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Since cAMP blocks meiotic maturation of mammalian and amphibian oocytes in vitro and cyclic nucleotide phosphodiesterase 3A (PDE3A) is primarily responsible for oocyte cAMP hydrolysis, we generated PDE3A-deficient mice by homologous recombination. The Pde3a–/– females were viable and ovulated a normal number of oocytes but were completely infertile, because ovulated oocytes were arrested at the germinal vesicle stage and, therefore, could not be fertilized. Pde3a–/– oocytes lacked cAMP-specific PDE activity, contained increased cAMP levels, and failed to undergo spontaneous maturation in vitro (up to 48 hours). Meiotic maturation in Pde3a–/– oocytes was restored by inhibiting protein kinase A (PKA) with adenosine-3′,5′-cyclic monophosphorothioate, Rp-isomer (Rp-cAMPS) or by injection of protein kinase inhibitor peptide (PKI) or mRNA coding for phosphatase CDC25, which confirms that increased cAMP-PKA signaling is responsible for the meiotic blockade. Pde3a–/– oocytes that underwent germinal vesicle breakdown showed activation of MPF and MAPK, completed the first meiotic division extruding a polar body, and became competent for fertilization by spermatozoa. We believe that these findings provide the first genetic evidence indicating that resumption of meiosis in vivo and in vitro requires PDE3A activity. Pde3a–/– mice represent an in vivo model where meiotic maturation and ovulation are dissociated, which underscores inhibition of oocyte maturation as a potential strategy for contraception.
Although competent to complete meiosis, mammalian oocytes are physiologically arrested in prophase I (prophase of the first meiotic division) until shortly before ovulation. Through protein kinase A–catalyzed (PKA-catalyzed) phosphorylation of unidentified proteins, cAMP prevents activation of maturation-promoting factor (MPF) and MAPK signaling in oocytes and inhibits the spontaneous maturation that occurs in vitro, thus maintaining meiotic arrest (1–5). It is unclear, however, whether the same mechanisms of meiotic arrest operate in vivo during each reproductive cycle, where preovulatory gonadotrophin triggers resumption of meiosis and progression through the second meiotic division until metaphase II. Only oocytes arrested in metaphase II can be fertilized.
Cyclic AMP apparently plays an important role in maintaining meiotic arrest in mammalian oocytes. The interplay of signals arising in both follicle cells and oocytes themselves (1, 2, 4, 6, 7) regulates synthesis and degradation of oocyte cAMP via adenylyl cyclases and cyclic nucleotide phosphodiesterases (PDEs), respectively. Cyclic AMP may enter oocytes from adjacent cumulus cells via gap junctions (2, 6). Recent studies in rodents, however, demonstrated that active oocyte adenylyl cyclase contributes to meiotic blockade (8), which can be released by microinjection of oocytes with antibodies that inactivate Gs, the heterotrimeric GTP-binding protein that activates adenylyl cyclase (9). These studies imply that generation of intra-oocyte cAMP is sufficient to maintain meiotic arrest. In Xenopus oocytes, meiotic arrest involves PKA-induced phosphorylation of protein phosphatase CDC25 (10), and in oocytes from sterile female Cdc25b–/– mice, which are arrested in prophase I, microinjection of CDC25B reinitiated meiosis (11), suggesting that phosphorylation/dephosphorylation of critical effectors is important in oocyte maturation (1, 3, 5, 10, 11).
PDEs belong to a complex and diverse superfamily of at least 11 structurally related, highly regulated, and functionally distinct gene families (PDE1–PDE11), which differ in their primary structures, affinities for cAMP and cGMP, responses to specific effectors, sensitivities to specific inhibitors, and regulatory mechanisms (12). Most PDE families comprise more than one gene, which generate multiple protein products via alternative mRNA splicing or utilization of different promoters and/or transcription initiation sites. The two PDE3 subfamilies, PDE3A and PDE3B, are encoded by closely related genes (13). PDE3A is relatively highly expressed in oocytes, platelets, and cardiac, vascular, and airway myocytes; PDE3B, in adipose tissue, liver, and pancreas, as well as cardiovascular tissues (13–16). PDE3 inhibitors increase myocardial contractility, inhibit platelet aggregation, and enhance vascular and airway smooth muscle relaxation (12, 13). Activation of PDE3B is thought to be important in the antilipolytic and antiglycogenolytic actions of insulin, as well as in IGF1- and leptin-induced inhibition of cAMP-stimulated secretion of insulin from pancreatic islets (16–19). Other studies suggest that, in pancreatic islets, PDE3B regulates intracellular cAMP pools that modulate glucose- and glucagon-like peptide-1–stimulated (GLP1-stimulated) insulin release (20, 21).
