Search tips
Search criteria 


Logo of jzusbLink to Publisher's site
J Zhejiang Univ Sci B. 2010 September; 11(9): 719–727.
PMCID: PMC2932882

Effect of interrupted endogenous BMP/Smad signaling on growth and steroidogenesis of porcine granulosa cells*


Bone morphogenetic proteins (BMPs) play a critical role in the growth and steroidogenesis of granulosa cells (GCs). BMP signals act through membrane-bound heteromeric serine/threonine kinase receptors. Upon ligand binding, BMPs activate intracellular Smad proteins and regulate growth and apoptosis in various cell types. The objective of this study was to demonstrate the effects of BMP/Smad signal on growth and steroidogenesis of porcine GCs. A strategy of RNA interference (RNAi)-mediated ‘gene silencing’ of Smad4, a core molecule mediating the intracellular BMP/Smad signal transduction pathways, was used to interrupt endogenous BMP/Smad signaling. Results indicate that Smad4-small interfering RNA (siRNA) caused specific inhibition of Smad4 mRNA and protein expression after transfection. Interrupted endogenous BMP/Smad signaling significantly inhibited growth, and induced apoptosis of porcine GCs, while decreasing estradiol production. In addition, interrupted BMP/Smad signaling significantly (P<0.05) changed the expression of Cyclin D2, CDK4, Bcl-2, and Cyp19a1. These findings provide new insights into how BMP/Smad signaling regulates the growth and steroidogenesis of porcine GCs.

Keywords: Porcine granulosa cells, Bone morphogenetic protein (BMP)/Smad, Smad4, RNA interference (RNAi), Growth, Steroidogenesis

1. Introduction

Female fertility in mammals is dependent on the growth and development of follicles. Folliculogenesis involves a series of sequential steps in which a growing follicle either develops to the ovulation stage or undergoes atresia. Significant disruption occurring at any of the stages of folliculogenesis impairs fertility (McGee and Hsueh, 2000).

Bone morphogenetic proteins (BMPs) belong to the transforming growth factor β (TGF-β) superfamily, and are key factors for normal folliculogenesis. Recent studies have established that BMPs play a crucial role in female fertility in mammals by regulating steroidogenesis as well as mitogenesis in granulosa cells (GCs) (Shimasaki et al., 2003; 2004). BMP-6 inhibits follicle-stimulating hormone (FSH)-induced progesterone synthesis through the suppression of cellular cyclic adenosine monophosphate (cAMP) synthesis (Otsuka et al., 2001a). BMP-15 also exhibits potent suppression of FSH actions by inhibiting FSH receptor (FSHR) expression (Otsuka et al., 2001b). In addition, growth differentiation factor-9 (GDF-9), which is highly homologous with BMP-15, also inhibits FSH-induced steroidogenesis and luteinizing hormone (LH) receptor expression in rat GCs (Vitt et al., 2000; Miyoshi et al., 2006).

TGF-β activates a cell surface receptor complex, which consists of two different transmembrane serine/threonine kinases that phosphorylate members of the downstream receptor-regulated Smads (R-Smads) upon ligand binding (Schmierer and Hill, 2007). The closely related R-Smads, Smad1, Smad5, and Smad8, transmit BMP and GDF signals, while Smad2 and Smad3 are phosphorylated in response to TGF-β, activin and nodal signals. The phosphorylated R-Smads in combination with the common mediators, Smad and Smad4, recruit appendant cofactors to form complexes that in turn regulate target gene expression (Massagué et al., 2005). Smad4, originally discovered to be a tumor suppressor gene, shares structural features with the R-Smads. However, its MH2 domain lacks the C-terminal SXS motif required for receptor-mediated phosphorylation. Smad complexes regulate various kinds of biological processes, including cell proliferation, differentiation, and apoptosis during embryonic development and adult tissue homeostasis (Costello et al., 2009).

In mammals, Smad4 is the only co-mediating Smad, translocating to the nucleus with phosphorylated R-Smads, and then modulating transcription of BMP target genes. Smad4 is extensively expressed in embryonic and adult diverse tissues. Smad4 nucleocytoplasmic shuttling is not required for R-Smad phosphorylation or nuclear localization (Biondi et al., 2007). R-Smad dephosphorylation and nuclear export are thought to be essential for optimal TGF-β signaling (Lin et al., 2006; Dai et al., 2009). Loss of Smad4 leads to increased steady state levels of both BMP and TGF-β phosphorylated R-Smads. Enhanced R-Smad phosphorylation levels potentially reflect reduced dephosphorylation and/or nuclear export (Lin et al., 2006; Dai et al., 2009; Costello et al., 2009). Therefore, Smad4 is crucial for BMP/Smad signaling.

