Evaluation of steroidogenic capacity after follicle stimulating hormone stimulation in bovine granulosa cells of Revalor 200® implanted heifers
© Stapp et al.; licensee BioMed Central Ltd. 2014
Received: 17 September 2013
Accepted: 3 January 2014
Published: 7 January 2014
Heifers not used as breeding stock are often implanted with steroids to increase growth efficiency thereby altering hormone profiles and potentially changing the environment in which ovarian follicles develop. Because bovine granulosa cell culture is a commonly used technique and often bovine ovaries are collected from abattoirs with no record of implant status, the objective of this study was to determine if the presence of an implant during bovine granulosa cell development impacts follicle stimulating hormone-regulated steroidogenic enzyme expression. Paired ovaries were collected from 16 feedlot heifers subjected to 1 of 3 treatments: non-implanted (n = 5), Revalor 200 for 28 d (n = 5), or Revalor 200 for 84 d (n = 6). Small follicle (1 to 5 mm) granulosa cells were isolated from each pair and incubated with phosphate buffered saline (n = 16) or 100 ng/mL follicle stimulating hormone (n = 16) for 24 h.
Granulosa cells of implanted heifers treated with follicle stimulating hormone produced medium concentrations of progesterone similar (P = 0.22) to non-implanted heifers, while medium estradiol concentrations were increased (P < 0.10) at 28 and 84 d compared to non-implanted heifers indicating efficacy of treatment. Additionally, real-time PCR analysis in response to follicle stimulating hormone treatment demonstrated a decrease in steroidogenic acute regulatory protein (P = 0.05) mRNA expression in heifers implanted for 84 d and an increase in P450 side chain cleavage mRNA in granulosa cells of heifers implanted for 28 (P < 0.10) or 84 d (P < 0.05) compared to non-implanted females. However, no difference in expression of 3-beta-hydroxysteroid dehydrogenase (P = 0.57) and aromatase (P = 0.23) were demonstrated in implanted or non-implanted heifers.
These results indicate follicles which develop in the presence of high concentrations of androgenic and estrogenic steroids via an implant tend to demonstrate an altered capacity to respond to follicle stimulating hormone stimulation. Thus, efforts should be made to avoid the use of implanted heifers to study steroidogenesis in small follicle granulosa cell culture systems.
KeywordsBovine Follicle stimulating hormone Granulosa cells Implant Steroidogenesis
Combination trenbolone acetate (TBA) and estradiol-17β (E2) implants are commonly used in feedlot cattle to increase feed efficiency and muscle mass . However, exposure to exogenous hormones also influences other physiological functions. SJ Jones, RD Johnson, CR Calkins and ME Dikeman  demonstrated that implanted bulls had reduced cortisol and testosterone serum concentrations and smaller testicular size compared to non-implanted bulls. These data indicate that combination implants alter adrenal and gonadal steroid production and normal gonadal development.
In females, elevated concentrations of hormones, including estradiol, can alter ovarian function and steroid hormone synthesis. Anabolic agents used to enhance growth inhibit pituitary release of gonadotropins  as a result of the androgenic activity as exhibited by TBA  or the estrogenic activity . Consequently, implanting developing heifers has marked impacts on reproductive function. Heifers receiving a TBA and E2 implant at 84 d of age had delayed puberty and retardation in reproductive tract development . Ewes prenatally treated with testosterone during mid-gestation did not display a delay in onset of puberty but demonstrated absent or disrupted progestogenic cycles, and had larger follicles with prolonged presence . Heifers receiving a TBA implant at estrus or d 13 of the estrous cycle were anestrus for a period of time during growth promotant release, thereafter d 13 implanted heifers remained anestrus due to follicle or luteal cysts .
Though steroid implants are not intended for use in breeding females, bovine ovaries are often harvested from abattoirs for GC culture to investigate mechanisms regulating follicle maturation and differentiation. To our knowledge there is no study demonstrating the impact of elevated levels of androgens and estrogens on the developing follicle. Therefore, the objective of this study was to determine if the presence of anabolic and estrogenic steroids impacts follicle stimulating hormone (FSH)-regulated steroidogenic enzyme expression.