Oocyte cAMP hydrolysis is thought to be primarily accomplished by PDE3A (22, 23), and selective PDE3 (not PDE4 or PDE5) inhibitors block meiotic resumption and oocyte maturation in Xenopus oocytes, cultured murine, macaque, and human oocytes, and in vivo in cycling rats (in the latter, without affecting ovulation) (1, 22–27). Moreover, murine oocyte maturation, induced by microinjection of an active PDE (3), is associated with decreases in cAMP (28, 29). In Xenopus oocytes, progesterone-induced inhibition of adenylyl cyclase and IGF1-induced activation of cAMP hydrolysis (via an enzyme with properties of PDE3) both signal by reducing cAMP (1, 30, 31). We previously reported that heterologous expression of PDE3A in Xenopus oocytes induced activation of mos translation and MAPK and resumption of meiosis (32).
To understand specific physiological roles of PDE3A, and to elucidate the role of cyclic nucleotides in oocyte maturation and female infertility, we generated mice deficient in PDE3A. These PDE3A-deficient mice represent the first murine genetic model demonstrating that disruption of cAMP signaling leads to meiotic arrest of oocytes and female infertility, that the processes of meiotic maturation and ovulation are dissociated, and that PDE3A is essential for oocyte maturation and subsequent fertilization.
To establish a model for delineating PDE3A functions, we generated PDE3A-deficient mice by homologous recombination in embryonic stem cells (Figure (Figure1).1). Since multiple PDE3A isoforms, generated from the single Pde3a gene, are found in cardiovascular tissues (33, 34), Pde3a–/– mice were generated by a targeted disruption of exon 13, which encodes a portion of the PDE3A catalytic domain (Figure (Figure1).1). As seen in Figure Figure1,1, mouse Pde3a (MPde3a) exon 13, encoding a portion of the second putative metal-binding site in the center of the PDE3A catalytic domain (Figure (Figure1A),1A), was replaced by the neomycin phosphotransferase II (NPTII) coding sequence (Figure (Figure1B).1B). Homologous recombination was confirmed by Southern blots (Figure (Figure1C,1C, top) or PCR of genomic DNA (Figure (Figure1C,1C, bottom). The mRNA of the rearranged gene, however, was transcribed and translated as shorter mutant PDE3A forms (Figure (Figure1,1, D and E), lacking that portion of the catalytic domain encoded by exon 13 (Figure (Figure1D).1D). The immunoreactive, smaller, mutant PDE3A forms are expressed at low levels in Pde3a–/– mice and are much less abundant than intact WT PDE3A (Figure (Figure1E).1E). Consistent with PDE3A being the predominant PDE in murine oocytes (22, 23) and PDE3B being absent from oocytes (14, 15), and with the mutant form of PDE3A being catalytically inactive, PDE3 activity was undetectable in isolated Pde3a–/– oocytes (Figure (Figure2A),2A), and cAMP content was greater in denuded Pde3a–/– than in Pde3a+/+ oocytes (P = 0.003) (Figure (Figure22B).
Because cells contain representatives of several PDE gene families, PDE3 activity in different tissue homogenates was measured (35) as that fraction of total PDE activity inhibited by 1 mM cilostamide, a specific PDE3 inhibitor. Cilostamide, however, inhibits both PDE3A and PDE3B isoforms with similar potency. As seen in Figure Figure2C,2C, there was also almost complete loss of PDE3 activity in homogenates from Pde3a–/– lungs, indicating that PDE3A is the predominant PDE3 expressed in lung. PDE3 activity was also markedly reduced in homogenates from Pde3a–/– hearts. Consistent with relatively high expression of PDE3B in liver and adipose tissue, PDE3 activities were only slightly lower in those tissues from Pde3a–/– mice than from WT Pde3a+/+ mice (Figure (Figure2C).2C). Further investigation by gel filtration chromatography demonstrated that PDE3B could account for the residual low levels of PDE3 activity detected in lung homogenates prepared from Pde3a–/– mice (Figure (Figure22D).
