1 mm3 approx.) of donor testis tissue were inserted subcutaneously under the dorsal skin using a 13G cancer implant needle (Popper and Sons, New York, US). Grafts (5–6 per mouse) were inserted on either side of the midline. Mice were housed individually and received analgesia (Carprofen; Pfizer, New York, USA) and antibiotics (Enrofloxacin; Bayer, Germany) in the drinking water for 5 days post-surgery. In general, 4–6 mice were xenografted with tissue from each fetus and half of these mice were then allocated to vehicle+hCG treatment and half to DES+hCG treatment.
Treatments of Host Mice
Host mice receiving xenografts from human fetal testis tissue were injected subcutaneously every 72 h with 20 IU hCG (Pregnyl, Organon Laboratories, Cambridge, UK) in 0.9% (w/v) saline containing 1% (v/v) fetal bovine serum, which has been shown to be required to maintain testosterone production by the xenografts and reflects the high levels of hCG in human pregnancy . Host mice were treated by subcutaneous injection with either vehicle (corn oil) or 100 µg/kg DES (Sigma, Poole, Dorset) diluted in corn oil. In xenografted host mice, all treatments commenced 7 days after grafting and continued 3 times a week until the end of the grafting period (~5 weeks). Ungrafted castrate mice (n = 6) were also treated with either DES or vehicle as above in order to provide baselines for seminal vesicles and testosterone and to ensure that any effects of the treatment were specific to the human fetal testis xenografts. The dose and treatment regimen for DES was based on studies by ourselves (see below and ) and others , which showed major suppression of intratesticular testosterone in fetal rats and mice using this regimen.
Retrieval of Xenografts
Xenografts of human fetal testis were retrieved after 6 weeks. Host mice were killed by cervical dislocation and blood obtained by cardiac puncture for measurement of testosterone. Seminal vesicles were removed and weighed and xenografts were retrieved, weighed and fixed for 2 h in Bouin’s fixative, before being transferred to 70% (v/v) ethanol and then processed into paraffin blocks.
Fetal Rat Studies
Wistar rats were maintained according to UK Home Office guidelines and were fed a soy-free breeding diet (RM3(E) soya free; SDS, Dundee, Scotland). Housing conditions were carefully controlled (lights on at 0700, off at 1900 h, temperature 19–21°C, GOLD shavings and LITASPEN standard bedding (SPPS, Argenteuil, France)). Time-mated female rats were injected subcutaneously with DES (Sigma-Aldrich) at a dose of 100 µg/kg in 1 ml/kg corn oil on e13.5, e15.5, e17.5, e19.5 and e20.5. Rat dams were killed on e21.5 by inhalation of CO2 followed by cervical dislocation. Fetuses were removed, decapitated and placed in ice cold phosphate buffered saline (PBS; Sigma-Aldrich). Testes were microdissected, and fixed in Bouin’s fixative for 1 h at room temperature or snap frozen and stored at −70°C for gene expression analysis or determination of intratesticular testosterone (ITT). For the latter, the testis was homogenized and its total testosterone content determined after extraction and measurement as described below. Bouin’s-fixed tissues were processed and embedded in paraffin wax, and 5 µm sections were cut and used for immunohistochemistry.
Xenograft host serum testosterone levels and rat fetal intra-testicular testosterone levels were measured at termination by competitive radioimmunoassay using an in-house radioimmunoassay method described previously . The method used radiolabelled testosterone (I125, MP Biomedicals, UK) and a rabbit primary antibody (1:600,000; AMS Biotech, Abingdon, UK). Residual I125 was measured with a gamma counter (WIZARD 1470, Perkin Elmer, Turku, Finland) and testosterone levels were expressed as ng/ml (human xenografts) or pg/testis (rat fetal testis). All samples were analysed in a single assay, the detection limit for which was 45 pg/ml and the intra-assay CV was 8%.