The aim of this study was to determine how BMP/Smad signaling regulates the growth and steroidogenesis of porcine GCs using highly potent small interfering RNA (siRNA) interference to suppress Smad4 gene expression.

2. Materials and methods

2.1. Isolation and culture of GCs

Porcine ovaries were obtained from a local slaughterhouse, and transported to the laboratory at 37 °C in saline containing gentamicin and amphotericin. The ovaries were washed three times with pre-warmed phosphate-buffered saline (PBS) supplemented with gentamicin and amphotericin. GCs were collected from follicles (3–5 mm) by needle (20 G) aspiration, and filtered through a stainless steel filter (100 μm) to remove the cumulus-oocytes complexes (COC). The cells were centrifuged at 800×g per min and washed twice in DMEM/F12 medium (Dulbecco’s modified Eagle medium/Ham’s nutrient mixture F-12; Shanghai Invitrogen Biotechnology Co., Ltd., China). GCs were cultured as described previously (Picton et al., 1999). GCs were counted in a hemocytometer, and the viability was determined by trypan blue dye exclusion, and then the GCs were seeded in six-well culture plates (Costar; Corning Inc., NY, USA) at a density of (3–5)×106 cells per well in 2 ml of DMEM/F12 medium containing 10% (v/v) fetal calf serum (FCS; Minhai Co., Lanzhou, China), 5 μl/ml of gentamicin, and 10 μl/ml amphotericin. The cells were cultured for 24 h at 37 °C in a 5% (v/v) CO2 atmosphere and then the wells were washed with PBS to remove unattached cells. Exponentially growing cells were used for the experiments.

2.2. Design and transfection of siRNA

The complementary DNA (cDNA) sequence of porcine Smad4 (GenBank accession No. NM_214072) was examined using Invitrogen’s web-based siRNA design software ( to select appropriate siRNA target sites. A pair of oligonucleotides corresponding to Smad4 cDNA were designed. A BLAST (basic local alignment search tool) search of these sequences confirmed their specificity to Smad4 only. In addition, a nonsense sequence with no similar match to any known sequence was used as control. The Smad4 small RNA interference (RNAi) was named Smad4-siRNA, and the nonsense sequence to Smad4 was named negative control siRNA (NC-siRNA).

GC cultures were transfected with Smad4-siRNA or NC-siRNA using Lipofectamine™ RNAiMAX Reagent (Shanghai Invitrogen Biotechnology Co., Ltd.). Briefly, RNAi duplex, Lipofectamine™ RNAiMAX, and 250 μl DMEM/F12 medium were combined and incubated for 20 min at room temperature. The transfection complex was added to the cells, and incubated for 48 h at 37 °C.

2.3. Measurement of Smad4 expression by real-time RT-PCR

Total RNA was extracted from GCs using TRIzol following the manufacturer’s instructions. RNA concentration and purity were determined by measuring optical density (OD) at wavelengths of 260 and 280 nm using a standard spectrophotometer. The OD260/OD280 ratios were more than 1.8 for all samples. Aliquots (100 ng) of total RNA from each pool of cultured GCs were independently reverse-transcribed to cDNA using Moloney murine leukemia virus (M-MLV) reverse transcriptase (Promega Corporation, USA) and oligonucleotide primers.

Target genes and the housekeeping gene glyceraldehyde-3-phosphate dehydrogenase (GAPDH) were quantified by real-time quantitative reverse transcription-polymerase chain reaction (RT-PCR) with an ABI 7300 using a commercial kit (SYBR® Premix Ex Taq™, TaKaRa, Dalian, China). The gene-specific primers were designed on the basis of porcine mRNA sequences (Table (Table1).1). The cDNA generated was used as a template for PCR using a 25-μl reaction mixture for 40–45 cycles. Relative concentrations of mRNA were calculated using the 2−ΔΔCT method (Livak and Schmittgen, 2001). A water control was included to identify possible contamination in all reactions. After amplification, each sample was applied to a 2% (w/v) agarose/ethidium bromide gel for electrophoresis.