Mice lacking PDE3A were viable and exhibited no obvious growth or developmental deficiencies. Male Pde3a–/– mice were fertile and produced viable offspring, whereas female Pde3a–/– mice were completely sterile, whether mated to Pde3a–/– or Pde3a+/+ males (Table (Table1).1). Female Pde3a+/– mice were also fertile, which indicates that the residual, catalytically inactive, shorter mutant PDE3A forms (cf. Figure Figure1,1, D and E) did not interfere with oocyte function by acting as “dominant negative” PDE3A forms. Pde3a–/– ovarian structure and morphology were unremarkable, with a normal complement of corpora lutea and antral follicles, which suggests normal folliculogenesis and ovulation (Figure (Figure3,3, A–H). As also seen in Figure Figure3,3, I–L, after injection of female mice with pregnant mare serum gonadotropin (PMSG) and human chorionic gonadotropin (hCG), cumulus expansion was normal and observed in ovarian follicles of both Pde3a+/+ and Pde3a–/– mice. Whereas the Pde3a+/+ oocyte progressed to metaphase, as evidenced by the presence of a metaphase spindle (Figure (Figure3,3, I and J), the Pde3a–/– oocyte remained arrested in meiotic prophase I, as demonstrated by the persistence of the nuclear germinal vesicle (GV), classified as the GV stage (Figure (Figure3,3, K and L). Although Pde3a–/– mice exhibit normal mating behavior and spontaneous and PMSG/hCG-stimulated ovulation (Table (Table2),2), nonfertilized Pde3a–/– oocytes retrieved from the ampulla (Table (Table2)2) also were arrested in meiotic prophase I (GV stage), as demonstrated by the persistence of the nuclear germinal vesicle (Figure (Figure4B).4B). After mating, two-cell embryos were collected from oviducts of Pde3a+/+ females (Table (Table22 and Figure Figure4A),4A), whereas immature GV-stage oocytes with sperm in the perivitelline space were retrieved from Pde3a–/– oviducts (Figure (Figure4B).4B). Thus, sterility of Pde3a–/– females, which apparently exhibit normal estrous cycles, ovulation, and mating behavior, is most likely related to the inability of Pde3a–/– oocytes to resume meiosis in response to the normal luteinizing hormone surge or exogenously administered gonadotropins.
As shown in Figure Figure4,4, C–H, immediately after harvesting from ovarian follicles (time 0), both Pde3a+/+ (Figure (Figure4C)4C) and Pde3a–/– (Figure (Figure4D)4D) oocytes contained intact GV, an interphase-like distribution of microtubules, and perinucleolar condensation of chromatin (surrounded nucleolus [SN] conformation). After removal from follicles, Pde3a+/+ oocytes, but not Pde3a–/–oocytes, resumed meiosis and completed germinal vesicle breakdown (GVBD) by approximately 3 hours, which was followed by extrusion of polar body (PB) (Figure (Figure5,5, A–C). After 20 hours in culture, Pde3a+/+ oocytes exhibited a well-defined spindle apparatus with condensed and aligned chromosomes typical of metaphase II (Figure (Figure4E).4E). In contrast, even after 20 hours, denuded Pde3a–/– oocytes did not resume meiosis in vitro and remained blocked at the GV stage, with an interphase pattern of dispersed tubulin and partially condensed chromatin (Figure (Figure4F).4F). MPF and MAPK were activated during spontaneous maturation (at 18 hours) of cultured Pde3a+/+ oocytes, but not Pde3a–/– oocytes (Figure (Figure5D).5D). Moreover, meiosis did not resume in cumulus-oocyte complexes cultured up to 12 hours with or without follicle-stimulating hormone (FSH), although the hormonal treatment produced normal expansion of cumulus cells (data not shown). Thus, complete blockade of spontaneous or gonadotropin-induced meiotic resumption occurs in Pde3a–/– oocytes.
Consistent with the absence of oocyte PDE3A, cAMP levels were higher in Pde3a–/– than in Pde3a+/+ oocytes (cf. Figure Figure2B).2B). Given the proposed role of cAMP and PKA in maintenance of meiotic arrest (1–5), in vitro treatment of Pde3a–/– oocytes with PKA inhibitors Rp-8-Br-cAMPS or adenosine-3′,5′-cyclic monophosphorothioate, Rp-isomer (Rp-cAMPS) induced resumption of meiosis (Figure (Figure5E).5E). As expected, incubation of Pde3a+/+ oocytes with cilostamide, a PDE3 inhibitor, blocked GVBD (Figure (Figure5E),5E), presumably due to high levels of cAMP and activation of PKA. Similar to effects of Rp-cAMPS in Pde3a–/– oocytes, incubation of cilostamide-treated Pde3a+/+ oocytes with Rp-cAMPS (Figure (Figure5E)5E) or Rp-8-Br-cAMPS (data not shown) induced resumption of meiosis. As seen in Figure Figure4,4, G–H, after treatment with Rp-8-Br-cAMPS, both Pde3a+/+ (Figure (Figure4G)4G) and Pde3a–/– oocytes (Figure (Figure4H)4H) appeared as mature eggs at metaphase II. Resumption of meiosis in Pde3a–/– oocytes occurred after only a brief exposure to PKA inhibitors (Figure (Figure5F).5F). Treated Pde3a–/– oocytes exhibited activated MPF and MAPK (Figure (Figure6A)6A) and were competent for fertilization in vitro (Figure (Figure6B).6B). Microinjection of PKI or protein phosphatase cdc25b mRNA also initiated resumption of meiosis in Pde3a–/– oocytes (Figure (Figure66C).