All procedures involving animals were approved by the Oklahoma State University Institutional Animal Care and Use Committee (AG-12-4). Sixteen predominantly Angus heifers (361 kg) were randomly assigned to one of three implant groups: non-implanted (n = 5), implanted for 28 d with a combination implant (200 mg TBA + 20 mg E2; Revalor 200®; Intervet, Inc., Millsboro, DE, USA; 28 d; n = 5), and 84 d with Revalor 200® (84 d; n = 6). Assigned heifers were implanted on d 0 (group implanted for 84 d) or d 56 (group implanted for 28 d) and were not re-implanted. Heifers were harvested on d 84 and 85 and paired ovaries were harvested (Robert M. Kerr Food and Agriculture Products Center, Oklahoma State University, Stillwater, OK) from each heifer for GC collection and culture.
Granulosa cell culture
Small follicle (1 to 5 mm) GC were isolated from ovaries of each animal and each animal’s GC were cultured separately using methods previously described . Follicle size selection was based on the intent of investigating FSH signaling cascades in implanted and non-implanted heifers. Previous observations indicate that 1) recruitment of bovine follicles able to respond to FSH occurs at a diameter of 1 to 3 mm ; 2) GC acquire FSH receptors prior to follicular recruitment [11, 12]; and 3) GC of recruited follicles express steroidogenic enzyme mRNAs before LH receptor mRNA is detected . Briefly, GC were resupended and washed twice in short-term media (1:1 mixture of Dulbecco’s Modified Eagle Medium (DMEM) and Ham’s F12 containing 0.12 mmol/L gentamycin and 38.5 mmol/L sodium bicarbonate) obtained from Sigma-Aldrich (St. Louis, MO, USA). After the final wash, cells were re-suspended in 0.5 to 2 mL of resuspension medium (serum-free medium with 2.5 mg/mL collagenase and 1 mg/mL DNase) (Sigma-Aldrich) to prevent cell clumping prior to plating. Cell number and viability were determined via hemocytometer using trypan blue dye exclusion. Granulosa cells from each animal were seeded in two-60-mm culture dishes at a density of 5.2 × 105 cells in DMEM complete medium (1:1 DMEM and Ham’s F-12 containing 10% fetal bovine serum, 0.12 mmol/L gentamycin, 2.0 mmol/L glutamine, and 38.5 mmol/L sodium bicarbonate). Incubation of cells occurred at 38.5˚C and 5% CO2 and medium was changed every 24 h until cell confluency reached 70-75%. Once confluency was reached, medium and unattached cells were removed. To test how each animal’s GC responded to FSH treatment, one culture dish of GC from each animal were incubated with phosphate buffered saline (PBS; Con; n = 16) in serum free media supplemented with 10-7 mol/L testosterone propionate (Sigma-Aldrich) for 24 h, allowing each animal to serve as its own control. The second culture dish was treated with 100 ng/mL purified human FSH (S1AFP-B-3; National Hormone and Peptide Program, National Institute of Diabetes and Digestive and Kidney Diseases, National Institutes of Health, Bethesda, MD, USA; n = 16) in serum free media supplemented with 10-7 mol/L testosterone propionate (Sigma-Aldrich) for 24 h. Treatment medium was collected and frozen at -80°C until analysis. Treatments were terminated by removing medium and rinsing cells once with ice cold PBS. Cells were scraped into 1 mL TRIzol (Invitrogen, Grand Island, NY, USA) reagent and stored at -80°C until isolation of RNA.