Table 1

Details of primers for target gene amplification

2.4. Measurement of Smad4 expression by immunofluorescence

GCs were grown in glass chamber slides. After treatments were applied, cells were washed with PBS three times, fixed with 4% (w/v) paraformaldehyde, washed in PBS, permeabilized with 0.3% (v/v) Triton X-100 in PBS, and blocked in 0.5% (w/v) bovine serum albumin (BSA) and 0.3% (v/v) Triton X-100 in PBS for 30 min at room temperature. Slides were then incubated with primary antibodies as follows: rabbit monoclonal antibody against Smad4 (1:200 dilution in PBS; Abcam; ab40759) for 2 h at room temperature. Slides were washed three times with cold PBS and incubated with biotinylated anti-rabbit immunoglobulin G (IgG; 1:200 dilution in PBS; Abcam; ab6939) for 1 h at room temperature, and then mounted with Vectashield mountant containing the nuclear counter-stain 4′,6-diamidino-2-phenylindole (DAPI; Sigma, USA). Fluorescent images were captured with a Leica DMLB2 fluorescent microscope. Morphometric analysis was carried out using the ImageJ program.

2.5. Measurement of Smad4 expression by Western blotting

Total proteins from GCs were extracted in a cell lysis buffer for Western and immunol precipitation (Beyotime, China) containing 10 mmol/L phenylmethyl sulfonylfluoride (PMSF; Beyotime, China), and the resultant cell suspension was centrifuged at 12 000 r/min for 5 min. The supernatant was removed and the amount of protein was quantified using the bicinchoninic acid (BCA) protein assay kit (Beyotime, China). The homogenized samples (15 μg crude proteins per lane) were subjected to electrophoresis on 12% (w/v) poly-acrylamide-sodium dodecyl sulfate (SDS) gels under standard reducing conditions with precision protein molecular weight marked (MBI Fermentas, China), and then transferred to polyvinylidene difluoride membranes (Millipore, Bedford, MA, USA) at 2.5 mA/cm2 for 45 min. Then they were blocked with 5% (w/v) BSA in PBS (blocking buffer) for 1 h at room temperature. Immunoblotting was carried out by incubating the membranes overnight at 4 °C with antibodies against Smad4 (Abcam; 1:2000 dilution) or GAPDH (Sigma, 1:2000 dilution). The membranes were washed three times with 1% (v/v) Tween-20 in PBS, then hybridized with horse radish peroxidase (HRP)-conjugated secondary goat anti-rabbit IgG antibody (Santa Cruz Biotechnology Inc., California, USA) diluted at 1:5000 for 2 h. After three washes with 1% (v/v) Tween-20 in PBS, the signals were detected as chemical luminescene by X-ray film with BeyoECL Plus kit (Beyotime, China).

2.6. Measurement of cell growth by MTT assay

GCs were counted in a hemocytometer, and the viability was determined by trypan blue dye exclusion, and then the GCs were seeded in 96-well culture plates (Costar; Corning Inc., NY, USA) at a density of (3–5)×104 cells per well. GCs were treated with or without siRNA. The number of live cells at the end of the process of culture was determined with the MTT (3-(4,5-dimethylthiazol-2-yl)-2,5-diphenyltetrazolium bromide) kit (KeyGEN Biotechnology Co., Ltd., Nanjing, China), as recommended by the manufacturer. The optical density at 550 nm (OD550) was determined using an enzyme-linked immunosorbent assay (ELISA) reader (Bio-TEK Instruments, USA).

2.7. Measurement of cell cycle and apoptosis by flow cytometry

After culture, GCs were digested and prepared by washing twice with PBS, and then fixed in 70% (v/v) ethanol and stained with 100 μg/ml propidium iodide (PI) at 4 °C for 1 h. DNA content was monitored by FACScan (COULTESR, Elite, USA).

Also after culture, GCs were digested and prepared by washing twice with PBS, and then 5 μl annexin V-rhodamine isothiocyanate (RITC) and PI were added to the cells, combined, and incubated for 15 min at room temperature. The rate of apoptosis was monitored by FACScan (COULTESR, Elite, USA).