The PDE gene superfamily apparently encodes more than 50 PDE proteins (12). Some cells are relatively enriched in specific PDEs; these include oocytes (22, 23) and retinal rods and cones (12), in which PDE3A and PDE6, respectively, are the predominant PDEs. Most cells, however, contain representatives of at least several PDE gene families and different subfamily isoforms from the same gene family, but in different amounts, proportions, and subcellular locations (12). Family-specific PDE inhibitors can pharmacologically define functions of individual PDEs and, in cells containing multiple PDEs, dissect out effects of specific PDEs in regulating specific signaling pathways and cellular functions. For example, PDE3 inhibitors, but not PDE4 inhibitors, increase insulin secretion in cultured pancreatic b cells (HIT-T15 or HIT cells), despite greater effects of PDE4 inhibitors on cAMP content in these cells (17, 18). In the female reproductive system, differential cellular expression of PDE4 and PDE3 isoforms in granulosa cells and oocytes, respectively, seems to be important in the integrating signals involved in luteinizing hormone (LH) induction of oocyte maturation, which apparently involves opposing effects of cAMP in somatic and germ cells (1, 15). Actions of PDE4 inhibitors in follicle cells enhance effects of LH on oocyte maturation, whereas PDE3 inhibitors act directly in oocytes, increasing cAMP and suppressing meiotic progression (1, 15). In PDE4D KO mice, however, the rate of ovulation and, consequently, fertility, is reduced (36). Other reports further support the view that multiplicity of PDEs does not serve merely a survival or protective function, but that differentially regulated and targeted PDEs are critical for selective compartmentalization and modulation of cyclic nucleotide signals and responses (37, 38).
Analysis of the phenotypic characteristics of mice with a targeted disruption of the Pde3a gene indicates that, in oocytes, PDE3A plays a unique role, which is apparently not replaced or functionally compensated for by other PDE gene families or by the other PDE3 family member, PDE3B. Inactivation of the Pde3a gene results in a phenotype characterized by female infertility. Despite normal ovarian structure, folliculogenesis, ovulation, and mating behavior, female PDE3A KO mice are sterile, most likely due to specific and direct effects of the absence of PDE3A in oocytes — i.e., inhibitory effects of elevated cAMP on meiotic progression and oocyte maturation and, consequently, the competency of oocytes for fertilization. Additional studies with PDE3A KO mice will undoubtedly prove useful in elucidating other physiological roles of PDE3A.
Targeted disruption of Pde4 genes has also similarly generated mice with unique phenotypes (36, 39–41). Analyses of these phenotypes support the concept that the ability of different PDEs to subserve different physiological roles is, at least in part, genetically determined. For example, PDE3B KO mice, although fertile and not frankly diabetic, demonstrate alterations in regulation of energy homeostasis and signs of insulin resistance (our unpublished data). Thus, discrete, nonoverlapping signaling pathways are disrupted when genes encoding specific PDEs are inactivated or when specific PDEs are pharmacologically inhibited, which thus supports the concept that different PDEs are functionally nonredundant and regulate different cAMP/cGMP pools and responses.
Although increases in cAMP and activation of PKA are crucial in the induction and maintenance of meiotic arrest, the precise targets and downstream effectors of cAMP signalling have not been completely defined (1, 42). Recent studies suggest that PKA may affect two parallel pathways that regulate activation of MPF (3, 10, 42, 43). PKA apparently blocks translation of Mos (the oocyte MAPK), perhaps by inhibiting polyadenylation of its mRNA (43). In frog oocytes, Mos activates MAPK, leading to inhibition of MYT1, a kinase that phosphorylates and inhibits MPF (3, 10, 42, 43). In addition, PKA-catalyzed phosphorylation of CDC25 may result in its sequestration by 14-3-3 and thus negatively regulate CDC25-induced activation of MPF (10).
