Hostname: page-component-586b7cd67f-tf8b9 Total loading time: 0 Render date: 2024-11-28T22:53:02.805Z Has data issue: false hasContentIssue false

Effect of follicle size and atresia grade on mitochondrial membrane potential and steroidogenic acute regulatory protein expression in bovine granulosa cells

Published online by Cambridge University Press:  18 December 2018

Angela Ostuni
Affiliation:
Department of Sciences, University of Basilicata, Campus di Macchia Romana, Via dell’Ateneo Lucano, 10-85100 Potenza, Italy
Maria Pina Faruolo
Affiliation:
Department of Sciences, University of Basilicata, Campus di Macchia Romana, Via dell’Ateneo Lucano, 10-85100 Potenza, Italy
Carmen Sileo
Affiliation:
Department of Sciences, University of Basilicata, Campus di Macchia Romana, Via dell’Ateneo Lucano, 10-85100 Potenza, Italy
Agata Petillo
Affiliation:
Department of Sciences, University of Basilicata, Campus di Macchia Romana, Via dell’Ateneo Lucano, 10-85100 Potenza, Italy
Raffaele Boni*
Affiliation:
Department of Sciences, University of Basilicata, Campus di Macchia Romana, Via dell’Ateneo Lucano, 10-85100 Potenza, Italy
*
Address for correspondence: R. Boni. Campus di Macchia Romana, Via dell’Ateneo Lucano, 10 – 85100 Potenza, Italy. E-mail: [email protected]

Summary

During follicular development, granulosa cells undergo functional and structural changes affecting their steroidogenic activity. Oestrogen synthesis mainly occurs in the endoplasmic reticulum and relies on aromatase activity to convert androgens that arise from theca cells. In the present study, indicators of mitochondria-related steroidogenic capacity, as steroidogenic acute regulatory (StAR) protein expression and mitochondrial membrane potential (MMP), have been evaluated in bovine granulosa cells (GCs) and related to follicle growth and atresia. Atresia was estimated by morphological examination of follicle walls and cumulus–oocyte complexes (COC) and assessed by terminal deoxynucleotidyl transferase (TdT)-mediated dUTP nick end labeling (TUNEL) assay for apoptosis detection. Bovine ovarian follicles were macroscopically classified according to their atresia grade and grouped into small, medium or large follicles. After follicle opening, the COCs were morphologically classified for follicle atresia and the GCs were collected. Granulosa cells were fixed for immunofluorescence (IF) and TUNEL assay, frozen for western blotting (WB) or freshly maintained for MMP analyses. StAR protein expression was assessed using both IF and WB analyses. The follicle atresia grade could be efficiently discriminated based on either follicle wall or COC morphological evaluations. Granulosa cells collected from small non-atretic follicles showed a higher (P <0.01) MMP and WB-based StAR protein expression than small atretic follicles. For IF analysis, StAR protein expression in large atretic follicles was higher (P <0.05) than that in large non-atretic follicles. These results suggest a role played by mitochondria in GC steroidogenic activity, which declines in healthy follicles along with their growth. In large follicles, steroidogenic activity increases with atresia and is possibly associated with progesterone production.

Type
Research Article
Copyright
© Cambridge University Press 2018 

Access options

Get access to the full version of this content by using one of the access options below. (Log in options will check for institutional or personal access. Content may require purchase if you do not have access.)