2.8. Measurement of estradiol and progesterone

GCs (2×105 viable cells) were cultured in 24-well plates. After treatment, the culture medium was collected and stored at −80 °C until assay. The levels of estradiol (E2) and progesterone (P4) in the medium were measured by chemiluminescent immunoassay (CLIA; ACCESS, Beckman Coulter Co., USA). Steroid contents were negligible (P4 <0.1 ng/ml and E2 <10 pg/ml). The intra- and inter-assay coefficients of variation were 15% and 20% for E2, and 5% and 10% for P4, respectively.

2.9. Statistical analysis

All results are shown as mean±standard error of the mean (SEM) from at least three separate experiments, each performed with triplicate samples. Data were analyzed by one-way analysis of variance (ANOVA), followed by the Fisher’s least significant difference (LSD) test for multiple comparisons using SPSS 16.0 software. Differences were considered to be statistically significant at the 95% confidence level (P<0.05).

3. Results

3.1. Effect of siRNA on Smad4 expression

We knocked down Smad4 in porcine GCs by siRNA. The expression of Smad4 mRNA and protein was analyzed by real-time PCR, immunofluorescence, and Western blotting at post-transfection, as described in Fig. Fig.1.1. The results in Fig. Fig.1a1a show that the expression of Smad4 mRNA was inhibited after transfection with Smad4-siRNA, the Smad4 transcript level being reduced by approximately 89% compared with that in the control cultures (blank and NC-siRNA). Western blotting and immunofluorescence staining analyses of Smad4 expression clearly revealed the suppressive effect of Smad4-siRNA on the expression of the Smad4 protein in the GCs (Figs. 1c and 1d). The results of the analyses demonstrate that the level of Smad4 protein also markedly decreased 48 h post-transfection with the Smad4-siRNA, by approximately 56.6% (Fig. (Fig.1b1b).

Fig. 1Fig. 1Fig. 1Fig. 1

Analyses of the expression of Smad4 mRNA and protein by real-time PCR, Western blotting, and immunofluorescence at post-transfection

3.2. Effect of interrupted BMP/Smad signaling on growth of GCs

MTT analysis was performed to test the effect of interrupted BMP/Smad signaling on the growth of GCs. As expected, interrupted BMP/Smad signaling significantly inhibited the growth of cells, as compared with the control cultures (blank and NC-siRNA) cells (Table (Table22).

Table 2

Effect of interrupted BMP/Smad signaling on cell growth of GCs

3.3. Effect of interrupted BMP/Smad signaling on cell cycle of GCs

To further determine the effect of interrupted BMP/Smad signaling on the growth of GCs, flow cytometry was used to analyze the cell cycle changes of GCs. The results in Table Table33 show that interrupted BMP/Smad signaling can significantly increase the proportion of cells in G1-phase, and decrease the cells in S-phase, and there are no significantly differences in the proportion of cells in G2-phase.

Table 3

Effect of interrupted BMP/Smad signaling on cell cycle of GCs

3.4. Effect of interrupted BMP/Smad signaling on cell cycle marker genes

To investigate the mechanism by which interrupted BMP/Smad signaling regulates the cell cycle of GCs, we measured the expression of Cyclin D2 and CDK4, functional markers of cell proliferation (Fig. (Fig.2).2). In Smad4 knockdown cells, Cyclin D2 and CDK4 mRNA levels were lower than those in the controls.

Fig. 2

Effect of interrupted BMP/Smad signaling on cell cycle marker gene mRNA levels

3.5. Effect of interrupted BMP/Smad signaling on apoptosis of GCs

Flow cytometry analysis was performed to test the effect of interrupted BMP/Smad signaling on the apoptosis of GCs. Table Table44 shows that interrupted BMP/Smad signaling increased the rate of apoptotic cells, as compared with the control cultures (blank and NC-siRNA).

Table 4

Effect of interrupted BMP/Smad signaling on apoptosis of GCs

3.6. Effect of interrupted BMP/Smad signaling on cell apoptosis related genes

To investigate the mechanism by which interrupted BMP/Smad signaling encourages the apoptosis of GCs, we measured the mRNA expression of Bcl-2 and Bax, related markers of apoptosis cell (Fig. (Fig.3).3). In Smad4 knockdown cells, Bcl-2 mRNA levels were significantly lower than those in controls. In contrast, the Bax mRNA levels were not affected by interrupted BMP/Smad signaling.

