Mitochondrial Stress Response Gene Clpp Is Not Required for Granulosa Cell Function

Mitochondrial unfolded protein response (UPRmt) is a highly conserved mechanism, which is activated upon cellular or metabolic stress and aims to help cells maintain homeostasis. CLPP (caseinolytic peptidase P) plays a crucial factor for UPRmt; it promotes the degradation of unfolded mitochondrial proteins. Global germline deletion of Clpp in mice results in female infertility and accelerated follicular depletion. Here, we asked whether CLPP is necessary for granulosa/cumulus cell function. Clppflox/flox mice were generated and crossbred with Cyp19a1-Cre mice to generate mice with granulosa/cumulus cell-specific Clpp deletion (Clpp−/−). Mature (8-week-old) Clpp−/− female mice (8-week-old) were compared to same age wild type (WT) mice. We found that mature Clpp−/− female mice were fertile and produced a similar number of pups per litter compared to WT. Folliculogenesis was not affected by the loss of CLPP in granulosa/cumulus cells as Clpp−/− and WT mice had a similar number of primordial, primary, secondary, early antral, and antral follicles. The number of germinal vesicles (GV) and MII oocytes collected from Clpp−/− and WT female mice were also similar. Our findings demonstrate that fertility in female mice is not affected by granulosa/cumulus cell-specific UPRmt disruption through CLPP deletion.


Introduction
Mitochondria play a central role in cellular energy production. Within the mitochondrial matrix, acetyl CoA molecules derived from glycolysis or fatty acid beta-oxidation enter the Krebs (citric acid) cycle, which results in the generation of reduced forms of NADH and FADH2, in addition to ATP [1]. Then, NADH and FADH2 move to the electron transport chain (ETC) localized at the inner mitochondrial membrane, become reduced to NAD+ and FAD, respectively, and result in further ATP generation through oxidative phosphorylation (OXPHOS) [1]. The aerobic (oxidative) mitochondrial mechanisms involved in energy generation are extremely efficient and result in a net gain of 38 ATP molecules per each glucose molecule metabolized, compared to only two that can be generated through anaerobic glycolysis in the cytoplasm.
Mitochondrial oxidative metabolism may also result in the generation of reactive oxygen species (ROS), such as hydrogen peroxide (H 2 O 2 ). When the amount of ROS is in excess of the cell's antioxidant response capacity, oxidative stress ensues and may lead to DNA damage and cell death. Mitochondria have several protective mechanisms used to maintain mitochondrial hemostasis, including the mitochondrial unfolded protein response (UPR mt ), which becomes activated when signs of mitochondrial stress, such as accumulation of unfolded or misfolded proteins, are detected [2][3][4][5]. As initially characterized in Caenorhabditis elegans, UPR mt causes increased expression of mitochondrial CLPP protease (Caseinolytic peptidase P), which cleaves misfolded proteins [6][7][8]. Cleavage of misfolded proteins and subsequent transport of cleavage products to the cytosol results in the activation of the transcription factor ATFS1, which then enters the nucleus and induces transcription of mitochondrial chaperones and ROS detoxification enzymes [3,8,9]. In addition, UPR mt induces glycolysis, mitochondrial fission, and coenzyme Q biosynthesis [3,10,11], altering mitochondrial metabolism and dynamics to promote mitochondrial function and cell survival during stress. UPR mt and the role of CLPP are conserved in mammals (reviewed in [12]).
Key metabolic functions of mitochondria make these organelles important determinants of female reproductive function and oocyte and embryo viability [13]. The number, size, and shape of mitochondria appear to be tightly controlled throughout oogenesis and early embryo development [14]. In mice, several models with targeted deletion of mitochondrial function genes result in infertility [15][16][17]. In humans, oocyte ATP production is associated with embryonic development [18], and some studies correlate mitochondrial DNA content of trophoectoderm biopsies obtained from blastocysts in women undergoing in vitro fertilization (IVF) with reproductive potential of euploid embryos [19,20], whereas other studies do not demonstrate such an association [21].
In a recent article, Wang et al. used a mouse model with a global germline deletion of Clpp to characterize the role of CLPP in female reproduction. They found that female mice lacking Clpp are infertile and their ovaries show accelerated follicular depletion, consistent with diminished ovarian reserve. In addition, these mice generate a lower number of mature oocytes and two-cell embryos, and do not make blastocysts [15]. These findings are consistent with the conclusions of another study that found female mice with global deletion of Clpp to be sterile and have altered follicular histology [22]. Although these studies generated highly interesting and relevant data, they did not determine which reproductive cell type (somatic vs. gonadal) is primarily dependent on CLPP for its function. In addition, the role of CLPP in granulosa/cumulus cells under conditions associated with mitochondrial stress has not yet been studied. Therefore, in the current study, we used a targeted deletion strategy that removed Clpp in granulosa/cumulus cells.