RNA extraction and quantitative real-time PCR
Primer sequences used in real-time PCR
Sequences of primers (5′-3′)
A working solution of cDNA was prepared by diluting 1:10 with DEPC-treated water. Five microliters of cDNA working solution was added to 20 μL master mix containing 13 μL SYBR green and fluorescein mix (Bioline, Taunton, MA, USA) and 0.75 μL of each forward primer (10 μmol/L) and reverse primer (10 μmol/L). Real-time PCR analysis for each sample was carried out in duplicate using a CFX real-time PCR detection system (Bio-Rad Laboratories, Hercules, CA, USA). Standard thermocycler conditions were as follows: 95°C for 10 min, followed by 40 cycles of 95°C for 15 s, 60°C for 30 s, and 72°C for 30 s. Relative fold change in target mRNAs was quantified using the ∆∆Cq method where the FSH ∆∆Cq for each animal was determined by subtracting each animals Con ∆Cq from their FSH ∆Cq . All reverse-transcribed cDNA samples were assayed in duplicate for each gene, and melt curve analyses were performed to ensure specificity of amplification. Melt curve analysis was carried out for 81 cycles with 0.5°C temperature increase from 55°C to 95°C.
To determine the appropriate reference gene to normalize cDNA variability between samples, a panel of three reference genes was analyzed including, glyceraldehyde-3-phosphate dehydrogenase (GAPDH), cyclophilin A (PPIA), and mitochondrial ribosomal protein L19 (MRPL19). The raw Cq values were obtained for each gene in all samples and analyzed using GeNorm (Biogazell qbasePLUS2, Zwijnaarde, Belgium) to determine the most stable normalization factor. The most stable housekeeping gene for target gene normalization was determined to be GAPDH and was used as the reference gene .
Granulosa cell culture medium was analyzed for E2 and progesterone (P4) by solid-phase radioimmunoassay using components of Siemens Medical Diagnostics Corp (Los Angeles, CA, USA) commercial kits as previously described . The E2 concentration in samples of cell culture medium was determined in 200 μL of medium and the specific binding was 62.5%. Detection limit (95% of maximum binding) of the assay was 2 pg/mL. Intra-assay CV for E2 was 6.5% for cell culture medium. The P4 concentration in samples of GC medium was assayed at 10 μL. The specific binding was 58.8%. Detection limit (95% of maximum binding) of the assay was 0.1 ng/mL. Intra-assay CV for P4 was 4.1% for cell culture medium.
Experiments were analyzed by analysis of variance for a completely randomized design in which three treatments were included; non-implanted (n = 5), Revalor 200® for 28 d (n = 5), and Revalor 200® for 84 d (n = 6). Relative fold changes in gene expression for steroidogenic acute regulatory protein (STAR), 3β-hydroxysteroid dehydrogenase (3β-HSD), P450 side chain cleavage (CYP11A1), and aromatase (CYP19A1) mRNA, and medium hormonal concentration of P4 and E2 are presented as the least square means ± standard error of the mean. For all culture experiments, GC from each animal were kept separate and each animal’s GC were subjected to either control treatment or FSH treatment. Thus, fold change values are each animal’s FSH response relative to that animal’s non-treated controls. A value in CYP11A1 mRNA expression of a non-implanted heifer at least three standard deviations from the mean and a missing fold change for CYP19A1 in the 84 d treatment group were excluded from statistical analysis. Quantitative real-time PCR data and hormone concentrations were analyzed using the GLM procedures of SAS (SAS Institute, Cary, NC, USA). Data were tested for homogeneity of variance using Hartley’s F max test and STAR and E2 were corrected by log transformation (log + 3 and log + 1, respectively). When a significant treatment effect was observed, means were separated using the least significant test computed by the predicted difference option of SAS. Statistical significance was set at P < 0.10.
Results and discussion
The anabolic effects of implants are likely a consequence of altering the endogenous hormonal milieu. This concept is supported by the demonstrated increase in plasma GH concentrations in response to E2 or TBA and E2 implants. High levels of anabolic hormones can also modulate reproduction as demonstrated by TBA induced anestrus in cows [8, 20] and delayed puberty and decreased fertility in TBA plus E2 implanted heifers compared to non-implanted controls [6, 21].