Fig. 3

Effect of interrupted BMP/Smad signaling on apoptosis related gene mRNA levels

3.7. Effect of interrupted BMP/Smad signaling on estradiol and progesterone production

We examined interrupted BMP/Smad signaling effects on steroidogenesis. As shown in Table Table5,5, interrupted BMP/Smad signaling decreased E2 production, and had no significant effect on P4 production.

Table 5

Effect of interrupted BMP/Smad signaling on estradiol (E2) and progesterone (P4) production

3.8. Effect of interrupted BMP/Smad signaling on steroidogenic enzyme genes

To confirm whether the effects of interrupted BMP/Smad signaling were involved in the expression changes of steroidogenic enzyme genes, levels of mRNA encoding Cyp19a1 and Cyp11a1, key enzymes regulating E2 and P4 production in GCs (Lee et al., 2001), were examined by quantitative real-time PCR. Interrupted BMP/Smad signaling decreased Cyp19a1 mRNA expression (Fig. (Fig.44).

Fig. 4

Effect of interrupted BMP/Smad signaling on steroidogenic enzyme gene mRNA levels

4. Discussion

The BMP family controls a variety of intraovarian reproductive processes (Shimasaki et al., 2004). To further understand the effect of endogenous BMP/Smad signaling on porcine GCs, in the present study, RNAi was employed to silence the Smad4 gene, the key mediator of BMP/Smad signaling. It was observed that the knockdown of endogenous Smad4 gene blocked BMP/Smad signaling, inhibited the growth of GCs, induced cell apoptosis, and decreased E2 production, suggesting that the endogenous BMP/Smad signaling is important to porcine GCs.

Pangas et al. (2006)’s study on the Smad4 conditional knockout (cKO) ovary suggested that one of the primary defects of Smad4 loss is premature luteinization of GCs. We silenced endogenous Smad4, as an alternative to block BMP/Smad signaling, in porcine GCs to characterize a potential role of BMP/Smad signaling. We selected RNAi technique in part because the sequence-specific knockdown of target mRNA is more efficient than that of antisense oligonucleotides or ribozymes (Dorsett and Tuschl, 2004; Mittal, 2004). Our results show that Smad4-siRNA can significantly inhibit the mRNA and protein expression of Smad4, as demonstrated by real-time RT-PCR, Western blotting, and immunofluorescence staining. We established a strategy for identifying efficient siRNA sequence for gene knockdown by transfecting porcine GCs.

It has been well documented that cell proliferation depends on the cell cycle. Therefore, we investigated the effects of blocked BMP/Smad signaling on cell cycle of porcine GCs. Blocked BMP/Smad signaling significantly increased and decreased the cells of G1 and S phase stages, respectively. We also investigated the mechanism by which blocked BMP/Smad signaling suppresses cell growth in GCs. The G1 checkpoint can be viewed as a master checkpoint of the mammalian cell cycle (Paterson et al., 2002; Matsuura et al., 2004). Regulation of the G1 phase of the cell cycle involves many different families of cyclins, Cyclin D and cyclin-dependent kinases (CDKs). Inhibition of growth of GCs by blocked BMP/Smad signaling was associated with a decrease in Cyclin D2 and CDK4 expression. Cyclin D2 and CDK4 act as a downstream gene of Smad4, participating in the regulation of BMPs in porcine GCs, and they may be involved in BMPs-induced cell growth in a Smad4-dependent manner. Thus, we postulate that at least part of blocked BMP/Smad signaling effect on GCs growth is mediated by the decrease in Cyclin D2 and CDK4 expression. RNAi-mediated Smad4 silencing resulted in decreased proliferation of the cells and G1 cell cycle arrest, indicating that BMP/Smad signaling plays a key role in the normal growth of porcine GCs.

