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Impact of delipidated estrous sheep serum supplementation on in vitro maturation, cryotolerance and endoplasmic reticulum stress gene expression of sheep oocytes

  • Natalibeth Barrera ,

    Contributed equally to this work with: Natalibeth Barrera, Alejo Menchaca

    Roles Conceptualization, Data curation, Formal analysis, Methodology, Project administration, Writing – original draft (NB); (AM)

    Affiliation Instituto de Reproducción Animal Uruguay, Fundación IRAUy, Montevideo, Uruguay

  • Pedro C. dos Santos Neto ,

    Roles Investigation

    ‡ These authors also contributed equally to this work.

    Affiliation Instituto de Reproducción Animal Uruguay, Fundación IRAUy, Montevideo, Uruguay

  • Federico Cuadro ,

    Roles Investigation, Methodology

    ‡ These authors also contributed equally to this work.

    Affiliation Instituto de Reproducción Animal Uruguay, Fundación IRAUy, Montevideo, Uruguay

  • Diego Bosolasco ,

    Roles Methodology

    ‡ These authors also contributed equally to this work.

    Affiliation Instituto de Reproducción Animal Uruguay, Fundación IRAUy, Montevideo, Uruguay

  • Ana P. Mulet ,

    Roles Conceptualization, Investigation, Methodology

    ‡ These authors also contributed equally to this work.

    Affiliation Unidad de Animales Transgénicos y de Experimentación, Institut Pasteur de Montevideo, Montevideo, Uruguay

  • Martina Crispo ,

    Roles Supervision, Validation, Writing – review & editing

    ‡ These authors also contributed equally to this work.

    Affiliation Unidad de Animales Transgénicos y de Experimentación, Institut Pasteur de Montevideo, Montevideo, Uruguay

  • Alejo Menchaca

    Contributed equally to this work with: Natalibeth Barrera, Alejo Menchaca

    Roles Conceptualization, Supervision, Validation, Writing – original draft (NB); (AM)

    Affiliation Instituto de Reproducción Animal Uruguay, Fundación IRAUy, Montevideo, Uruguay

Impact of delipidated estrous sheep serum supplementation on in vitro maturation, cryotolerance and endoplasmic reticulum stress gene expression of sheep oocytes

  • Natalibeth Barrera, 
  • Pedro C. dos Santos Neto, 
  • Federico Cuadro, 
  • Diego Bosolasco, 
  • Ana P. Mulet, 
  • Martina Crispo, 
  • Alejo Menchaca


High lipid content of oocytes and embryos in domestic animals is one of the well-known factors associated with poor cryosurvival. Herein, we wanted to determine whether the use of delipidated estrous sheep serum during in vitro maturation (IVM) of ovine oocytes reduces the cytoplasmic lipid droplets content and improves embryo development and cryotolerance after vitrification. Cumulus oocytes complexes (COCs) were matured in vitro for 24 h in medium supplemented with whole or delipidated estrous sheep serum prior to vitrification. Neutral lipid present in lipid droplets of COCs, cleavage rate, embryo development rate on Day 6 and Day 8, and hatching rate on Day 8, were compared among experimental groups. Endoplasmic reticulum stress genes were evaluated in in vitro matured COCs under different lipid conditions prior to vitrification. The lipid droplets’ content (mean fluorescence intensity) of oocytes cultured with IVM media supplemented with delipidated serum was lower than COCs matured with whole serum (7.6 ± 1.7 vs. 22.8 ± 5.0 arbitrary units, respectively; P< 0.05). Despite IVM treatment, oocytes subjected to vitrification showed impaired competence compared with the non-vitrified groups (P<0.05). No significant differences in embryo production were observed in non-vitrified COCs after maturation in delipidated or whole serum (33.4±4.9 vs 31.9 ±4.2). COCs matured in delipidated serum and subjected to vitrification showed increased expression of ATF4, ATF6, GRP78, and CHOP10 genes (ER stress markers). Collectively, our results demonstrate that although supplementation of IVM medium with delipidated estrous sheep serum reduces the presence of cytoplasmic lipid droplets in oocytes after maturation, oocyte cryotolerance is not improved. Notably, the expression of genes associated with the unfolded protein response (UPR) was increased in COCs, with fewer lipid droplets subjected to vitrification, suggesting that oocyte cryopreservation is associated with ER stress and activation of adaptive responses.