Immunohistochemistry was performed on human fetal testis tissue (ungrafted, n = 5; vehicle-exposed grafts, n = 3; DES-exposed grafts, n = 3), human adult endometrium obtained at endometrial biopsy (n = 1) and rat fetal testis (n = 3) as previously described . Sections (5 µm) were subjected to heat induced antigen retrieval in 0.01 M citrate buffer (pH 6), and endogenous peroxidase blocked with 3% (v/v) H2O2 in methanol for 30 min. Endogenous biotin was blocked using an avidin/biotin blocking kit (Vector Laboratories Inc., Peterborough, UK), according to manufacturer’s instructions. Sections were incubated in normal rabbit serum diluted 1:5 with TBS containing 5% (w/v) BSA for 30 min. Sections were incubated overnight with primary antibody (ESR1, mouse anti-human 1:50; Vector Laboratories, Peterborough, UK) diluted in serum at 4°C in a humidified chamber and then incubated for 30 min with a biotinylated secondary antibody (rabbit anti-mouse; DAKO, Ely, Cambridgeshire, UK) at 1:500, diluted in normal serum/TBS/BSA, followed by 30 min incubation with Streptavidin-HRP (DAKO) at 1:1000, diluted in TBS. Visualization was performed using 3,3-diaminobenzidine tetrahydrochloride (DAB, DAKO) and sections were counterstained with hematoxylin before mounting in Pertex mounting medium (CellPath plc, Hemel Hempstead, UK). Negative controls were sections in which the primary antibody was replaced with the appropriate normal serum/TBS/BSA. Images were captured as previously described .
Gene Expression Analysis
For quantitative analysis of gene expression by RT-PCR, total RNA was extracted from pre-graft control human fetal testis samples (n = 3) and adult human endometrium obtained at endometrial biopsy (n = 1) using the RNeasy Micro Kit with on-column DNase digestion (Qiagen, UK). Random hexamer primed cDNA was prepared using the Applied Biosystems Taqman™ RT kit (Applied Biosystems, CA). Quantitative real time PCR (qRT-PCR) was performed on the ABI Prism Sequence Detection System (Applied Biosystems). Expression of human ESR1 was determined using the Roche Universal Probe Library (human ESR1 forward primer 5′-AACCAGTGCACCATTGATAAAA-3′, reverse primer 5′-TCCTCTTCGGTCTTTTCGTATC-3′, probe number 69 Cat no. 04688686001; Roche Applied Sciences, Burgess Hill, UK). The expression level of human ESR1 was corrected using 18S ribosomal RNA as internal control (Applied Biosystems Cat no. 4308329). All samples were performed in triplicate for 3 separate fetuses (14–19 weeks old) and a relative comparison was made to human adult endometrium for ESR1.
Statistical analysis was performed using Graphpad Prism 5 software (La Jolla, California USA). Results were analysed using paired t-test with Bonferroni post-hoc test. For human fetal testis xenografts data were also analysed by two-way ANOVA to take account of the variation between replicate grafts (ie grafts from the same fetus but into separate hosts that then receive comparable treatment) and between individual fetuses. Data for fetal ITT and mRNA levels were log transformed prior to analysis to normalise variances.
Xenograft Retrieval from Vehicle- and DES-exposed Mice
At the end of the xenografting period, grafts were easily identified and retrieved from the subcutaneous tissue. The majority of the 182 grafts were retrieved at the end of the grafting period with no difference between vehicle or DES-exposed groups (78 v 70% retrieval, p>0.05; Fig. 1A). Total recovered graft weight per mouse was almost identical for vehicle- and DES-exposed groups (6.98 v 6.99 mg; Fig. 1B).
A) Graft survival (%). B) Total graft weight (mg). Data analysed by unpaired t-test; Mean ± SEM for n = 15, p>0.05.
Effect of Exposure to DES on Testosterone Production by Xenografts
To determine the effect of exposure to DES on testosterone production from the xenografts, serum testosterone and seminal vesicle weight were measured in the host animals. Unexpectedly, seminal vesicle weight was significantly increased in the DES-exposed hosts compared to vehicle (26.6 v 44.3 mg, p = 0.002; Fig. 2A). Serum testosterone levels at termination were not significantly different in the DES-exposed hosts compared to vehicle (0.33 v 0.51 ng/ml, p>0.05; Fig. 2B). There was variation between individual fetuses for baseline seminal vesicle weight (Fig. 2C) and serum testosterone (Fig. 2D) and therefore two-way ANOVA was performed to take into account this variation. In order to ensure that these results were due to effects on the xenografts and not the host animal, we measured seminal vesicle weight and serum testosterone in ungrafted mice. There was no effect of DES on seminal vesicle weight or serum testosterone in ungrafted control mice (Fig. 2A,B)).