Animal Breeding and Genotyping
Sperm carrying mutant Clpp allele in C57BL/6 background with reporter-tagged insertion were purchased from Wellcome Trust Sanger Institute (Colony ID: EPD0665_3_D05) and used to fertilize wild-type (WT) female mice oocytes through in vitro fertilization (IVF). WT surrogate carriers were used to generate offspring (n = 6). Half of the offspring (n = 3) carrying the mutant allele were crossbred with a mouse carrying FLP gene following vendor instructions to obtain mice with Clpp flox allele. Female mice (n = 3) with Clpp flox allele were fertilized with sperm with Cyp19a1-Cre (where Cre is driven by Cyp19a1 promoter), which was obtained from the University of California Davis (stock number: 037056-UCD-SPERM) to obtain a generation of mice with Clpp flox /Cyp19a1-Cre ( Figure 1). Colony numbers gradually expanded as needed.
Genotyping was carried out using primers listed in Supplementary Table S1. For simplicity, mice with cumulus cell-specific Clpp deletion, i.e., Clpp flox /Cyp19a1-Cre mice, will be referred to as Clpp −/− hereafter. Female Clpp −/− mice and their WT litter mates were used for the experiments detailed below. Mice care, breeding, and experimental procedures were conducted according to Yale University animal research requirements, using protocols approved by Institutional Animal Care and Use Committee (protocol #2020-11207).Genotyping was carried out using primers listed in Supplementary Table S1. For simplicity, mice with cumulus cell-specific Clpp deletion, i.e., Clpp flox /Cyp19a1-Cre mice, will be referred to as Clpp −/− hereafter. Female Clpp −/− mice and their WT litter mates were used for the experiments detailed below. Mice care, breeding, and experimental procedures were conducted according to Yale University animal research requirements, using protocols approved by Institutional Animal Care and Use Committee (protocol #2020-11207). For simplicity, mice with cumulus cell-specific Clpp deletion, i.e., Clpp flox /Cyp19a1-Cre mice, will be referred to as Clpp −/− hereafter. Female Clpp −/− mice and their WT litter mates were used for the experiments detailed below. Mice care, breeding, and experimental procedures were conducted according to Yale University animal research requirements, using protocols approved by Institutional Animal Care and Use Committee (protocol #2020-11207).
Quantitative Reverse Transcription-Polymerase Chain Reaction (qRT-PCR) RNA was extracted from pooled cumulus cells(CCs) obtained from ten cumulus oocyte complexes (COCs) per mice, liver, uterus, and kidney (n = 5 for each genotype per experiment) using an RNAqueous Micro Kit (Invitrogen, Carlsbad, CA). Reverse transcription was performed following manufacturer's instructions in two sequential steps using a RETROscript Kit (Invitrogen, Carlsbad, CA). Briefly, to eliminate any secondary structures, extracted RNA and random decamers were incubated at 85 °C for 3 min. This was followed by adding buffer, reverse transcriptase enzyme, RNAse inhibitor, and dNTP mix and incubating at 42 °C for 1 h. cDNA obtained from this reaction was assessed in triplicate using an iCycler (Bio-Rad Laboratories, Hercules, CA). For each 10 μL reaction, 5 μL SYBR Green Supermix (Bio-Rad Laboratories, Hercules, CA), 1 μL of each primer, 2 μL H2O, and 1 μL cDNA were used. Each experiment was repeated at least three times using different animals of the same genotype each time. The 2 (−ΔΔCT) (cycle threshold) method was used to assess relative expression levels after normalization to β-actin levels. Primers used in qRT-PCR are listed in Supplementary Table S1.

Fertility Assessment
To evaluate the fertility of Clpp −/− female mice, 2-month-old Clpp −/− and WT (n = 6, for each group) were mated with adult WT males with proven fertility. In each cage, one female mouse was hosted with one male mouse for 12 weeks. The number of litters and pups were recorded with daily monitoring.