Within the last decade, there have been significant advances in methods to improve oocyte cryotolerance. Difficulties associated to oocyte cryopreservation are related with inherent structural and physiological features. Particularly in domestic animals, the high intracellular lipid content of oocytes adds greater complexity to cryopreservation. Different strategies have been developed to reduce lipid droplets in oocytes including mechanical removal and pharmacological options[13]. Furthermore, it is generally accepted that in vitro embryo production (IVEP) systems are not as efficient as in vivo embryo production, mainly due to lower oocyte competence acquisition when maturation is induced under in vitro conditions [1,4,5]. Although the underlying mechanisms behind oocyte competence have not yet been fully elucidated, there is increasing evidence that oocyte metabolism and the somatic environment play crucial roles in determining oocyte growth and developmental competence [6]. Lipid metabolism provides a good source of energy during oocyte maturation upon demand. For example, fatty acids stored within lipid droplets provide adenosine triphosphate (ATP) molecules through β-oxidation, largely serving as an energy source during oocyte maturation and early embryo development [7]. Therefore, components within the culture medium supplied to the cumulus-oocytes complexes (COCs) during in vitro maturation have the potential of affecting oocyte competence [8].

Studies show that when oocytes are matured in vitro, energy substrates as fatty acids provided through culture media can lead to increased intracellular lipid droplet (LD) accumulation [911] and alter oocyte metabolism, thereby affecting their quality. A recent report showed that exposure of mice COCs to high lipid content follicular fluid was associated with endoplasmic reticulum (ER) stress induction and led to a decrease in oocyte competence [12]. Moreover, increased accumulation of lipids in oocytes was correlated with reduced cryopreservation resistance [13]. It is well established that in sheep and other species, in vitro generated embryos exhibit reduced cryotolerance [14,15]. The process of cryopreservation leads to multiple changes, including structural modifications and alterations in gene expression patterns [16]. For example, increased expression of genes associated with ER stress has been reported after oocyte cryopreservation. In domestic animals, the high lipid content in oocytes may pose challenges for cryopreservation [10]. Specifically, bovine, ovine, and porcine oocytes are highly susceptible to cryoinjuries, with the majority of studies reporting a blastocyst rate of 0 to 20% [2,1720] after oocyte vitrification. Additional studies have suggested that tolerance of oocytes to chilling injuries can be increased when cytoplasmic lipid content is reduced, thereby improving cleavage and blastocyst rates[10,21]. Interestingly, the introduction of controlled stress during in vitro culture led to improved cleavage and blastocyst rates and suggests that oocytes perform better under specific types of stress signals [22,23]. Induction of pathways related to ER stress have been reported in oocytes subjected to vitrification [12]. ER stress is a mechanism associated with excess intracellular lipid accumulation in COCs [24]

The addition of animal serum to IVEP medium is a standard practice and helps promote oocyte maturation and subsequent embryo development [25]. During culture of ovine oocytes, estrous serum is routinely used to supplement the maturation medium, since it is known that it contains a range of beneficial components, including hormones, growth factors, amino acids, binding proteins. Conversely, estrous serum also provides a significant source of lipids. Therefore, the reduction of lipid content is necessary to improve in vitro embryo cryosurvival and blastocyst rates in IVP systems. One strategy to reduce lipid exposure involves incorporation of serum-free media during IVM. [26]. Nutrient restriction in the maturation medium promotes the use of the oocyte’s own endogenous reserves, thereby reducing the amount of intracellular lipids [10]. However, oocyte competence is impaired under serum-free culture conditions compared to undefined media in which serum has been added [21]. Alternatively, restriction of lipid content in the serum may be a more optimal strategy to reduce lipid droplets in the oocyte and may improve oocyte cryosurvival.

The objective of this study was to determine whether supplementation of IVM medium with delipidated estrous sheep serum affects the amount of cytoplasmic LD in in vitro matured sheep oocytes. Furthermore, we investigate whether intracellular lipid content variations in oocytes is associated with oocyte developmental competencies, cryotolerance, embryo production, and ER stress.