Seminal vesicle weight A) and serum testosterone B) in ungrafted (n = 6) and xenografted (n = 15) mice. Mean ± SEM. Bars with letters in common are not significantly different. Data analysed by unpaired t-test. Base-line variation in seminal vesicle weight C) and serum testosterone D) for host mice xenografted with individual fetuses (n = 6). Mean ± SEM. Data analysed by two-way ANOVA.
To compare the results obtained for the human fetal testis with those in the rat, we exposed pregnant rats to DES (n = 4) or vehicle (n = 3) from e13.5– e20.5 and intratesticular testosterone was determined at e21.5; because of the small blood volume of e21.5 fetuses it was not feasible to measure blood levels of testosterone. There was a significant overall decrease (89%) in intratesticular testosterone in DES-exposed fetal rat testes compared to vehicle-exposed controls (260.2 v 29.1 pg/testis, p<0.001; Fig. 3). This finding was consistent between litters with a significant reduction in ITT in all DES-exposed litters compared with controls.
Data is presented as litter means (unpaired t-test, p = 0.004).
ESR1 Expression in the Fetal Testis of Human and Rat
The effects of DES in rodents have been shown to be mediated through ESR1 signalling . We compared ESR1 expression in control fetal human testis (n = 3) with that of rat. ESR1 mRNA was barely detectable in the human fetal testis (Fig. 4A). Human fetal testis exhibited 175-fold lower mRNA expression compared with human adult endometrium. Immunoexpression of ESR1 protein was not detected in the Leydig cells of the human fetal testis (Fig. 4B). In addition no expression was identified in either vehicle-exposed or DES-exposed xenografts (not shown). In contrast, in rats, there was clear immunoexpression in fetal rat Leydig cells (Fig. 4C). As a positive control ESR1 protein expression was detected in the human endometrium demonstrating the specificity of this antibody in human tissue (Fig. 4B, inset).
A) Relative ESR1 mRNA expression in adult human endometrium compared with human fetal testis (n = 3). w = weeks. Note: data presented on a log-scale. ESR1 protein expression in B) a 20 week gestation ungrafted human fetal testis and human endometrium (positive control; inset.) and C) e21.5 rat fetal testis. SC = seminiferous cords, arrows indicate Leydig cells. Original magnification 20×. Scale bar = 50 µm.
The original ‘estrogen hypothesis’  proposed that the increase in male reproductive abnormalities (testis cancer, cryptorchidism, hypospadias, low sperm counts) over recent decades might have occurred because of increased exposure to estrogens from various potential sources. Subsequent studies in rats and mice that involved manipulation of fetal estrogen exposure confirmed that supranormal estrogen exposure could act on steroidogenic pathways that can underlie male reproductive disorders , , . However, direct evidence of an effect of DES on the human fetal testis has so far been lacking. The present studies aimed to determine the effect of exposure to DES on testosterone production by the human fetal testis using a xenograft approach, shown to recapitulate normal human fetal testis development and to be a useful model in which to determine the effects of exposure to proposed ‘endocrine disruptors’ , .
The present studies have demonstrated that exposure to DES, given at a dose in the equivalent range to previous clinical use (100 µg/kg three times a week), does not lead to any detectable reduction in testosterone production/action by second trimester human fetal testis xenografts. In fact we found a significant increase in seminal vesicle weight in xenografted host mice exposed to DES, indicating an increase in overall testosterone production from the xenografts during the grafting period, although there was no significant difference in single measurements of serum testosterone concentration at the time of graft recovery. The increase in seminal vesicle weight is unexplained and requires further study. In non-castrate adult mice exposed to DES, seminal vesicle weights are reported to decrease . We have ruled out the possibility that a direct action of DES on the mouse seminal vesicles is causing the increase in seminal vesicle weight by exposing ungrafted castrate mice to DES and found no difference, therefore the increase in seminal vesicle weight in xenografted mice must involve the human fetal testis. Our results do not rule out the possibility that DES can affect testosterone production via indirect mechanisms that involve effects on the placenta or the fetal brain, however we consider it unlikely that the increased testosterone production is being stimulated centrally via the hypothalamo-pituitary-gonadal axis, given that high gonadotrophin levels induced by castration of the host animal have been shown to result in low (baseline) levels of testosterone production from the xenografts in the absence of exogenous hCG .