Histomorphometric Analysis of Folliculogenesis in Ovaries
Histomorphometric analysis was performed on ovarian sections stained with hematoxylin and eosin (H&E). Ovaries from 2-, 6-, and 9-month-old Clpp −/− and WT (both ovaries of 3 mice for each genotype at each age group) were collected and fixed in 4% (w/v) paraformaldehyde in Dulbecco's phosphate-buffered saline (Sigma, St. Louis, MO, USA) at room temperature overnight. They were then dehydrated and embedded in paraffin. Five micrometer (μm) serial sections were obtained and stained with H&E using standard RNA was extracted from pooled cumulus cells(CCs) obtained from ten cumulus oocyte complexes (COCs) per mice, liver, uterus, and kidney (n = 5 for each genotype per experiment) using an RNAqueous Micro Kit (Invitrogen, Carlsbad, CA). Reverse transcription was performed following manufacturer's instructions in two sequential steps using a RETROscript Kit (Invitrogen, Carlsbad, CA). Briefly, to eliminate any secondary structures, extracted RNA and random decamers were incubated at 85 • C for 3 min. This was followed by adding buffer, reverse transcriptase enzyme, RNAse inhibitor, and dNTP mix and incubating at 42 • C for 1 h. cDNA obtained from this reaction was assessed in triplicate using an iCycler (Bio-Rad Laboratories, Hercules, CA). For each 10 µL reaction, 5 µL SYBR Green Supermix (Bio-Rad Laboratories, Hercules, CA), 1 µL of each primer, 2 µL H2O, and 1 µL cDNA were used. Each experiment was repeated at least three times using different animals of the same genotype each time. The 2 (−∆∆CT) (cycle threshold) method was used to assess relative expression levels after normalization to β-actin levels. Primers used in qRT-PCR are listed in Supplementary Table S1.

Fertility Assessment
To evaluate the fertility of Clpp −/− female mice, 2-month-old Clpp −/− and WT (n = 6, for each group) were mated with adult WT males with proven fertility. In each cage, one female mouse was hosted with one male mouse for 12 weeks. The number of litters and pups were recorded with daily monitoring.

Histomorphometric Analysis of Folliculogenesis in Ovaries
Histomorphometric analysis was performed on ovarian sections stained with hematoxylin and eosin (H&E). Ovaries from 2-, 6-, and 9-month-old Clpp −/− and WT (both ovaries of 3 mice for each genotype at each age group) were collected and fixed in 4% (w/v) paraformaldehyde in Dulbecco's phosphate-buffered saline (Sigma, St. Louis, MO, USA) at room temperature overnight. They were then dehydrated and embedded in paraffin. Five micrometer (µm) serial sections were obtained and stained with H&E using standard protocols [23]. Every 5th section (a total of 35 sections per ovary) was marked and assessed. Only follicles containing a visible nucleus were counted to determine the number of primordial, primary, secondary, early antral, and antral follicles as previously described [24]. The total number of follicles counted were reported without normalization. Primordial follicles were defined with an oocyte surrounded by a single layer of squamous granulosa cells. Primary follicles were formed by an oocyte surrounded by a single layer of cuboidal granulosa cells. Secondary follicles contained an oocyte surrounded by two or more layers of cuboidal granulosa cells. Early antral follicles and antral follicles possessed an oocyte with four or more layers of surrounding granulosa cells multiple small antral spaces and one large antral space, respectively.

Oocyte and Cumulus Cell Collection
Germinal vesicle (GV) stage oocytes, oocytes at metaphase of second meiotic division (MII), and cumulus cells were obtained by superovulation of mature 2-month-old Clpp −/− and WT mice as previously described [25]. To obtain GV stage oocytes, mice were euthanized by CO 2 inhalation 44 h after intraperitoneal injection of 5IU PMSG. Ovaries were removed and punctured in M2 medium (Sigma, St. Louis, MO, USA) with 10 µM milrinone (Sigma, St. Louis, MO, USA) under dissecting microscope (Olympus SZH-ILLK) with 26-1/2-gauge needle to isolate cumulus-oophorus complexes containing GV stage oocytes and cumulus cells. Oocytes were stripped from neighboring cumulus cells with a mouth pipette and collected in individual tubes. To obtain mature, M2 stage oocytes, 5IU of human chorionic gonadotropin (hCG; Sigma, St. Louis, MO, USA) was injected intraperitoneally 48 h after PMSG injection. Unfertilized MII oocytes were collected from mice oviducts 14 h after hCG injection. To collect fertilized embryos, females were mated with WT males immediately after the hCG injection. The following morning, mating was confirmed by the presence of a vaginal plug. Two-cell embryos were collected 44 h after hCG injection from the oviducts in KSOM medium (Millipore, Darmstadt, Germany). Blastocysts were collected 92 h after hCG injection from uterus into M2 medium (Sigma, St. Louis, MO, USA).