Follicular development in mammals is dependent on many factors, such as gonadotropin hormones, FSH and LH, and the steroid hormones, E2, and P4, as well as ovarian local factors including TGF-β superfamily. Yamashita et al. (2007) and Kawashima et al. (2008) believed that the pituitary gonadotropin FSH is essential for GCs’ E2 production and increases estrogen concentrations in follicular fluid during the development of mammalian ovarian follicles. Changes in the expression of mRNA encoding steroidogenic genes exhibit patterns of expression that coordinated with steroid production. In vivo, the growth and differentiation of GCs are tightly regulated by gonadotropins and ovarian local factors such as estrogen, GDF-9/BMP-15, and insulin-like growth factor 1 (IGF-1). However, in vitro, people cannot mimic these conditions. We investigated the effects of interrupted endogenous BMP/Smad signaling on steroidogenesis of porcine GCs. After transfection, the E2 level of Smad4-siRNA group significantly decreased, while transfection had no significant effect on P4. A possible reason is that we measured the basal levels of E2 and P4 in cultured GCs; thus, unknown factors in the serum may have affected GC steroidogenesis. These require further elucidation.

A widely accepted opinion is that the Ras-MAPK (mitogen-activated protein kinase) pathway (activated after LH surge) plays a major role in regulating GC steroidogenesis (Fan et al., 2008; 2009). The TGF-β superfamily members are critical in maintaining cell growth and differentiation in the ovary (Pangas et al., 2008). BMPs play a key role in regulating GC steroidogenesis. In particular, they change the expression of steroidogenic enzymes such as Cyp19a1 (aromatase) and Cyp11a1 (p450scc) (Winters et al., 1998), and these actions are important, and are modulated by various growth factors, acting in a paracrine or autocrine way (Khamsi and Roberge, 2001). In vitro, BMP-4 and BMP-7 enhanced FSH-dependent E2 production (Shimasaki et al., 1999), whereas BMP-4, BMP-6, BMP-7, BMP-15, and GDF-9 inhibited FSH-induced P4 secretion by rat GCs in culture (Shimasaki et al., 1999; Otsuka et al., 2000; Vitt et al., 2000; Fraser et al., 2001; Lee et al., 2001), suggesting that BMP factors regulate GC differentiation, particularly in delaying luteinization. In the present study, blocked BMP/Smad signaling inhibited E2 secretion, but did not affect P4 secretion. In order to evaluate the regulation of E2 and P4 production, we examined the steady-state level of mRNA for Cyp19a1 and Cyp11a1 genes, two of the key regulators in the steroidogenesis implicated in the E2 and P4 synthesis pathways. Our results show that blocked BMP/Smad signaling significantly inhibited Cyp19a1 expression.

In conclusion, the interruption of endogenous BMP/Smad signaling by RNAi-mediated Smad4 gene silencing not only inhibits the growth but also induces the apoptosis of porcine GCs. In addition, interrupted BMP/Smad signaling changes steroidogenesis. Our findings provide a new insight that interrupted BMP/Smad signaling plays an important and specific role in mediating porcine GC growth and steroidogenesis.


We thank Prof. Christopher A. PRICE for his kind help in reviewing the manuscript.


*Project (No. 2006AA10Z136) supported by National High-Tech R & D Program (863) of China