The rapid reversal of cAMP/PKA-induced meiotic arrest by PKA inhibitors in Pde3a–/– oocytes (cf. Figures Figures55 and and6)6) is consistent with the reported activation of PDE3A (23) and decrease in cAMP (28, 29) that apparently precede spontaneous or hCG-induced maturation of murine oocytes. Thus, a brief period of reduced PKA activity (via PKA inhibition in Pde3a–/– oocytes or activation of PDE3A and reduction in cAMP and PKA activity in murine oocytes) is sufficient to trigger resumption of meiosis. If cAMP is assumed to remain elevated in Pde3a–/– oocytes after removal of the PKA inhibitors, reactivation of PKA apparently does not affect meiotic progression. From this, one may infer that PKA activity per se is not critical, but rather it is the temporal and spatial distribution and localization of cAMP signals and/or signaling pathways and modules (37, 38, 44, 45) that organize and orchestrate the signals that regulate meiotic arrest and progression. Research has indicated that during oocyte maturation, A-kinase–anchoring proteins (AKAPs) (44, 45) might compartmentalize, and thereby regulate actions of, PKA and other effector molecules, i.e., protein kinases and phosphatases and other scaffolding proteins. Whether PDE3A is physically targeted to these putative spatially segregated signaling modules (similar to the association of PDE4 isoforms with AKAP in regulating ryanodine-sensitive channels [ref. 46] or with β-arrestin in downregulation of the β-adrenergic receptor [ref. 47]), and/or regulates their signaling output, is uncertain. These considerations are also consistent with recent studies indicating that some of the inhibitory effects of PKA on meiotic arrest may be independent of kinase activity and perhaps mediated via its direct interaction with and sequestration of critical regulatory effectors rather than via phosphorylation of these molecules (48).
Taken together, these experiments strongly suggest that absence of PDE3A in oocytes leads to high levels of cAMP, persistent activation of PKA, and phosphorylation of critical regulatory effectors, resulting in inhibition of MPF/MAPK signals involved in resumption of meiosis and subsequent development of competency for fertilization (Figure (Figure7).7). Under these conditions, the physiological signal that triggers meiosis in vivo is ineffective, which underscores the critical role of PDE3A in meiotic resumption and female fertility. Thus, Pde3a–/– mice provide a novel genetic model for studies of female sterility and present the possibility that some idiopathic infertility in women may be the result of mutations that cause inactivation of this gene. More importantly, the apparently reversible, perhaps “physiological,” nature of the meiotic arrest in Pde3a–/– oocytes clearly suggests — along with earlier reported in vivo and in vitro effects of PDE3 inhibitors on meiotic progression and oocyte maturation (26, 27) — that PDE3A could be an excellent potential target for contraceptives (Figure (Figure7).7). It should be pointed out that ovulation and oocyte maturation are completely dissociated in the Pde3a–/– mouse, which emphasizes the concept that oocyte maturation can be targeted independently of somatic cells and without affecting the hormonal milieu. At the present time, however, use of PDE3 inhibitors, such as cilostamide or cilostazol, as contraceptives is not feasible, since inhibitors specific for PDE3A or PDE3B isoforms have not been developed, and methods to selectively target oocyte PDE3A are not available. Nevertheless, as outlined in Figure Figure7,7, Pde3a–/– mice provide a valuable model in which to dissect and reconstitute signaling pathways downstream of cAMP that regulate meiosis in oocytes (and perhaps division and proliferation in other cAMP-responsive cells). It is also conceivable that some of these downstream effectors and pathways will offer more accessible and efficacious contraceptive targets.
Pde3a–/– mice were generated by a targeted disruption of exon 13, which encodes a portion of the second putative metal-binding site in the center of the PDE3A catalytic domain. The pKO Scrambler NTK Vector-1903 (Stratagene, La Jolla, California, USA) was used to construct the replacement vector. An approximately 16-kb SalI genomic DNA fragment, containing five putative exons (exons 10–14) that encode much of the catalytic domain of MPDE3A, was isolated from a 129/SvJ l FIXII mouse genomic library (Stratagene), using a [32P]-labeled probe generated from a cDNA clone containing the catalytic domain of rat PDE3A. A 7.0-kb SacI DNA fragment containing putative exons 11–14 was subcloned from this original clone into pUC18 (SacI site). This 7.0-kb genomic subclone includes an approximately 1.5-kb AocI restriction fragment that contains exon 13. Two segments, SacI-AocI (~2.0 kb, called fragment A) and AocI-SacI (~3.5 kb, called fragment B) were amplified by PCR and purified. Fragment A was digested with Ecl136II and EcoRI; fragment B, with BamHI and Ecl136II. These were sequentially cloned into the two polylinker sites of the pKO Scrambler NTK vector upstream and downstream of the region containing the NPTII coding sequence (Neo), the phosphoglycerol kinase (PGK) promoter, and the bovine growth hormone (BGH) polyadenylation (polyA) signal. The targeting vector thus consisted of fragment A containing MPde3a exons 11 and 12, the NPTII coding sequence, fragment B containing MPde3a exon 14, and the TK coding sequence. The vector was linearized and electroporated into 129/SvJ ES cells (Genome Sciences, St. Louis, Missouri, USA) where, by homologous recombination, MPde3a exon 13 was replaced by the NPTII coding sequence. Positive ES cell clones, identified by Southern blots and PCR, were microinjected into C57BL/6J blastocysts and implanted into pseudopregnant females. The resulting chimera was mated with C57BL/6J to produce the F1 generation. F1 Pde3a+/– heterozygous mice were mated to generate Pde3a–/– mice (designated as C57BL/6J-129/SvJ). For some of the experiments described herein, C57BL/6J-129/SvJ mice were mated with Black Swiss mice (Taconic Farms, Germantown, New York, USA) to generate Black Swiss/C57BL/6J-129/SvJ mice.