DES has been shown to exert its major adverse effects mainly through classical estrogen receptor signalling, in particular via ESR1 , . In a mouse fetal testis organ culture system the reduction in testosterone production that occurred following DES exposure in wild-type testes did not occur in ESR1 deficient mice . Given that the effects in mice are mediated by ESR1 we examined the expression of ESR1 in the human fetal testis and did not detect expression of this protein in fetal Leydig cells, consistent with previous findings , . However, we confirmed that ESR1 expression was present in fetal rat Leydig cells; this difference offers a straightforward explanation for the differential sensitivity of fetal Leydig cells in terms of testosterone production following DES-exposure in rodents versus the human. It also indicates that any stimulatory effects on testosterone production in human fetal testes are likely to be mediated via an alternative estrogen signalling pathway. This is supported by evidence for actions of DES involving alternative pathways, such as the estrogen-related receptors  and/or the orphan receptor Nr0b2 .
We confirmed that exposure of the fetal rat testis to the same DES treatment regimen resulted in ~90% reduction in fetal intra-testicular testosterone , . As a reduction in testosterone production by the fetal testis is widely viewed as being the most likely mechanism for the origin of TDS disorders, the present findings suggest that exposure of the human fetal testis to estrogenic environmental chemicals, or indeed to any supranormal estrogen exposure, is unlikely to induce such effects, at least where this is mediated via ESR1.
Our findings are consistent with a recent study that used in vitro culture of human 1st trimester fetal testes, which also showed that testosterone production was not reduced by exposure to DES . The limitations of the in vitro approach, such as the short duration of exposure and decline in tissue integrity, are addressed by the current approach which permits long term treatments and maintenance of tissue integrity in addition to exposure via the circulation of the host animal .
From the 1940’s until the early 1970’s DES (~60–70 µg/kg daily from gestational weeks 8–14, increasing by 5 mg/week thereafter), was prescribed to pregnant mothers for its proposed role in reducing spontaneous miscarriage and pre-term labour , . It was subsequently shown that DES exposure in utero had a causal role in the development of vaginal malignancy . It has also been reported that DES-exposure is associated with structural abnormalities of the male reproductive tract including epididymal cysts, microphallus and testicular hypoplasia (Reviewed in ). However there is conflicting evidence regarding DES and the disorders that comprise TDS. Several studies report an increased risk of testicular cancer following prenatal exposure to exogenous estrogen , , , , . Of the two studies which specifically investigated DES effects, one found no increased risk . All the other studies reported increased risks that were not statistically significant , , , , . To date there remains no conclusive evidence of an increased risk of testicular cancer following prenatal DES exposure , , . Hypospadias has been reported to be more prevalent in DES exposed males , however these data related to urethral abnormalities rather that hypospadias per se . A recent meta-analysis reported a small increased risk of hypospadias in DES/estrogen exposed males . However, any such effect may perhaps result from direct effects on the developing penis  , rather than as the consequence of reduced testosterone production by the fetal human testis. In addition the available epidemiological evidence suggests that human exposure in utero to estrogens other than DES, such as environmental estrogens and those in the oral contraceptive pill do not result in increased risk of TDS disorders in male offspring , .
A more recent study has shown an increased risk of cryptorchidism in males exposed in utero to DES, although this was associated with initial exposure before the 11th week of gestation with no significant effect in those initially exposed after 11 weeks . Rat studies have demonstrated that testosterone production/action within a discrete masculinization programming window (MPW), is responsible for programming subsequent normal male reproductive development, and TDS disorders may only result if there is a reduction in androgen production/action in this period ; the present studies investigated effects of DES exposure on the human testis from 15 weeks of gestation, which is after the postulated MPW . It is therefore possible that this could explain the lack of effect of DES on testosterone production. However, the effects of DES on testosterone production by the fetal testis in rats occur beyond the MPW, as shown in the present study (e21.5). In addition, DES exposure of first trimester human fetal testes in vitro had no effect on testosterone production . Taken together, it seems unlikely that our present negative findings regarding DES effects are simply due to the gestational age of the fetus. An alternative mechanism for the reported increased incidence of cryptorchidism could be via effects on Insl3, a key factor in testicular descent in rodents , . In humans, Insl3 is believed to be important during early testicular descent between 8–15 weeks gestation . Further studies to investigate the effects of DES on Insl3 in first trimester human fetal testis would address this.