1. Biondi CA, Das D, Howell M, Islam A, Bikoff EK, Hill CS, Robertson EJ. Mice develop normally in the absence of Smad4 nucleocytoplasmic shuttling. Biochem J. 2007;404(2):235–245. doi: 10.1042/BJ20061830. [PubMed] [Cross Ref]
2. Costello I, Biondi CA, Taylor JM, Bikoff EJ, Robertson EJ. Smad4-dependent pathways control basement membrane deposition and endodermal cell migration at early stages of mouse development. BMC Devel Biol. 2009;9(1):54. doi: 10.1186/1471-213X-9-54. [PMC free article] [PubMed] [Cross Ref]
3. Dai F, Lin X, Chang C, Feng XH. Nuclear export of Smad2 and Smad3 by RanBP3 facilitates termination of TGF-β signaling. Dev Cell. 2009;16(3):345–357. doi: 10.1016/j.devcel.2009.01.022. [PMC free article] [PubMed] [Cross Ref]
4. Dorsett Y, Tuschl T. siRNAs: applications in functional genomics and potential as therapeutics. Nat Rev Drug Discov. 2004;3(4):318–329. doi: 10.1038/nrd1345. [PubMed] [Cross Ref]
5. Fan HY, Shimada M, Liu ZL, Cahill N, Noma N, Wu Y, Gossen J, Richards JS. Selective expression of KrasG12D in granulosa cells of the mouse ovary causes defects in follicle development and ovulation. Development. 2008;135(12):2127–2137. doi: 10.1242/dev.020560. [PubMed] [Cross Ref]
6. Fan HY, Liu ZL, Shimada M, Sterneck E, Johnson PF, Hedric SM, Richards JS. MAPK3/1 (ERK1/2) in ovarian granulosa cells are essential for female fertility. Science. 2009;324(5929):938–941. doi: 10.1126/science.1171396. [PMC free article] [PubMed] [Cross Ref]
7. Fraser M, Braems GA, Challis JR. Developmental regulation of corticotrophin receptor gene expression in the adrenal gland of the ovine fetus and newborn lamb: effects of hypoxia during late pregnancy. J Endocrinol. 2001;169(1):1–10. doi: 10.1677/joe.0.1690001. [PubMed] [Cross Ref]
8. Kawashima I, Okazaki T, Noma N, Nishibori M, Yamashita Y, Shimada M. Sequential exposure of porcine cumulus cells to FSH and/or LH is critical for appropriate expression of steroidogenic and ovulation-related genes that impact oocyte maturation in vivo and vitro. Reproduction. 2008;136(1):9–21. doi: 10.1530/REP-08-0074. [PubMed] [Cross Ref]
9. Khamsi F, Roberge S. Granulosa cells of the cumulus oophorus are different from mural granulosa cells in their response to gonadotrophins and IGF-1. J Endocrinol. 2001;170(3):565–573. doi: 10.1677/joe.0.1700565. [PubMed] [Cross Ref]
10. Lee WS, Otsuka F, Moore RK, Shimasaki S. Effect of bone morphogenetic protein-7 on folliculo-genesis and ovulation in the rat. Biol Reprod. 2001;65(4):994–999. doi: 10.1095/biolreprod65.4.994. [PubMed] [Cross Ref]
11. Lin X, Duan XY, Liang YY, Su Y, Wrighton KH, Long JY, Hu M, Davis CM, Wang JR, Brunicardi FC, et al. PPM1A functions as a Smad phosphatase to terminate TGFβ signaling. Cell. 2006;125(5):915–928. doi: 10.1016/j.cell.2006.03.044. [PubMed] [Cross Ref]
12. Livak KJ, Schmittgen TD. Analysis of relative gene expression data using real-time quantitative PCR and the 2−ΔΔCT method. Methods. 2001;25(4):402–408. doi: 10.1006/meth.2001.1262. [PubMed] [Cross Ref]
13. Massagué J, Seoane J, Wotton D. Smad transcription factors. Genes Dev. 2005;19(23):2783–2810. doi: 10.1101/gad.1350705. [PubMed] [Cross Ref]
14. Matsuura I, Denissova NG, Wang G, He DM, Long JY, Liu F. Cyclin-dependent kinases regulate the antiproliferative function of Smads. Nature. 2004;430(6996):226–231. doi: 10.1038/nature02650. [PubMed] [Cross Ref]
15. McGee EA, Hsueh AJW. Initial and cyclic recruitment of ovarian follicles. Endocr Rev. 2000;21(2):200–214. doi: 10.1210/er.21.2.200. [PubMed] [Cross Ref]
16. Mittal V. Improving the efficiency of RNA interference in mammals. Nat Rev Genet. 2004;5(5):355–365. doi: 10.1038/nrg1323. [PubMed] [Cross Ref]
17. Miyoshi T, Otsuka F, Suzuki J, Takeda M, Inagaki K, Kano Y, Otani H, Mimura Y, Ogura T, Makino H. Mutual regulation of follicle-stimulating hormone signaling and bone morphogenetic protein system in human granulosa cells. Biol Reprod. 2006;74(6):1073–1082. doi: 10.1095/biolreprod.105.047969. [PubMed] [Cross Ref]