References

Aitken, RJ, Gibb, Z, Mitchell, LA, Lambourne, SR, Connaughton, HS De Iuliis, GN (2012) Sperm motility is lost in vitro as a consequence of mitochondrial free radical production and the generation of electrophilic aldehydes but can be significantly rescued by the presence of nucleophilic thiols. Biol Reprod 87, 111.Google Scholar
Albertini, DF, Combelles, C, Benecchi, Carabatsos, MJ (2001) Cellular basis for paracrine regulation of ovarian follicle development. Reproduction 121, 647653.Google Scholar
Allen, JA, Shankara, T, Janus, P, Buck, S, Diemer, T, Held Hales, K Hales, DB (2006) Energized, polarized, and actively respiring mitochondria are required for acute Leydig cell steroidogenesis. Endocrinology 147, 39243935.Google Scholar
Anguita, B, Vandaele, L, Mateusen, B, Maes, D Van Soom, A (2007) Developmental competence of bovine oocytes is not related to apoptosis incidence in oocytes, cumulus cells and blastocysts. Theriogenology 67, 537549.Google Scholar
Armstrong, D, Goff, A Dorrington, J (1979) Regulation of follicular estrogen biosynthesis. In Ovarian follicular development and function (eds AR Midgley and WA Sadler) Raven Press, New York, pp. 169182.Google Scholar
Backway, KL, McCulloch, EA, Chow, S Hedley, DW (1997) Relationships between the mitochondrial permeability transition and oxidative stress during ara-C toxicity. Cancer Res 57, 24462451.Google Scholar
Bao, B, Calder, MD, Xie, S, Smith, MF, Salfen, BE, Youngquist, RS Garverick, HA (1998) Expression of steroidogenic acute regulatory protein messenger ribonucleic acid is limited to theca of healthy bovine follicles collected during recruitment, selection, and dominance of follicles of the first follicular wave. Biol Reprod 59, 953959.Google Scholar
Blondin, P Sirard, MA (1995) Oocyte and follicular morphology as determining characteristics for developmental competence in bovine oocytes. Mol Reprod Dev 41, 5462.Google Scholar
Boni, R, Cocchia, N, Silvestre, F, Tortora, G, Lorizio, R Tosti, E (2008) Juvenile and adult immature and in vitro matured ovine oocytes evaluated in relation to membrane electrical properties, calcium stores, IP3 sensitivity and apoptosis occurrence in cumulus cells. Mol Reprod Dev 75, 17521760.Google Scholar
Boni, R, Cuomo, A Tosti, E (2002) Developmental potential in bovine oocytes is related to cumulus–oocyte complex grade, calcium current activity, and calcium stores. Biol Reprod 66, 836842.Google Scholar
Boni, R, Gallo, A Cecchini, S (2017) Kinetic activity, membrane mitochondrial potential, lipid peroxidation, intracellular pH and calcium of frozen/thawed bovine spermatozoa treated with metabolic enhancers. Andrology 5, 133145.Google Scholar
Boni, R, Gallo, A, Montanino, M, Macina, A Tosti, E (2016) Dynamic changes in the sperm quality of Mytilus galloprovincialis under continuous thermal stress. Mol Reprod Dev 83, 162173.Google Scholar
Camp, TA, Rahal, JO Mayo, KE (1991) Cellular localization and hormonal regulation of follicle-stimulating hormone and luteinizing hormone receptor messenger RNAs in the rat ovary. Mol Endocrinol 5, 14051417.Google Scholar
De Wit, A, Wurth, Y Kruip, T (2000) Effect of ovarian phase and follicle quality on morphology and developmental capacity of the bovine cumulus–oocyte complex. J Anim Sci 78, 12771283.Google Scholar
Dorrington, JH, Moon, YS Armstrong, DT (1975) Estradiol-17β biosynthesis in cultured granulosa cells from hypophysectomized immature rats; stimulation by follicle-stimulating hormone. Endocrinology 97, 13281331.Google Scholar