Materials and methods

Experimental design

Three experiments were conducted by using a total of 2,986 COCs at Fundación IRAUy and Transgenic and Experimental Animal Unit of Institut Pasteur of Montevideo, Uruguay. The experimental design is shown in Fig 1. Unless stated otherwise, all media and chemicals were purchased from Sigma (St. Louis, MO, USA).

Fig 1. Experimental design.

Schematic representation for determination of the effect of control whole estrous sheep serum vs. delipidated serum used during in vitro maturation of cumulus oocytes complexes (COCs) on oocyte lipid content and: embryo development (Experiment 1), cryotolerance after vitrification (Experiment 2), and expression of endoplasmic reticulum (ER) stress genes (Experiment 3).

Experiment 1.

Experiment 1 was conducted to evaluate the effect of the lipid content (based on the concentrations of Triglycerides, total Cholesterol, and non-esterified fatty acid (NEFAs)) of IVM medium supplemented with estrous sheep serum on: (a) neutral lipid stored in LD of in vitro matured oocytes, and (b) oocyte developmental competence. A total of 866 COCs were collected from slaughterhouse ovaries and subjected to IVM in a supplemented medium with whole estrous sheep serum (Control whole serum group, n = 452) or delipidated estrous sheep serum (Delipidated serum group, n = 414). Neutral lipid present in LD of partially denuded COCs, cleavage rate, development rate on Day 6 and Day 8, and hatching rate on Day 8, were compared between the two experimental groups (Fig 1). Seven replicates of this experiment were performed for each treatment group.

Experiment 2.

Experiment 2 was conducted in order to further investigate the effect of vitrification on the survival rates of oocytes previously matured under different lipid content conditions. Viable immature COCs (1280) were randomly assigned to two experimental groups consisting of IVM medium supplemented with control or delipidated estrous serum sheep.

After IVM, COCs were submitted to IVF and IVC (Control whole serum group, n = 344; Delipidated serum group, n = 357); or were vitrified using the Cryotop method (Control whole serum + vitrification group, n = 288; Delipidated serum + vitrification group, n = 291) before IVF and IVC. Oocyte lipid content was assessed by LD staining before and after vitrification/warming, and cleavage rate, development rate on Day 6 and Day 8, and hatching rate on Day 8 were compared among groups (Fig 1). A total of thirteen replicates of this experiment were performed for each treatment group.

Experiment 3.

Experiment 3 was performed in order to determine whether in vitro matured COCs under different lipid conditions followed by vitrification expresses different levels of ER stress markers. A total of 840 COCs were used to determine ER stress gene expression (ATF4, ATF6, GRP78, and CHOP10) by real time PCR in five experimental groups (Immature, Control whole serum group, Delipidated serum group, Control whole serum + Vitrification group, and Delipidated serum + Vitrification group). Seven replicates of this experiment were performed using 30 COCs per replicate for each treatment group.

Estrous sheep serum source, lipid removal and lipid determinations

For serum preparation, blood samples were collected from 15 ewes in estrus previously treated with a hormonal protocol for estrous synchronization [27]. The procedure was approved by the Internal Animal Care Committee of Fundación IRAUy that is certified by the National Council of Animal Care of Uruguay. The blood was allowed to clot at room temperature during one hour and then centrifuged at 1500 g for 20 min at 4°C. Serum was collected, pooled and heat inactivated at 56°C for 30 min. Lipid removal from serum was performed by using Cleanascite™ (Biotech Support Group, NJ, USA) according to the instructions provided by the manufacturer. In brief, 1 ml of CleanasciteTM was added to 4 ml of serum (1:4 v/v), samples were gently mixed for 10 min at room temperature, lipid’s agglomeration was improved by incubation at 4°C for 1 h, samples were centrifuged at 1000 g for 15 min at 4°C, and then, the supernatants were pooled and filtered with a 0.22 μm filter.