Quantification of mtDNA Copy Number in Cumulus Cells and Oocytes
To quantify mtDNA in cumulus cells and oocytes, Cox3 plasmid fragment was amplified by subcloning into pCR TM 2.1-TOPO ® -colony vector (Invitrogen, Carlsbad, CA, USA), as previously described [14]. One-Shot TOP10 Chemically Competent E. coli was transformed with plasmid and grown overnight at 37 • C. The recombinant plasmid was then purified using Qiagen plasmid isolation kit (catalogue number 27104) and the inserted mtDNA fragment was confirmed by DNA sequence analysis. The amount of plasmid DNA was quantified using a NanoDrop 2000 spectrophotometer (Thermo Scientific, Waltham, MA, USA). A standard curve with 10 9 to 10 2 plasmid molecules was generated by serial 10-fold dilutions. Individual GV stage oocytes and approximately 50 cumulus cells stripped from cumulus-oophorus complexes of 2-month-old Clpp −/− and WT mice (n = 3) were lysed in 10 µl lysis solution at 55 • C for 2 h. Lysis solution was inactivated at 95 • C for 10 min and the mix was used directly for qPCR in triplicate as previously described [15]. Individual oocytes' and aggregate cumulus cells' mtDNA copy numbers were extrapolated from the standard curve.

Determination of ROS Levels
Reactive oxygen species (ROS) generation was induced by exposing COCs from 2month-old Clpp −/− and WT mice to 20mM H 2 O 2 dissolved in M2 medium for 5 min at 37 • C. COCs were then washed 3 times with M2 medium and incubated in M2 medium containing 6-carboxy-2 , 7 -dichlorodihydrofluorescein diacetate (carboxy-H2DCFDA) (Life Technologies, Thermofisher Scientific, Carlsbad, CA, USA). Carboxy-H2DCFDA is a nonfluorescent chemical, which has the ability to pass through the plasma membrane and converts to green fluorescent upon oxidation with ROS [26]. H2DCFDA is a fluorescent probe commonly employed and may react with several ROS, including hydrogen peroxide, hydroxyl radicals, and peroxynitrite. The cell-permeant H2DCFDA passively diffuses into cells and is retained in the intracellular level after cleavage by intracellular esterases. Upon oxidation by ROS, the nonfluorescent H2DCFDA is converted to the highly fluorescent 2',7' dichlorofluorescein (DCF) [26]. A quantity of 5 µL of H2DCFDA was dissolved in 1 mL of M2 medium, and COCs were incubated for 20 min at 37 • C in the dark. COCs were then washed with H2DCFDA-free media and images were captured with a Leica SP5 spectral scanning confocal microscope. Fluorescence in images was quantified using Image J software (National Institute of Health). In total, 5 COCs per group were analyzed for each experiment; experiments were repeated 3 times.

Statistical Analysis
All statistical analysis was performed using Graph Pad Prism software, version 8.3.0. The Student's t-test was used to analyze statistical significance between groups. Quantitative analysis was expressed as mean ± SEM and significance was assessed at p < 0.05.

Lack of Clpp in Granulosa/Cumulus Cells did not Affect Fertility Potential in Mice
The fertility of mature Clpp −/− mice was similar to that of WT females ( Table 1). Loss of CLPP in cumulus cells of female mice did not affect fertility potential compared to same-age WT counterparts. After 12 weeks of mating with male WT mice with proven fertility, the total number of litters (15 vs. 15, n = 6) and litters per female mouse (2.50 ± 0.5 vs. 2.50 ± 0.5, p = 1) was the same. The total number of pups obtained from Clpp −/− and WT mothers was also similar (122 vs. 120). There was no significant change in pups per litter (8.13 ± 1.28 vs. 8.00 ± 1.70, p > 0.05) between Clpp −/− and WT female mice. Fertility of female Clpp −/− and WT mice (8-week-old, n = 4 for each genotype) was assessed by mating with WT males of proven fertility (male/female; 1:1) for 12 weeks.
Clpp −/− mice had a similar litter size (pups per litter) and litters per female compared with WT females.