In rodents, exposure to DES in utero results in disorders of the reproductive tract mediated by a reduction in testosterone production. It has been postulated that similar effects occur in humans. Using a xenograft approach, we have demonstrated that exposure to DES does not result in a reduction in production of testosterone by the human fetal testis. This lack of effect on testosterone may be due to the lack of ESR1 in human fetal Leydig cells, in contrast to rodents. The findings highlight important species differences between humans and rodents, with implications for assessing the risk to human health that fetal exposure to environmental estrogens might pose.
We gratefully acknowledge the work of Anne Saunderson and the staff of the Bruntsfield Suite of the Royal Infirmary of Edinburgh in provision of tissue for these studies. We would also like to acknowledge William Mungall and Christine Marshall for assistance with the animal work.
Conceived and designed the experiments: RTM RMS CJK WHW SvdD. Performed the experiments: RTM RMS CM SM SvdD. Analyzed the data: RTM CM SvdD LBS RMS. Contributed reagents/materials/analysis tools: RTM RAA RMS. Wrote the paper: RTM RMS LBS CJK WHW SvdD.
- 1. Skakkebaek NE, Rajpert-De Meyts E, Main KM (2001) Testicular dysgenesis syndrome: an increasingly common developmental disorder with environmental aspects. Hum Reprod 16: 972–978. doi: 10.1111/j.1600-0463.2001.tb05770.x
- 2. Sharpe RM (2003) The ‘oestrogen hypothesis’ - where do we stand now? Int J Androl 26: 2–15. doi: 10.1046/j.1365-2605.2003.00367.x
- 3. Hsieh MH, Breyer BN, Eisenberg ML, Baskin LS (2008) Associations among hypospadias, cryptorchidism, anogenital distance, and endocrine disruption. Curr Urol Rep 9: 137–142. doi: 10.1007/s11934-008-0025-0
- 4. Eisenberg ML, Hsieh MH, Walters RC, Krasnow R, Lipshultz LI (2011) The relationship between anogenital distance, fatherhood, and fertility in adult men. PLoS One 6: e18973. doi: 10.1371/journal.pone.0018973
- 5. Sharpe RM, Skakkebaek NE (2008) Testicular dysgenesis syndrome: mechanistic insights and potential new downstream effects. Fertil Steril 89: e33–38. doi: 10.1016/j.fertnstert.2007.12.026
- 6. Sharpe RM, Skakkebaek NE (1993) Are oestrogens involved in falling sperm counts and disorders of the male reproductive tract? Lancet 341: 1392–1395. doi: 10.1016/0140-6736(93)90953-e
- 7. Haavisto T, Nurmela K, Pohjanvirta R, Huuskonen H, El-Gehani F, et al. (2001) Prenatal testosterone and luteinizing hormone levels in male rats exposed during pregnancy to 2,3,7,8-tetrachlorodibenzo-p-dioxin and diethylstilbestrol. Mol Cell Endocrinol 178: 169–179. doi: 10.1016/s0303-7207(01)00425-7
- 8. van den Driesche S, Walker M, McKinnell C, Scott HM, Eddie SL, et al. (2012) Proposed role for COUP-TFII in regulating fetal Leydig cell steroidogenesis, perturbation of which leads to masculinization disorders in rodents. PLoS One 7: e37064. doi: 10.1371/journal.pone.0037064
- 9. Couse JF, Dixon D, Yates M, Moore AB, Ma L, et al. (2001) Estrogen receptor-alpha knockout mice exhibit resistance to the developmental effects of neonatal diethylstilbestrol exposure on the female reproductive tract. Dev Biol 238: 224–238. doi: 10.1006/dbio.2001.0413
- 10. Marselos M, Tomatis L (1992) Diethylstilboestrol: I, Pharmacology, Toxicology and carcinogenicity in humans. Eur J Canc 28A: 1182–1189. doi: 10.1016/0959-8049(92)90482-h
- 11. Williams K, McKinnell C, Saunders PT, Walker M, Fisher JS, et al. (2001) Neonatal exposure to potent and environmental oestrogens and abnormalities of the male reproductive system in the rat: evidence for importance of the androgen-oestrogen balance and assessment of the relevance to man. Hum Reprod Update 7: 236–247. doi: 10.1111/j.1600-0463.2001.tb05805.x