Based on the apparent change in estrogen production as a result of implant status and that estrogen production by the follicle is determined by FSH regulation of genes encoding key steroidogenic enzymes, we next evaluated gene expression of the steroidogenic enzymes of non-implanted and implanted heifers in response to FSH. Analysis of steroidogenic enzyme mRNAs of pubertal heifers implanted with TBA and E2 in the presence or absence of FSH demonstrated differences in expression as compared to non-implanted heifers. The first rate limiting step in steroid synthesis is the delivery of cholesterol to the inner mitochondrial membrane which is mediated by steroid acute regulatory protein (STAR). Expression of STAR was reduced (P < 0.05) in response to FSH in cells from heifers exposed to TBA and E2 for 84 d when compared to non-implanted heifers and heifers implanted for 28 d (Figure 2A). STAR is fundamental to the biosynthesis of steroid hormones as it provides cholesterol to the cytochrome P450 side-chain cleavage enzyme (CYP11A1). Mitochondrial CYP11A1 catalyzes the cleavage of the cholesterol side chain to form pregnenolone and this reaction represents the first committed step in steroidogenesis. Follicle stimulating hormone increased mRNA expression of CYP11A1, in GC from 28 d (P < 0.10) and 84 d (P < 0.05) implanted heifers as compared to non-implanted (Figure 2B). Studies indicate that both delivery of cholesterol to the enzyme system and the expression of CYP11A1 are important factors controlling the rate of steroid hormone synthesis  and may contribute to the increase in medium estrogen detected on d 28 and 84. In the female, ovarian androgens and estrogens regulate release of LH and FSH by feedback mechanisms on the hypothalamus and pituitary and it is not unexpected that exposure to anabolic steroids may disrupt this delicate balance. Elevated concentrations of anabolic and estrogenic steroids from the implants did not have a marked effect on mRNA expression of 3β-HSD (P = 0.57; Figure 2C) the enzyme responsible for converting pregnenolone to progesterone. Next, we evaluated CYP19A1, the enzyme in granulosa cells responsible for converting androgens to estrogen. However, no change in gene expression was detected for CYP19A1 in control versus heifers implanted for 28 or 84 d (P = 0.22; Figure 1D). This may be explained in part by the relatively short 3 h half-life of CYP19A1 in FSH-stimulated bovine granulosa cells compared to the more stable 14 h half-life demonstrated for CYP11A1.
Additionally, although implant status did not result in significant changes in CYP19A1 mRNA expression, E2 concentrations however, were elevated in both FSH treated implanted groups. This is consistent with previous work in cattle showing that minimal regulation in CYP19A1 gene expression can contribute to measurable differences in E2 synthesis [9, 25]. Normal follicular development relies on increasing concentrations of E2 corresponding with follicle maturation and resultant proliferation and differentiation of GC . Additionally, elevated levels of E2 in culture medium improves growth of oocytes from early antral follicles  supporting an important role of E2 in folliculogenesis. However, elevated exogenous concentration of E2 can increase the chance of developing cystic follicles and decreases fertility in heifers .
In conclusion, these results indicate that follicles which develop in the presence of high concentrations of androgenic and estrogenic steroids via an implant have an altered ability to respond to FSH stimulation as demonstrated by varied steroidogenic enzyme expression and elevated estradiol production. Thus, efforts should be made to avoid the use of implanted heifers to study steroidogenesis in small follicle GC culture systems.
Research supported by the Oklahoma Agric. Exp. Sta., Stillwater (OKL02789).
The authors would like to thank the NIDDK’s National Hormone & Peptide Program and A.F. Parlow for supplying the FSH reagent. Additionally, authors appreciate the Willard Sparks Beef Research Center personnel for overseeing care of experimental animals and lab members for assistance in granulosa cell collection.