Immature and Mature Oocyte Production was not Altered in Mice with Granulosa/Cumulus Cell-Specific Deletion of Clpp
GV or MII oocyte production was not affected by CLPP loss in cumulus cells. In 2month-old mice, Clpp −/− and WT mice produced a similar number of GV stage oocytes (38.4 ± 8.7 vs. 42.8 ± 5.4; p = 0.37). The number of mature, MII stage oocytes was also not significantly different between the two groups (21.3 ± 6.8 vs. 23

Clpp −/− Cumulus Cells did not have any Abnormal mtDNA Copy Number or ROS Production
Mitochondrial copy number in both cumulus cells and oocytes were similar in mature Clpp −/− and WT female mice. In cumulus cells, mtDNA copy numbers for Clpp −/− and WT were 27,793,262 ± 9,070,406 and 24,163,434 ± 10,191,895, respectively (p = 0.24). In GV-stage oocytes collected from Clpp −/− and WT mice, mtDNA numbers were 5,826,568 ± 1,688,408 and 6,422,192 ± 3,047,395, respectively (p = 0.45). These parameters were not different between the groups (Figure 4).

Clpp −/− Cumulus Cells did not have any Abnormal mtDNA Copy Number or ROS Production
Mitochondrial copy number in both cumulus cells and oocytes were similar in mature Clpp −/− and WT female mice. In cumulus cells, mtDNA copy numbers for Clpp −/− and WT were 27,793,262 ± 9,070,406 and 24,163,434 ± 10,191,895, respectively (p = 0.24). In GVstage oocytes collected from Clpp −/− and WT mice, mtDNA numbers were 5,826,568 ± 1,688,408 and 6,422,192 ± 3,047,395, respectively (p = 0.45). These parameters were not different between the groups (Figure 4).
Loss of CLPP did not have a significant effect on the ROS production of cumulus cells. The percentage of ROS in cumulus cells of secondary follicles collected from 2month-old Clpp −/− and WT mice were not significantly different (10.8 ± 2.86 vs. 8.4 ± 1.24, p = 0.13) (Figure 4). In each experiment, five mice were included in each group, and five GV oocytes/mice (a total of 25 GV oocytes per experiment) were analyzed. Each experiment was repeated three times. (B) mtDNA copy number was determined by qPCR in granulosa/cumulus cells collected from 2month-old Clpp −/− and WT mice. In each experiment, five mice were included in each group, and granulosa/cumulus cells obtained from five COCs/mice (a total of 25 COCs per experiment) were analyzed. Each experiment was repeated three times. (C) Fluorescence intensity of carboxy-H2DCFDA was used to measure ROS levels in cumulus-oophorus complexes after treatment with H2O2. (D) Pixel intensity in granulosa cumulus cells is reported using Image J. Data presented as mean ± SEM.

Discussion
CLPP plays a central role in UPR mt by promoting degradation of unfolded or misfolded mitochondrial proteins. We had previously demonstrated that the global deletion of Clpp in mice results in female infertility and accelerated follicular depletion [15]. In the current study, we investigated whether CLPP expression in granulosa/cumulus cells is required for reproductive competence. We found the fertility of mature female mice with targeted deletion of Clpp in granulosa/cumulus cells to be similar to that of WT. Our findings suggest that, although CLPP is an essential protein for UPR mt and its global expression is required for female and male fertility [15,22], follicular somatic cell CLPP expression is not a requirement for female fertility. In each experiment, five mice were included in each group, and five GV oocytes/mice (a total of 25 GV oocytes per experiment) were analyzed. Each experiment was repeated three times. (B) mtDNA copy number was determined by qPCR in granulosa/cumulus cells collected from 2-month-old Clpp −/− and WT mice. In each experiment, five mice were included in each group, and granulosa/cumulus cells obtained from five COCs/mice (a total of 25 COCs per experiment) were analyzed. Each experiment was repeated three times. (C) Fluorescence intensity of carboxy-H2DCFDA was used to measure ROS levels in cumulus-oophorus complexes after treatment with H 2 O 2 . (D) Pixel intensity in granulosa cumulus cells is reported using Image J. Data presented as mean ± SEM.
Loss of CLPP did not have a significant effect on the ROS production of cumulus cells. The percentage of ROS in cumulus cells of secondary follicles collected from 2month-old Clpp −/− and WT mice were not significantly different (10.8 ± 2.86 vs. 8.4 ± 1.24, p = 0.13) (Figure 4).