- 12. Wilcox AJ, Baird DD, Weinberg CR, Hornsby PP, Herbst AL (1995) Fertility in men exposed prenatally to diethylstilbestrol. New Eng J Med 332: 1411–1416. doi: 10.1056/nejm199505253322104
- 13. Storgaard L, Bonde JP, Olsen J (2006) Male reproductive disorders in humans and prenatal indicators of estrogen exposure. A review of published epidemiological studies. Reprod Toxicol 21: 4–15. doi: 10.1016/j.reprotox.2005.05.006
- 14. Martin OV, Shialis T, Lester JN, Scrimshaw MD, Boobis AR, et al. (2008) Testicular dysgenesis syndrome and the estrogen hypothesis: a quantitative meta-analysis. Environ Health Perspect 116: 149–157. doi: 10.1289/ehp.10545
- 15. Palmer JR, Herbst AL, Noller KL, Boggs DA, Troisi R, et al. (2009) Urogenital abnormalities in men exposed to diethylstilbestrol in utero: a cohort study. Environmental health : a global access science source 8: 37. doi: 10.1186/1476-069x-8-37
- 16. Gaskell TL, Robinson LL, Groome NP, Anderson RA, Saunders PT (2003) Differential expression of two estrogen receptor beta isoforms in the human fetal testis during the second trimester of pregnancy. J Clin Endocrinol Metab 88: 424–432. doi: 10.1210/jc.2002-020811
- 17. Boukari K, Ciampi ML, Guiochon-Mantel A, Young J, Lombes M, et al. (2007) Human fetal testis: source of estrogen and target of estrogen action. Hum Reprod 22: 1885–1892. doi: 10.1093/humrep/dem091
- 18. Mitchell RT, Childs AJ, Anderson RA, van den Driesche S, Saunders PT, et al. (2012) Do phthalates affect steroidogenesis by the human fetal testis? Exposure of human fetal testis xenografts to di-n-butyl phthalate. J Clin Endocrinol Metab. 97(3): E341–8. doi: 10.1210/jc.2011-2411
- 19. Mitchell RT, Saunders PT, Childs AJ, Cassidy-Kojima C, Anderson RA, et al. (2010) Xenografting of human fetal testis tissue: a new approach to study fetal testis development and germ cell differentiation. Hum Reprod 25: 2405–2414. doi: 10.1093/humrep/deq183
- 20. Polkinghorne J (1989): Review of the Guidance on the Research Use of Fetuses and Fetal Material. London: Her Majesty’s Stationary Office.
- 21. Corker CS, Davidson DW (1978) A radioimmunoassay for testosterone in various biological fluids without chromatography. J Steroid Biochem 9: 373–374. doi: 10.1016/0022-4731(78)90634-9
- 22. Mitchell RT, Cowan G, Morris KD, Anderson RA, Fraser HM, et al. (2008) Germ cell differentiation in the marmoset (Callithrix jacchus) during fetal and neonatal life closely parallels that in the human. Hum Reprod 23: 2755–2765. doi: 10.1093/humrep/den295
- 23. Walker VR, Jefferson WN, Couse JF, Korach KS (2012) Estrogen receptor-alpha mediates diethylstilbestrol-induced feminization of the seminal vesicle in male mice. Environ Health Perspect 120: 560–565. doi: 10.1289/ehp.1103678
- 24. Delbes G, Levacher C, Duquenne C, Racine C, Pakarinen P, et al. (2005) Endogenous estrogens inhibit mouse fetal Leydig cell development via estrogen receptor alpha. Endocrinology 146: 2454–2461. doi: 10.1210/en.2004-1540
- 25. Cederroth CR, Schaad O, Descombes P, Chambon P, Vassalli JD, et al. (2007) Estrogen receptor alpha is a major contributor to estrogen-mediated fetal testis dysgenesis and cryptorchidism. Endocrinology 148: 5507–5519. doi: 10.1210/en.2007-0689
- 26. Inaoka Y, Yazawa T, Uesaka M, Mizutani T, Yamada K, et al. (2008) Regulation of NGFI-B/Nur77 gene expression in the rat ovary and in leydig tumor cells MA-10. Mol Reprod Dev 75: 931–939. doi: 10.1002/mrd.20788
- 27. Volle DH, Decourteix M, Garo E, McNeilly J, Fenichel P, et al. (2009) The orphan nuclear receptor small heterodimer partner mediates male infertility induced by diethylstilbestrol in mice. J Clin Invest 119: 3752–3764. doi: 10.1172/jci38521