To confirm the MPde3a genetic rearrangement, DNA was extracted from tail samples and analyzed by Southern blots and PCR. Since the Neo sequence introduced a BamH1 site into the Pde3a–/– genome, DNA was digested with BamHI, separated by agarose-gel electrophoresis, and hybridized with a 32P-labeled probe designed to detect intron 10, upstream from fragment A. Restriction fragments of approximately 12 kb and approximately 7.5 kb from Pde3a+/+ and Pde3a–/– mice, respectively, were predicted and observed. The PCR primers designed to detect the normal (+) allele (forward primer [FP]: 5′-TGCTATACAACGACCGTTCT-3′, reverse primer (RP): 5′-ATGACTAGGAAGCGGAAGTG-3′) amplified exon 13 (~136 bp), while PCR primers designed to detect the mutant (–) allele (FP: 5′- GATGGCTGGCAACTAGAAGG-3′, RP: 5′-CATACGCTTGATCCGGCTAC-3′) amplified the NPTII coding sequence (~487 bp). Reactions were conducted using the Advantage GC-cDNA polymerase mix (BD Biosciences, San Jose, California, USA) in the GeneAmp 9700 thermal cycler (Applied Biosystems, Foster City, California, USA), for 1 minute at 94°C, 10 seconds at 94°C, 45 seconds at 60°C, and 2 minutes at 68°C for 35 cycles, and final extension, 7 minutes at 68°C.
Pde3a+/+ and Pde3a–/– C57BL/6J-129/SvJ mice were generated and maintained and studies performed in accord with protocols approved by animal care and use committees at NHLBI, NIH, and Stanford University School of Medicine. After mice (3–6 weeks old) were sacrificed by asphyxiation (CO2), ovaries were harvested, placed in maturation medium (MEM [Invitrogen Corp., Carlsbad, California, USA] with 2 mM L-glutamine [Invitrogen Corp.], 25 mM HEPES [Sigma-Aldrich, St. Louis, Missouri, USA], 100 U/ml penicillin [Invitrogen Corp.], 100 μg/ml streptomycin [Invitrogen Corp.], 0.23 mM sodium pyruvate [Sigma-Aldrich], and 3 mg/ml BSA [Sigma-Aldrich]), and punctured with a fine needle to release cumulus-oocyte complexes from the antral follicles. Denuded oocytes were obtained by repeated pipetting with a pulled Pasteur pipette and, after washing, were incubated under embryo-tested mineral oil (Sigma-Aldrich) for indicated times in a drop (~0.05 ml) of maturation medium without or with the indicated concentrations of Rp-8-Br-cAMPS (Calbiochem; EMD Biosciences, La Jolla, California, USA) or Rp-cAMPS in a 5% CO2 atmosphere at 37°C. To induce “superovulation,” females (6 to 12 weeks old) were injected with 5 U/mouse of pregnant mare serum gonadotropin (PMSG) (Sigma-Aldrich) and, 44–46 hours later, injected intraperitoneally) with 5 U/mouse of hCG (Cortex Biochem, San Leandro, California, USA). In some experiments, female mice were sacrificed 9 hours after hCG injection; ovaries were collected, fixed in Bouin’s solution, embedded, sectioned stained with H&E, and analyzed for the presence of cumulus expansion and progression of oocyte meiosis in vivo. In other experiments, after hCG injection, females were caged with males, and the following morning, after being checked for the presence of vaginal plugs, were sacrificed by asphyxiation (CO2). Oviducts were dissected, ovulated oocytes and two-cell–stage embryos were collected and incubated in maturation medium, and oocytes were examined for their meiotic stage under a dissecting stereomicroscope (model Stemi SV6; Carl Zeiss Inc., Thornwood, New York, USA). Oocytes showing clear nuclear membranes (GV) and nucleoli were classified as GV stage; those without visible nuclear structure and exhibiting GVBD were classified as GVBD stage; and metaphase II–arrested oocytes, with a PB, were classified as PB stage (27). After spontaneous or induced ovulation, the ovulated cells were examined; those at the two-cell stage were classified as embryos, whereas those still exhibiting a clear GV were defined as GV stage ovulated oocytes. Progression of meiotic maturation of denuded oocytes in vitro was scored by monitoring GVBD with an inverted microscope fitted with a Hoffman contrast lens.