- Johnson BJ, Anderson PT, Meiske JC, Dayton WR: Effect of a combined trenbolone acetate and estradiol implant on feedlot performance, carcass characteristics, and carcass composition of feedlot steers. J Anim Sci. 1996, 74 (2): 363-371.PubMedGoogle Scholar
- Jones SJ, Johnson RD, Calkins CR, Dikeman ME: Effects of trenbolone acetate on carcass characteristics and serum testosterone and cortisol concentrations in bulls and steers on different management and implant Schemes. J Anim Sci. 1991, 69 (4): 1363-1369.PubMedGoogle Scholar
- Cooper RA: Some aspects of the use of the growth promoter zeranol in ewe lambs retained for breeding: III. effect on plasma LH levels. Br Vet J. 1985, 141 (4): 424-426. 10.1016/0007-1935(85)90094-6.View ArticlePubMedGoogle Scholar
- Neumann F: Pharmacological and endocrinological studies on anabolic agents. Environ Qual Saf Suppl. 1976, 5: 253-264.PubMedGoogle Scholar
- Katzenellenbogen BS, Katzenellenbogen JA, Mordecai D: Zearalenones: characterization of the estrogenic potencies and receptor interactions of a series of fungal beta-resorcylic acid lactones. Endocrinology. 1979, 105 (1): 33-40. 10.1210/endo-105-1-33.View ArticlePubMedGoogle Scholar
- Moran C, Prendiville DJ, Quirke JF, Roche JF: Effects of oestradiol, zeranol or trenbolone acetate implants on puberty, reproduction and fertility in heifers. J Reprod Fertil. 1990, 89 (2): 527-536. 10.1530/jrf.0.0890527.View ArticlePubMedGoogle Scholar
- Manikkam M, Steckler TL, Welch KB, Inskeep EK, Padmanabhan V: Fetal programming: prenatal testosterone treatment leads to follicular persistence/luteal defects; partial restoration of ovarian function by cyclic progesterone treatment. Endocrinology. 2006, 147 (4): 1997-2007. 10.1210/en.2005-1338.View ArticlePubMedGoogle Scholar
- Reynolds IP, Harrison LP, Mallinson CB, Harwood DJ, Heitzman RJ: The effect of trenbolone acetate on the bovine estrous-cycle. Anim Reprod Sci. 1981, 4 (2): 107-116. 10.1016/0378-4320(81)90037-3.View ArticleGoogle Scholar
- Castañon BI, Stapp AD, Gifford CA, Spicer LJ, Hallford DM, Gifford JAH: Follicle-stimulating hormone regulation of estradiol production: possible involvement of WNT2 and β-catenin in bovine granulosa cells. J Anim Sci. 2012, 90: 3789-3797. 10.2527/jas.2011-4696.View ArticlePubMedGoogle Scholar
- Jaiswal RS, Singh J, Adams GP: Developmental pattern of small antral follicles in the bovine ovary. Biol Reprod. 2004, 71 (4): 1244-1251. 10.1095/biolreprod.104.030726.View ArticlePubMedGoogle Scholar
- Xu Z, Garverick HA, Smith GW, Smith MF, Hamilton SA, Youngquist RS: Expression of follicle-stimulating hormone and luteinizing hormone receptor messenger ribonucleic acids in bovine follicles during the first follicular wave. Biol Reprod. 1995, 53 (4): 951-957. 10.1095/biolreprod53.4.951.View ArticlePubMedGoogle Scholar
- Evans AC, Fortune JE: Selection of the dominant follicle in cattle occurs in the absence of differences in the expression of messenger ribonucleic acid for gonadotropin receptors. Endocrinology. 1997, 138 (7): 2963-2971.PubMedGoogle Scholar
- Bao B, Garverick HA, Smith GW, Smith MF, Salfen BE, Youngquist RS: Changes in messenger ribonucleic acid encoding luteinizing hormone receptor, cytochrome P450-side chain cleavage, and aromatase are associated with recruitment and selection of bovine ovarian follicles. Biol Reprod. 1997, 56 (5): 1158-1168. 10.1095/biolreprod56.5.1158.View ArticlePubMedGoogle Scholar