- 28. N’Tumba-Byn T, Moison D, Lacroix M, Lecureuil C, Lesage L, et al. (2012) Differential effects of bisphenol a and diethylstilbestrol on human, rat and mouse fetal leydig cell function. PLoS One 7: e51579. doi: 10.1371/journal.pone.0051579
- 29. Toppari J, Larsen JC, Christiansen P, Giwercman A, Grandjean P, et al. (1996) Male reproductive health and environmental xenoestrogens. Environ Health Perspect 104 Suppl 4741–803. doi: 10.1289/ehp.96104s4741
- 30. Herbst AL, Ulfelder H, Poskanzer DC (1971) Adenocarcinoma of the vagina. Association of maternal stilbestrol therapy with tumor appearance in young women. New Engl J Med 284: 878–881. doi: 10.1056/nejm197104222841604
- 31. Strohsnitter WC, Noller KL, Hoover RN, Robboy SJ, Palmer JR, et al. (2001) Cancer risk in men exposed in utero to diethylstilbestrol. J Natl Cancer Inst 93: 545–551. doi: 10.1093/jnci/93.7.545
- 32. Weir HK, Marrett LD, Kreiger N, Darlington GA, Sugar L (2000) Pre-natal and peri-natal exposures and risk of testicular germ-cell cancer. Int J Cancer 87: 438–443. doi: 10.1002/1097-0215(20000801)87:3<438::aid-ijc20>3.0.co;2-1
- 33. Moss AR, Osmond D, Bacchetti P, Torti FM, Gurgin V (1986) Hormonal risk factors in testicular cancer. A case-control study. Am J Epidemiol 124: 39–52.
- 34. Depue RH, Pike MC, Henderson BE (1986) Cryptorchidism and testicular cancer. J Natl Cancer Inst 77: 830–833.
- 35. Schottenfeld D, Warshauer ME, Sherlock S, Zauber AG, Leder M, et al. (1980) The epidemiology of testicular cancer in young adults. Am J Epidemiol 112: 232–246.
- 36. Gershman ST, Stolley PD (1988) A case-control study of testicular cancer using Connecticut tumour registry data. Int J Epidemiol 17: 738–742. doi: 10.1093/ije/17.4.738
- 37. Henderson BE, Benton B, Cosgrove M, Baptista J, Aldrich J, et al. (1976) Urogenital tract abnormalities in sons of women treated with diethylstilbestrol. Pediatrics 58: 505–507. doi: 10.1097/00006254-197703000-00024
- 38. Joffe M (2002) Myths about endocrine disruption and the male reproductive system should not be propagated. Hum Reprod 17: 520–523. doi: 10.1093/humrep/17.2.520
- 39. Liu B, Lin G, Willingham E, Ning H, Lin CS, et al. (2007) Estradiol upregulates activating transcription factor 3, a candidate gene in the etiology of hypospadias. Pediatr Dev Pathol 10: 446–454. doi: 10.2350/06-04-0079
- 40. Qiao L, Rodriguez E Jr, Weiss DA, Ferretti M, Risbridger G, et al. (2012) Expression of estrogen receptor alpha and beta is decreased in hypospadias. J Urol 187: 1427–1433. doi: 10.1016/j.juro.2011.12.008
- 41. Norgaard M, Wogelius P, Pedersen L, Rothman KJ, Sorensen HT (2009) Maternal use of oral contraceptives during early pregnancy and risk of hypospadias in male offspring. Urology 74: 583–587. doi: 10.1016/j.urology.2009.04.034
- 42. Welsh M, Saunders PT, Fisken M, Scott HM, Hutchison GR, et al. (2008) Identification in rats of a programming window for reproductive tract masculinization, disruption of which leads to hypospadias and cryptorchidism. J Clin Invest 118: 1479–1490. doi: 10.1172/jci34241
- 43. Emmen JM, McLuskey A, Adham IM, Engel W, Verhoef-Post M, et al. (2000) Involvement of insulin-like factor 3 (Insl3) in diethylstilbestrol-induced cryptorchidism. Endocrinology 141: 846–849. doi: 10.1210/endo.141.2.7379
- 44. Zimmermann S, Steding G, Emmen JM, Brinkmann AO, Nayernia K, et al. (1999) Targeted disruption of the Insl3 gene causes bilateral cryptorchidism. Mol Endocrinol 13: 681–691. doi: 10.1210/mend.13.5.0272
- 45. Hughes IA, Acerini CL (2008) Factors controlling testis descent. Eur J Endocrinol 159 Suppl 1S75–82. doi: 10.1530/eje-08-0458