Twenty to 30 oocytes were fixed for 1 hour at room temperature (rt) in 2% paraformaldehyde in PBS, washed 5 times in blocking solution (PBS, pH7.4, containing 0.3% BSA [Sigma-Aldrich] and 100 mM glycine [ICN Biomedicals Inc., Costa Mesa, California, USA)]), permeabilized with blocking solution containing 0.1% Triton X-100 (Sigma-Aldrich), washed 3 times in blocking solution, and incubated 1 hour (rt) under embryo-tested mineral oil (Sigma-Aldrich) in 0.05 ml of anti–α-tubulin antibody (Accurate Chemical and Scientific Corp., Westburn, New York, USA), which had been diluted 1:100 in blocking solution. After five washes in blocking solution, the oocytes were incubated for 1 hour (rt) in 0.05 ml of the secondary, Alexa Fluor 488–conjugated anti-rat antibody (Molecular Probes, Eugene, Oregon, USA), and washed 5 times. After 10 minutes in PBS, pH 8.1/glycerol (1:1 vol/vol), the oocytes were mounted in mounting medium (DAPI; Vectashield, Burlingame, California, USA) using a Hybaid Easyseal frame (Continental Lab Products, San Diego, California, USA) with regular glass slides and coverslips and viewed with a confocal microscope (Leica Microsystems, Heidelberg, Germany).
Denuded oocytes from Pde3a–/– and Pde3a+/+ mice (20 for each PDE assay) were collected within 30 minutes after follicle puncture in Leibowitz’s L-15 medium (Invitrogen Corp., Grand Island, New York, USA) with 5% FBS and 100 IU/ml penicillin/streptomycin, washed, and frozen in PBS (3 μl). Immediately before assay, 20 μl of IPA buffer (10 mM sodium phosphate buffer, pH 7.2, 50 mM NaF, 150 mM NaCl, 2 mM EDTA, 5 mM mercaptoethanol, 30 mM pyrophosphate, 3 mM benzamidine, 5 μg/ml leupeptin, 20 μg/ml pepstatin, 2 mM PMSF, 1 μM microcystin, and 0.5% Triton X-100) were added. Samples were centrifuged at 12,000 g at 4°C for 30 minutes, supernatants collected, and PDE activity was measured for 20 minutes.
After sacrifice of mice by asphyxiation (CO2), heart, lung, liver, and fat pads were dissected from 3–3.5–month-old C57BL/6J-129/SvJ males, quickly washed in ice-cold PBS, and homogenized (5 ml/g tissue) in buffer (50 mM HEPES, pH 7.5 [Sigma-Aldrich], 25 mM KCl [Sigma-Aldrich], 5 mM MgCl2 [Quality Biological Inc., Gaithersburg, Maryland, USA], protease inhibitor cocktail tablets [Roche, Nutley, New Jersey, USA]) with a rotor-stator homogenizer (Omni International, Marietta, Georgia, USA) at 30,000 rpm (15 to 90 seconds, on ice), followed by homogenization (on ice, 20 strokes in a glass Dounce tissue grinder [B pestle; Thomas Scientific, Swedesboro, New Jersey, USA]) and sonification (on ice, 20 pulses, 40% duty cycle, output scale 4). NP-40 (Calbiochem) (1% final) was then added and samples incubated (on ice, 1 hour), before centrifugation (15,000 g, 20 minutes, 4°C). Supernatants (total tissue lysates) were used for PDE assays (35) or gel filtration chromatography (FPLC-superose 12; AKTA FPLC System; Amersham-Pharmacia Biotech Inc., Piscataway, New Jersey, USA). For PDE assays, samples (usually 5–15 μg protein in 100 μl) were incubated for 10 minutes in a total volume of 0.3 ml containing 50 mM HEPES, pH 7.4, 100 μM EGTA, 8.3 mM MgCl2, and [3H]-cAMP. PDE3 activity is that portion of total PDE activity inhibited by 1 mM cilostamide (Calbiochem), a specific PDE3 inhibitor. Inhibitor vehicle, DMSO (Sigma-Aldrich), added in equal quantities to samples without inhibitors, did not alter PDE activity. Protein was determined by BCA protein assay (Pierce, Rockford, Illinois, USA).