18. Otsuka F, Yao ZX, Lee TH, Yamamot S, Erickson GF, Shimasaki S. Bone morphogenetic protein-15. Identification of target cells and biological functions. J Biol Chem. 2000;275(50):39523–39528. doi: 10.1074/jbc.M007428200. [PubMed] [Cross Ref]
19. Otsuka F, Moore RK, Shimasaki S. Biological function and cellular mechanism of bone morphogenetic protein-6 in the ovary. J Biol Chem. 2001;276(35):32889–32895. doi: 10.1074/jbc.M103212200. [PubMed] [Cross Ref]
20. Otsuka F, Yamamoto S, Erickson GF, Shimasaki S. Bone morphogenetic protein-15 inhibits follicle-stimulating hormone (FSH) action by suppressing FSH receptor expression. J Biol Chem. 2001;276(14):11387–11392. doi: 10.1074/jbc.M010043200. [PubMed] [Cross Ref]
21. Pangas SA, Li XH, Robertson EJ, Matzuk MM. Premature luteinization and cumulus cell defects in ovarian-specific Smad4 knockout mice. Mol Endocrinol. 2006;20(6):1406–1422. doi: 10.1210/me.2005-0462. [PubMed] [Cross Ref]
22. Pangas SA, Li XH, Umans L, Zwijsen A, Huylebroeck D, Gutierrez C, Wang DG, Martin JF, Jamin SP, Behringer RR, et al. Conditional deletion of Smad1 and Smad5 in somatic cells of male and female gonads leads to metastatic tumor development in mice. Mol Cell Biol. 2008;28(1):248–257. doi: 10.1128/MCB.01404-07. [PMC free article] [PubMed] [Cross Ref]
23. Paterson IC, Davies M, Stone A, Huntley S, Smith E, Pring M, Eveson JW, Robinson CM, Parkinson EK, Prime SS. TGF-β1 acts as a tumor suppressor of human malignant keratinocytes independently of Smad4 expression and ligand-induced G(1) arrest. Oncogene. 2002;21(10):1616–1624. doi: 10.1038/sj.onc.1205217. [PubMed] [Cross Ref]
24. Picton HM, Campbell BK, Hunter MG. Maintenance of oestradiol production and exression of cytochrome P450 aromatase enzyme mRNA in long-term serum-free cultures of pig granulosa cells. J Reprod Fertil. 1999;115(1):67–77. doi: 10.1530/jrf.0.1150067. [PubMed] [Cross Ref]
25. Schmierer B, Hill CS. TGFβ-SMAD signal transduction: molecular specificity and functional flexibility. Nat Rev Mol Cell Biol. 2007;8(12):970–982. doi: 10.1038/nrm2297. [PubMed] [Cross Ref]
26. Shimasaki S, Zachow RJ, Li DM, Kim H, Iemura SI, Ueno N, Sampath K, Chang RJ, Erickson GF. A functional bone morphogenetic protein system in the ovary. PNAS. 1999;96(13):7282–7287. doi: 10.1073/pnas.96.13.7282. [PubMed] [Cross Ref]
27. Shimasaki S, Moore RK, Erickson GF, Otsuka F. The role of bone morphogenetic proteins in ovarian function. Reprod Suppl. 2003;61:323–337. [PubMed]
28. Shimasaki S, Moore RK, Otsuka F, Erickson GF. The bone morphogenetic protein system in mammalian reproduction. Endocr Rev. 2004;25(1):72–101. doi: 10.1210/er.2003-0007. [PubMed] [Cross Ref]
29. Vitt UA, Hayashi M, Klein C, Hsueh AJ. Growth differentiation factor-9 stimulates proliferation but suppresses the follicle-stimulating hormone-induced differentiation of cultured granulosa cells from small antral and preovulatory rat follicles. Biol Reprod. 2000;62(2):370–377. doi: 10.1095/biolreprod62.2.370. [PubMed] [Cross Ref]
30. Winters TA, Hanten JA, Veldhuis JD. In situ amplification of the cytochrome P-450 cholesterol side-chain cleavage enzyme mRNA in single porcine granulosa cells by IGF-1 and FSH acting alone or in concert. Endocrine. 1998;9(1):57–63. doi: 10.1385/ENDO:9:1:57. [PubMed] [Cross Ref]
31. Yamashita Y, Kawashima I, Yanai Y, Nishibori M, Tichards JS, Shimada M. Hormone-induced expression of tumor necrosis factor α-converting enzyme/A disintegrin and metalloprotease-17 impacts porcine cumulus cell oocyte complex expansion and meiotic maturation via ligand activation of the epidermal growth factor receptor. Endocrinology. 2007;148(12):6164–6175. doi: 10.1210/en.2007-0195. [PubMed] [Cross Ref]

Articles from Journal of Zhejiang University. Science. B are provided here courtesy of Zhejiang University Press