- Rozen S, Skaletsky H: Primer3 on the WWW for general users and for biologist programmers. Methods Mol Biol. 2000, 132: 365-386.PubMedGoogle Scholar
- Gifford CA, Racicot K, Clark DS, Austin KJ, Hansen TR, Lucy MC, Davies CJ, Ott TL: Regulation of interferon-stimulated genes in peripheral blood leukocytes in pregnant and bred, nonpregnant dairy cows. J Dairy Sci. 2007, 90 (1): 274-280. 10.3168/jds.S0022-0302(07)72628-0.View ArticlePubMedGoogle Scholar
- Kubista M, Andrade JM, Bengtsson M, Forootan A, Jonák J, Lind K, Sindelka R, Sjöback R, Sjögreen B, Strömbom L: The real-time polymerase chain reaction. Mol Aspects Med. 2006, 27 (2–3): 95-125.View ArticlePubMedGoogle Scholar
- Vandesompele J, De Preter K, Pattyn F, Poppe B, Van Roy N, De Paepe A, Speleman F: Accurate normalization of real-time quantitative RT-PCR data by geometric averaging of multiple internal control genes. Genome Biol. 2002, 3 (7): research0034.0031 - research0034.0011Google Scholar
- Rumsey TS, Elsasser TH, Kahl S: Roasted soybeans and an estrogenic growth promoter affect growth hormone status and performance of beef steers. J Nutr. 1996, 126 (11): 2880-2887.PubMedGoogle Scholar
- Hongerholt DD, Crooker BA, Wheaton JE, Carlson KM, Jorgenson DM: Effects of a growth hormone-releasing factor analogue and an estradiol-trenbolone acetate implant on somatotropin, insulin-like growth factor I, and metabolite profiles in growing Hereford steers. J Anim Sci. 1992, 70 (5): 1439-1448.PubMedGoogle Scholar
- Heitzman RJ, Harwood DJ: Residue levels of trenbolone and oestradiol-17beta in plasma and tissues of steers implanted with anabolic steroid preparations. Br Vet J. 1977, 133 (6): 564-571.PubMedGoogle Scholar
- Heitzman RJ, Harwood DJ, Kay RM, Little W, Mallinson CB, Reynolds IP: Effects of implanting prepuberal dairy heifers with anabolic steroids on hormonal status, puberty and parturition. J Anim Sci. 1979, 48 (4): 859-866.PubMedGoogle Scholar
- Langhout DJ, Spicer LJ, Geisert RD: Development of a culture system for bovine granulosa cells: effects of growth hormone, estradiol, and gonadotropins on cell proliferation, steroidogenesis, and protein synthesis. J Anim Sci. 1991, 69 (8): 3321-3334.PubMedGoogle Scholar
- Miller WL: Molecular biology of steroid hormone synthesis. Endocr Rev. 1988, 9 (3): 295-318. 10.1210/edrv-9-3-295.View ArticlePubMedGoogle Scholar
- Sahmi M, Nicola ES, Price CA: Hormonal regulation of cytochrome P450 aromatase mRNA stability in non-luteinizing bovine granulosa cells in vitro. J Endocrinol. 2006, 190 (1): 107-115. 10.1677/joe.1.06827.View ArticlePubMedGoogle Scholar
- Luo W, Gumen A, Haughian JM, Wiltbank MC: The role of luteinizing hormone in regulating gene expression during selection of a dominant follicle in cattle. Biol Reprod. 2011, 84 (2): 369-378. 10.1095/biolreprod.110.085274.View ArticlePubMedGoogle Scholar
- Richards JS, Midgley AR: Protein hormone action: a key to understanding ovarian follicular and luteal cell development. Biol Reprod. 1976, 14 (1): 82-94. 10.1095/biolreprod14.1.82.View ArticlePubMedGoogle Scholar
- Endo M, Kimura K, Kuwayama T, Monji Y, Iwata H: Effect of estradiol during culture of bovine oocyte–granulosa cell complexes on the mitochondrial DNA copies of oocytes and telomere length of granulosa cells. Zygote. 2012, 1-9.Google Scholar
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