Duarte, A, Castillo, AF, Podestá, EJ Poderoso, C (2014) Mitochondrial fusion and ERK activity regulate steroidogenic acute regulatory protein localization in mitochondria. PLoS One 9, e100387.Google Scholar
Eppig, J, Chesnel, F, Hirao, Y, O’Brien, M, Pendola, F, Watanabe, S Wigglesworth, K (1997) Oocyte control of granulosa cell development: how and why. Hum Reprod 12, 127132.Google Scholar
Falck, B (1960) Site of Production of oestrogen in rat ovary as studied in micro-transplants. Acta Physiol Scand 47, 1101.Google Scholar
Feng, W-G, Sui, H-S, Han, Z-B, Chang, Z-L, Zhou, P, Liu, D-J, Bao, S Tan, J-H (2007) Effects of follicular atresia and size on the developmental competence of bovine oocytes: a study using the well-in-drop culture system. Theriogenology 67, 13391350.Google Scholar
Gallo, A, Boni, R, Buttino, I Tosti, E (2016) Spermiotoxicity of nickel nanoparticles in the marine invertebrate Ciona intestinalis (ascidians). Nanotoxicology 10, 10961104.Google Scholar
Gallo, A, Menezo, Y, Dale, B, Coppola, G, Dattilo, M, Tosti, E Boni, R (2018) Metabolic enhancers supporting 1-carbon cycle affect sperm functionality: an in vitro comparative study. Sci Rep 8, 11769.Google Scholar
Garner, DL, Thomas, CA, Joerg, HW, Dejarnette, JM Marshall, CE (1997) Fluorometric assessments of mitochondrial function and viability in cryopreserved bovine spermatozoa. Biol Reprod 57, 14011406.Google Scholar
Gilchrist, R, Ritter, L Armstrong, D (2004) Oocyte–somatic cell interactions during follicle development in mammals. Anim Reprod Sci 82, 431446.Google Scholar
Gottlieb, E, Armour, S, Harris, M Thompson, C (2003) Mitochondrial membrane potential regulates matrix configuration and cytochrome c release during apoptosis. Cell Death Differ 10, 709717.Google Scholar
Guerrero-Netro, HM, Chorfi, Y Price, CA (2015) Effects of the mycotoxin deoxynivalenol on steroidogenesis and apoptosis in granulosa cells. Reproduction 149, 555561.Google Scholar
Henricks, DM (1991) Biochemistry and physiology of the gonadal hormones. In Reproduction in Domestic Animals (ed. PT Cupps), pp. 81118. Elsevier: San Diego, CA.Google Scholar
Hillier, SG, Whitelaw, PF Smyth, CD (1994) Follicular oestrogen synthesis: the ‘two-cell, two-gonadotrophin’ model revisited. Mol Cell Endocrinol 100, 5154.Google Scholar
Janowski, D, Salilew-Wondim, D, Torner, H, Tesfaye, D, Ghanem, N, Tomek, W, El-Sayed, A, Schell ander, K Hölker, M (2012) Incidence of apoptosis and transcript abundance in bovine follicular cells is associated with the quality of the enclosed oocyte. Theriogenology 78, 656669.e655.Google Scholar
Kluck, RM, Bossy-Wetzel, E, Green, DR Newmeyer, DD (1997) The release of cytochrome c from mitochondria: a primary site for Bcl-2 regulation of apoptosis. Science 275, 11321136.Google Scholar
Kruip, TA Dieleman, S (1982) Macroscopic classification of bovine follicles and its validation by micromorphological and steroid biochemical procedures. Reprod Nutr Dev 22, 465473.Google Scholar
Kruip, TA Dieleman, S (1985) Steroid hormone concentrations in the fluid of bovine follicles relative to size, quality and stage of the oestrus cycle. Theriogenology 24, 395408.Google Scholar
Landry, DA, Rossi-Perazza, L, Lafontaine, S Sirard, M-A (2018) Expression of atresia biomarkers in granulosa cells after ovarian stimulation in heifers. Reproduction 156, 239248.Google Scholar