Discussion
CLPP plays a central role in UPR mt by promoting degradation of unfolded or misfolded mitochondrial proteins. We had previously demonstrated that the global deletion of Clpp in mice results in female infertility and accelerated follicular depletion [15]. In the current study, we investigated whether CLPP expression in granulosa/cumulus cells is required for reproductive competence. We found the fertility of mature female mice with targeted deletion of Clpp in granulosa/cumulus cells to be similar to that of WT. Our findings suggest that, although CLPP is an essential protein for UPR mt and its global expression is required for female and male fertility [15,22], follicular somatic cell CLPP expression is not a requirement for female fertility.
In the current study, we evaluated follicle development in mice with granulosa/ cumulus cell-specific deletion of Clpp, throughout their reproductive lifetime. We did not found any impairment in follicle development or the number of primordial, primary, secondary, early antral, or antral follicles at 2, 6, or 9 months. Our findings are in contrast with studies that used global germline deletion of Clpp, a strategy that causes the deletion of Clpp in all cells [15,22] In one such study, Gispert et al. reported that ovaries of mice with global deletion of Clpp were smaller and had reduced layers of follicular granulosa cells with a higher number of apoptotic bodies. They suggested that this finding was consistent with ovarian failure associated with CLPP missense and splice-site mutations found in a variant of human Perrault syndrome [27], in which streak ovaries with few scattered follicles had been described [28,29]. In a more recent study, Wang et al. used the same model and confirmed that global Clpp-deletion causes female infertility associated with loss of primordial and primary follicles at 6, 9, and 12 months, and increased follicular atresia. Collectively, our findings and the findings in the two prior studies suggest that, although global Clpp-deletion causes infertility, granulosa/cumulus cell function is not dependent on CLPP expression. Therefore, the requirement for CLPP must be elsewhere. Although one could speculate that this requirement is in oocytes, this remains to be proven.
Oocytes are unable to metabolize glucose and require pyruvate for survival and maturation [30][31][32][33]. Follicular somatic cells, therefore, play an important role in the nutritional support of the oocyte. Pyruvate is produced from glucose in granulosa/cumulus cells and transported to the oocyte through gap junctions [30][31][32][33]. Not surprisingly, glycolysis is active in cumulus cells, whereas oocytes metabolize pyruvate through oxidative phosphorylation to produce energy for growth and maturation [34]. In addition to pyruvate, the cumulus cells supply the oocyte with amino acids (such as L-alanine) and cholesterol as substrates [35]. The ability of Clpp-deficient granulosa/cumulus cells to support reproduction could potentially be explained by the fact that mitochondrial metabolic activity and OXPHOS in granulosa/cumulus cells may not be central to oocyte and follicle viability.
The interactions between the oocyte and neighboring somatic cells that regulate metabolism are bidirectional. The metabolic activity of cumulus cells requires secretion of oocyte-specific paracrine factors (such as fibroblast growth factor 8B (FGF8B), bone morphogenetic protein 15 (BMP15), and growth differentiation factor 9 (GDF9)) [36]. In the current study, we found that the number of immature or mature oocytes produced by female mice with granulosa/cumulus cell-specific targeted deletion of Clpp were similar to that of WT. In addition, these oocytes did not have increased ROS or mtDNA, which occur in association with oxidative stress. These findings are in contrast to those found in mice with global deletion of Clpp, in which the GV and MII oocytes were decreased, and ROS and mtDNA significantly increased [15,22]. Collectively, these data suggest that the requirement for Clpp in reproduction may be in oocytes.
In this study, we built on the work of previous researchers in delineating the role of UPR mt and CLPP in female fertility. Our findings clearly show that female fertility is not disrupted in the absence of CLPP in granulosa/cumulus cells, and suggest that UPR mt and CLPP requirement may be in oocytes. Further studies are needed to delineate the role of UPR mt and CLPP in reproduction and to exploit these pathways for diagnostic and therapeutic purposes.

Conclusions
Despite the well-described role of granulosa/cumulus cells in oocyte metabolism, our findings demonstrate that Clpp-mediated UPR mt in these cells is not required for female fertility. Therefore, female infertility observed in models with global loss of Clpp is likely caused by oocyte-related effects, and UPR mt is not a crucial pathway in granulosa/cumulus cells.