Aliquots from the whole and the delipidated estrous sheep serum (five samples of each group, same batch) were analyzed for Triglycerides, total Cholesterol, and NEFAs by using the commercial kits TG color GPO/PAP AA, Colestat enzimático (Wiener Lab, Rosario, Argentina), and NEFA-HR (2) (Wako Chemicals USA, Inc., Richmond, VA, USA), respectively. All enzymatic colorimetric assays were performed according to the manufacturer's instructions. Measurements were obtained with a biochemical analyzer (Vitalab Selectra-2 Merck, Darmstadt, Germany). The lipid removal efficiency was 54.4% for total cholesterol, 21.2% for triglycerides and 30.6% for NEFAs. For this reason, delipidated serum was in fact partially delipidated. Data presented on Table 1 show the mean values and inter-assay coefficient of variation (CV) for each metabolite.

Table 1. Lipid content of whole and delipidated estrous sheep serum (prior to be added to maturation medium).

Oocyte collection

Sheep ovaries were collected from the slaughterhouse and transported to the laboratory within 1 h in saline solution with 50 IU/ml of Penicillin and 50 μg/ml of Streptomycin at 35–37°C. The COCs were aspirated from antral follicles (2 to 6 mm) using a 21 gauge needle and a 5 ml syringe containing 0.5 ml of collection medium containing HEPES-buffered Tissue Cultured Media 199 (TCM 199) supplemented with 5 IU/ml of Heparin, 50 IU/ml of Penicillin, 50 μg/ml of Streptomycin, and 0.3% fatty acid-free Bovine Serum Albumin (BSA). Only COCs surrounded with three or more layers of granulosa cells and with homogeneous cytoplasm were selected for maturation purposes.

In vitro maturation (IVM)

Embryo production was performed according to the standard operative procedures of our laboratory using the method described by Menchaca et al. (2016) [3]. Briefly, selected COCs were washed three times in a washing medium containing TCM 199 + HEPES supplemented with 50 IU/ml of Penicillin, 50 μg/ml of Streptomycin, and 0.3% fatty acid-free BSA. Groups of 25–30 COCs were placed into 100 μl droplets of maturation medium under mineral oil at 39°C in a humidified atmosphere of 5% CO2 in air for 22–24 hours. For IVM, the medium was supplemented with either 10% estrous sheep serum (whole or delipidated), 10 μg/ml FSH, 10 μg/ml LH, 100 μM Cysteamine, 50 IU/ml Penicillin, and 50 μg/ml of Streptomycin.

In vitro fertilization (IVF)

COCs were removed from maturation drops and washed three times in IVF medium consisting of synthetic oviduct fluid (SOF), 2% estrous sheep serum, 10 μg/ml Heparin, and 10 μg/ml Hypotaurine. For fertilization (Day 0), frozen semen from a single ram previously frozen and tested in our lab for IVF was used. Motile spermatozoa were obtained by swim-up method [28] with slight modifications. COCs were placed into 100 μl of IVF medium, covered with mineral oil and inseminated with 1 x 106 spermatozoa/drop. In vitro fertilization was carried out at 39°C in 5% CO2 with humidified atmosphere for 22 hours.

In vitro culture (IVC)

Presumptive zygotes were denuded by gentle pipetting and were washed three times in drops of culture medium (SOFaaBSA bicarbonate buffered) containing 5% (v/v) Basal Medium Eagle (BME)-essential amino acids, 2.5% (v/v) Minimum Essential Medium (MEM)-nonessential amino acids, and 4 mg/ml of BSA. Embryonic development took place in a humidified atmosphere of 5% CO2, 5% O2, 90% N2 at 39°C and the medium was renewed on Day 3 and Day 6 [3]. The percentage of cleaved embryos on Day 2 was recorded (2–8 cell embryos/total oocytes). Development rate on Day 6 (number of morulae and blastocysts) and on Day 8 (number of blastocysts) were expressed on the basis of number of presumptive zygotes at the onset of IVC. Percentage of hatching blastocysts on Day 8 (hatching rate) was determined on the basis of the total number of blastocysts on the same day.