Maillet, G, Breard, E, Benhaim, A, Leymarie, P Feral, C (2002) Hormonal regulation of apoptosis in rabbit granulosa cells in vitro: evaluation by flow cytometric detection of plasma membrane phosphatidylserine externalization. Reproduction 123, 243251.Google Scholar
Manna, PR, Dyson, MT Stocco, DM (2009) Regulation of the steroidogenic acute regulatory protein gene expression: present and future perspectives. Mol Hum Reprod 15, 321333.Google Scholar
Miglionico, R, Gerbino, A, Ostuni, A, Armentano, MF, Monné, M, Carmosino, M Bisaccia, F (2016) New insights into the roles of the N-terminal region of the ABCC6 transporter. J Bioenerg Biomembr 48, 259267.Google Scholar
Nebert, DW, Adesnik, M, Coon, MJ, Estabrook, RW, Gonzalez, FJ, Guengerich, FP, Gunsalus, IC, Johnson, EF, Kemper, B Levin, W (1987) The P450 gene superfamily: recommended nomenclature. DNA 6, 111.Google Scholar
Rodgers, R, Rodgers, H, Hall, P, Waterman, M Simpson, E (1986) Immunolocalization of cholesterol side-chain-cleavage cytochrome P-450 and 17α-hydroxylase cytochrome P-450 in bovine ovarian follicles. J Reprod Fertil 78, 627638.Google Scholar
Sahmi, M, Nicola, E, Silva, J Price, C (2004) Expression of 17β-and 3β-hydroxysteroid dehydrogenases and steroidogenic acute regulatory protein in non-luteinizing bovine granulosa cells in vitro . Mol Cell Endocrinol 223, 4354.Google Scholar
Stapp, AD, Gifford, CA, Hallford, DM Gifford, JAH (2014) Evaluation of steroidogenic capacity after follicle stimulating hormone stimulation in bovine granulosa cells of Revalor 200® implanted heifers. J Anim Sci Biotechnol 5, 2.Google Scholar
Thomas, FH, Ethier, J-F, Shimasaki, S V anderhyden, BC (2005) Follicle-stimulating hormone regulates oocyte growth by modulation of expression of oocyte and granulosa cell factors. Endocrinology 146, 941949.Google Scholar
Tosti, E, Boni, R, Gallo, A Silvestre, F (2013) Ion currents modulating oocyte maturation in animals. Syst Biol Reprod Med 59, 6168.Google Scholar
Wu, LL-Y, Dunning, KR, Yang, X, Russell, DL, Lane, M, Norman, RJ Robker, RL (2010) High-fat diet causes lipotoxicity responses in cumulus–oocyte complexes and decreased fertilization rates. Endocrinology 151, 54385445.Google Scholar
Wurth, YA, Boni, R, Hulshof, SCJ Kruip, TAM (1994) Bovine embryo production in vitro after selection of ovaries, follicles and oocytes. In Bovine Embryo Production In Vitro: Influencing Factors (eds SW de Laat, CJG Wensing and TA Kruip), pp. 6785. Odijk. The Netherlands: Utrecht University Press.Google Scholar
Yang, MY Rajamahendran, R (2000) Morphological and biochemical identification of apoptosis in small, medium, and large bovine follicles and the effects of follicle-stimulating hormone and insulin-like growth factor-I on spontaneous apoptosis in cultured bovine granulosa cells 1. Biol Reprod 62, 12091217.Google Scholar
Zeuner, A, Müller, K, Reguszynski, K Jewgenow, K (2003) Apoptosis within bovine follicular cells and its effect on oocyte development during in vitro maturation. Theriogenology 59, 14211433.Google Scholar
Zhang, JY, Wu, Y, Zhao, S, Liu, ZX, Zeng, SM Zhang, GX (2015) Lysosomes are involved in induction of steroidogenic acute regulatory protein (StAR) gene expression and progesterone synthesis through low-density lipoprotein in cultured bovine granulosa cells. Theriogenology 84, 811817.Google Scholar
Zhu, L, Yuan, H, Guo, C, Lu, Y, Deng, S, Yang, Y, Wei, Q, Wen, L He, Z (2012) Zearalenone induces apoptosis and necrosis in porcine granulosa cells via a caspase-3- and caspase-9-dependent mitochondrial signaling pathway. J Cell Physiol 227, 18141820.Google Scholar