Samples of solubilized tissue homogenates (~100 mg protein) were subjected to SDS-PAGE (4–12% Tris-Glycine gels [Invitrogen Corp., Carlsbad, California, USA]). After electrophoretic transfer, nitrocellulose membranes were blocked overnight at 4°C in T-PBS (0.05% Tween 20 [Bio-Rad Laboratories, Hercules, California, USA] in PBS) containing 5% non-fat dry milk (Bio-Rad Laboratories) and 1% BSA, incubated 1–4 hours with the indicated primary antibody diluted in T-PBS/5% milk, washed and incubated 1 hour with HP-conjugated secondary antibody against rabbit IgG (Amersham-Pharmacia Biotech Inc.) diluted 1:4000 in T-PBS. The signal was detected using ECL-Plus Detection System (Amersham-Pharmacia Biotech Inc.).
Primary antibodies, which were purified by chromatography on DEAE columns, included: rabbit IgG raised against a peptide corresponding to AAs 424–460 (regulatory domain) of human PDE3A, diluted 1:400 in T-PBS/5% milk; rabbit IgG raised against a peptide corresponding to AAs 2–18 (N-terminal domain) of rat PDE3B, diluted 1:200 in T-PBS/5% milk.
Groups of 50 denuded oocytes were collected in L-15 medium, quickly washed, and frozen in PBS (3 μl). After thawing and extraction with 100 μl of 0.1% trichloroacetic acid in 95% ethyl alcohol, followed by centrifugation (800 g, 30 min, 4°C), the supernatant was dried, and the residue dissolved in PBS (100 μl). After acetylation, cAMP content was measured by radioimmunoassay (8).
Harvested oocytes were incubated for the indicated times prior to in vitro assay of MPF and MAPK as described (49), using histone H1 and myelin basic protein (MBP) as substrates, respectively. Briefly, 3 denuded oocytes (in 1.5 μl of maturation medium) were immediately frozen on dry ice in 3.5 μl of lysis buffer (7 μg/ml aprotinin, 7 μg/ml leupeptin, 7 mM p-nitrophenyl phosphate, 14 mM β-glycerophosphate, 70 μM sodium orthovanadate, and 3.5 mM EGTA) and stored at –80°C prior to assay)10 μl final vol, 30 min at 30°C, 2 mg/ml histone [type III-S], 0.5 mg/ml MBP, and 500 μCi/ml [γ-32P]ATP [3,000 Ci/mmol; Amersham-Pharmacia Biotech Inc.]). Reactions were terminated and proteins separated by SDS-PAGE (15% gels), followed by gel drying and exposure to x-ray film.
Denuded Pde3a–/– oocytes were exposed to 5 mM Rp-cAMPS in maturation medium for 2 hours, washed, and incubated overnight at 37°C in L-15 medium supplemented with 5% fetal bovine serum and 100 IU/ml penicillin/streptomycin. After 20 hours, oocytes at MII stage were incubated with capacitated sperm in modified KSOM embryo culture medium containing 5.6 mM glucose and 4 mg/ml BSA. After 4 hours, oocytes and attached sperm were transferred to fresh medium and further incubated at 37°C in 5% CO2 for 20 hours.
Marco Conti is supported in part by The National Institute of Child Health and Human Development, NIH, though a cooperative agreement (U54-HD31398), as part of the Specialized Cooperative Centers Program in Reproduction Research. We also wish to thank Martha Vaughan (NHLBI) for her critical reading of the manuscript and Faiyaz Ahmad (NHLBI) and Tanya Hoodbhoy (National Institute of Diabetes and Digestive and Kidney Diseases) for advice and technical assistance.
S. Masciarelli and K. Horner contributed equally to characterization of the phenotype of PDE3A–/– mice.
The PDE3A/PDE3B nomenclature in this report conforms to that suggested by a PDE nomenclature group (50). In an earlier report (14), the PDE3A/PDE3B nomenclature had been reversed. An erratum (see ref. 14) was published to correct and clarify this nomenclature discrepancy.
Nonstandard abbreviations used: adenosine-3′,5′-cyclic monophosphorothioate, Rp-isomer (Rp-cAMPS); A-kinase anchoring protein (AKAP); cyclic nucleotide phosphodiesterase (PDE); follicle-stimulating hormone (FSH); germinal vesicle breakdown (GVBD); glucagon-like peptide-1 (GLP1); human chorionic gonadotropin (hCG); luteinizing hormone (LH); maturation promoting factor (MPF); mouse Pde3a (MPde3a); neomycin phosphotransferase II (NPTII); polar body (PB); pregnant mare serum gonadotropin (PMSG); protein kinase A (PKA); protein kinase inhibitor peptide (PKI).
Conflict of interest: The authors have declared that no conflict of interest exists.