Oocyte-vitrification and warming procedure

For the experimental groups submitted to vitrification (Experiment 2 and 3), cryopreservation was performed using the Cryotop method first described by Kuwayama et al. (2005)[29]. This method was performed using methodology and media previously reported by our group [14,15]. Following IVM, COCs were mechanically denuded by exposure to 0.1 mg/ml of hyaluronidase at 37°C for 30 seconds through pipetting using a 200 μl pipette tip. Partially denuded COCs were washed three times in a washing medium. Oocytes were first equilibrated at room temperature for 15 min in TCM 199 medium supplemented with 20% Fetal Bovine Serum (FBS), Basic Solution (BS) containing 7.5% (v/v) Ethylene Glycol (EG) and 7.5% (v/v) Dimethyl sulfoxide (DMSO), referred to as Equilibrium Solution (ES). Four oocytes were equilibrated at the same time. They were checked for recovery of the initial shape before the vitrification step. Following equilibration, oocytes were placed in a Vitrification Solution (VS) containing BS supplemented with 15% (v/v) EG, 15% (v/v) DMSO, and 0.5 M Sucrose. After 90 s in this solution, oocytes were placed on the Cryotop device (Kitazato Biopharma, Fujinomiya, Japan) in a minimum volume (e.g. <0.1 μl) and immediately submerged in liquid nitrogen. No more than four oocytes were loaded per Cryotop device. For warming, the Cryotop was removed from the liquid nitrogen and instantly placed in a solution containing BS plus 1.0 M sucrose at 37°C. After 1 minute, the oocytes were transferred to a solution consisting of BS plus 0.5 M Sucrose for 3 minutes at RT. Finally, a 5minute wash followed by a 1 minute wash was performed with BS at RT. The oocytes were then placed in IVM medium at 39°C with 5% CO2 humidified atmosphere for 2 h before IVF to allow microtubule repolymerization [30].

Lipid droplet staining

In Experiment 1 and 2, BODIPY 493/503 dye (Invitrogen, Carlsbad, CA, USA), which stains intracellular neutral lipids, was used to localize LD. The neutral lipid dye BODIPY493/503 has been used to demonstrate differences in oocyte lipid content on a variety of species including mice, cows, sheep, pigs, and humans [8]. The methodology previously described for bovine oocytes was followed with few modifications [31]. COCs were partially denuded by exposure to 0.1 mg/ml of Hyaluronidase at 37°C for 30 s through pipetting using a 200 μl tip. Oocytes were washed three times in serum-free Polyvinylpyrrolidone in Phosphate-buffered saline (PBS-PVP; 0.2% w/v). COCs were fixed in 4% paraformaldehyde at 37°C for 1 h and washed twice in PBS-PVP. Oocytes were allowed to permeate for 30 min in PBS containing 0.1% (w/v) Saponin, 0.1 M Glycine (PBS-S). The DNA was stained with 10 μg/ml of TO-PRO-3 (Molecular Probes, Eugene, OR) for 20 min and subsequently washed in PBS-S. Next, LDs were stained with BODIPY 493/503 in PBS (20μg/ml) for 1 h in the dark, and oocytes were washed three times in PBS-PVP. Oocytes were then placed on a glass slide covered with 80% glycerol (in PBS) and sealed with a microscope slide.

Lipid droplet determinations

Lipid droplet content was determined in Experiment 1 and 2. Images of oocytes were obtained using a confocal laser scanning microscope (Model LSM 800; Zeiss, Thornwood, NY, USA) attached to an inverted microscope (Model AxioObserver Z1; Zeiss, Thornwood, NY, USA) at 25X magnification. BODIPY 493/503 and TO-PRO-3 were subsequently excited with diode 488 nm lasers and diode 640nm laser. Emitted light was selected with emission detection wavelengths ranges for BODIPY 410–617 nm and for TOPRO-3 645–700 nm. Images were reconstructed using ZEN 2.1 software (Blue edition). From the in vitro matured groups only metaphase II stage oocytes were analyzed for lipid determination. Using ImageJ v.1.44g software, sum slices Z-projection was generated to a stack of images, same number of slices was used for each projection created (from 1 to 30 endpoint slice). The BODIPY fluorescence (arbitrary units of fluorescence) in the oocyte was determined after selection of the area covering entire ooplasm and the background region of each partially denuded oocyte [4]. After background correction Integrated density (Int Den) was calculated using Image J v.144- software. Finally IntDen mean ± SEM for each experimental group was determined.

RNA isolation and reverse transcription

For RNA isolation, 30–35 COCs from each group of Experiment 3 (Immature, Control whole serum group, Delipidated serum group, Control whole serum + vitrification group, and Delipidated serum + vitrification group) were denuded, washed in PBS, and placed into a 1.5 ml microcentrifuge tube. The tubes were immediately submerged in liquid nitrogen and stored at -80°C until RNA extraction. Total RNA was isolated using the RNeasy Plus Micro Kit (QIAGEN, Hilden, Germany) according to the manufacturer’s instructions. The extracted RNA concentration and purity was estimated using a ND-1000 spectrophotometer (NanoDrop Technologies, Delaware USA). Sample purity was assessed using the A260/ A280nm ratio with expected values between 1.8 and 2.0. Reverse transcription was carried out with 50ng of total RNA using SuperScript®III First-Strand Synthesis System for RT-PCR (Invitrogen) and a random hexamer primer in a final reaction volume of 10 μl according to the manufacturer’s instructions. The cDNA synthesis reactions were carried out at 25°C for 5 min for annealing, 50°C for 50 min for extension, followed by enzyme heat inactivation at 85°C for 5 min.

Real-time polymerase chain reaction

For Experiment 3, gene expression was assessed by quantitative real-time PCR (qPCR). Oligonucleotide primers were designed for GRP78, CHOP10, ATF4, and ATF6 using NCBI Primer Blast. Genes were selected as markers of activation of UPR, signaling branch activated under ER stress[32]. The primer sequences for PPIA and TUBB were taken from a published report where those genes were found most stable for normalization when random hexamers were used for cDNA priming in ovine oocytes [33]. Expected fragment size and GenBank accession numbers are listed on Table 2. All primers were synthesized by IDT (Integrated DNA Technologies, Coralville, IA, USA). The PCR mix in each include 5 μl of Power SYBR Green PCR Mix (2X) (Applied Biosystems, UK), 2μl of nuclease-free water, 1 μl of each forward and reverse primer pair (10 μM), and 1 μl of cDNA in a final volume of 10 μl. The PCR was carried out on an Eco™ Real-time PCR System (Illumina, San Diego, USA). The program used for the amplification of the genes consisted of an enzyme activation step of 10 min at 95°C followed by 45 cycles of PCR of a 15s denaturation at 95 ˚C, 60 s annealing/extension at 60 ˚C and a dissociation step consisting of 95°C for 15 s, 60°C for 15 s and finally 95°C for 15 s. At the end of the PCR reactions, melt curve analyses were performed for all genes to confirm the integrity of PCR products and specificity by the presence of a single peak. All samples were run in duplicate and mean value was used for calculations. Standard curves were created for each gene using a 3-fold dilution of cDNA and used to calculate individual real time PCR efficiencies (E) according to the formula %E = (10−1/slope– 1) × 100 [34]. The data generated by Eco Real-Time PCR System Software v5.0 (IIlumina, CA, USA) were transferred to Microsoft Excel for analysis.

All target gene transcriptions were expressed as an n-fold difference relative to the calibrator (Control serum group). Different amplification efficiencies for individual genes were considered [35]. The geometrical mean of two internal reference genes (TUBB and PPIA) was used to correct the raw values for the genes of interest.

Statistical analysis

Statistical analysis was performed using Infostat software (Cordoba, Argentina). The criterion of data normality was evaluated by the Shapiro-Wilk test and percentage data was subjected to arcsine transformation and expressed as Mean ± SEM. Significance differences in Experiment 1 were tested by a two-way analysis of variance (ANOVA) followed by Tukey’s test when variables were normally distributed. A non-parametric Kruskal-Wallis test was conducted for comparison of variables that did not follow normal distribution. For Experiment 2 and 3, in which 2x2 factorial design was performed, mixed models were used with fixed effect for cryopreservation (vitrification or not), serum (whole or delipidated) and its interaction, and the replicate as random effect (13 replicates for Experiment 2 and seven replicates for Experiment 3). Values of p less than 0.05 were considered statistically significant.


Experiment 1

The lipid content of immature oocytes measured soon after follicular aspiration was 9.9 ± 2.9 (expressed as the mean fluorescence intensity). After maturation, the lipid droplet content in oocytes cultured in medium containing whole estrous serum increased more than twofold compared to immature oocytes (22.8 ± 5.0; P< 0.05). In contrast, oocytes that were matured in medium containing delipidated estrous serum showed a significantly lower content of lipid droplets (7.6 ± 1.7; P< 0.05), which was similar to the levels measured in immature oocytes (P = NS). Fig 2 shows the results of lipid droplet localization and quantification of immature, control whole, and delipidated in vitro matured COCs after BODIPY 493/503 staining. Differences found in the oocyte neutral lipid content did not influence subsequent embryo development (Table 3). No significant differences (P = NS) were observed in the cleavage rate, developmental rates on Day 6 and Day 8, or hatching rate between groups.

Fig 2. Lipid quantification of partially denuded COCs in vitro matured with control whole serum or delipidated serum (Experiment 1).

a) Nuclei of cells were stained with ToPro-3 (red) and merged with bright field image (BF). Neutral lipid staining with BODIPY 493/503 (green) show an increase in lipid droplets of oocytes after exposure to IVM media supplemented with control whole serum. b) Comparison of the lipid content of immature (Immature, n = 23) and COCs in vitro matured in a medium supplemented with control whole (n = 24) or delipidated (n = 24) estrous sheep serum. Values are expressed as average of BODIPY fluorescence intensity in the ooplasma per area ± SEM. a vs b indicates significant differences (P<0.05).

Table 3. In vitro ovine embryo development after maturation of COCs supplemented with control whole or delipidated estrous sheep serum (Experiment 1, seven replicates).

Experiment 2

Oocyte lipid content assessed by LD staining before and after vitrification are shown in Fig 3. Lipid droplets in oocytes exhibited reduced fluorescence after vitrification when matured in vitro with either medium supplemented with control whole serum or delipidated serum. Despite IVM treatment, oocytes subjected to vitrification exhibited reduced competence after in vitro fertilization and culture, with lower cleavage rate, embryo development rates on Day 6 and Day 8, and hatching rate when compared with the non-vitrified oocytes (P<0.05). No significant differences (P = NS) were found among non-vitrified groups, which is in agreement with the results obtained in Experiment 1 (serum effect: whole vs. delipidated). No interaction between vitrification and the type of serum (whole or delipidated) were found for cleavage, embryo development, and hatching rates (P = NS) (Table 4).

Fig 3. Effect of vitrification on lipid droplet content of partially denuded COCs after IVM under different lipid content conditions (Experiment 2).

a) Nuclei of cells were stained with ToPro-3 (red) and merged with bright field image (BF). Neutral Lipid staining with BODIPY 493/503 (green) shows a decrease in lipid droplets of oocytes after vitrification. b) Comparison of the lipid content of immature (Immature, n = 12) versus IVM COCs in a medium supplemented with control whole (n = 16) or delipidated estrous sheep serum (n = 19) before or after vitrification (control whole serum+ vitrification group, n = 12; Delipidated serum+ vitrification n = 11). Values are expressed as average of BODIPY fluorescence intensity in the ooplasma per area ± SEM. Different superscripts indicate significant differences (P< 0.05).

Table 4. In vitro embryo development of ovine oocytes subjected to IVM under different lipid content conditions induced by supplementation of whole or delipidated serum followed by vitrification (Experiment 2).

Experiment 3

The expression of ER stress genes was affected by the serum type used during IVM of COCs as well as by the vitrification/warming process, with interaction between both main effects (P<0.05). The expression of classic ER stress markers (ATF4, ATF6, GRP78, and CHOP10) examined in COCs exposed to IVM media supplemented with control whole or delipidated serum and either submitted to vitrification or not is shown in Fig 4. The COCs matured in delipidated serum and subjected to vitrification exhibited increased expression of ATF4 (4.4 fold), ATF6 (4.0 fold), GRP78 (3.6 fold), and CHOP10 (2.5 fold) compared with COCs matured in IVM media supplemented with control whole serum (calibrator sample). No significant differences (P = NS) were found in the expression levels of those ER stress markers in COCs matured in control whole serum and subject to vitrification (control whole serum + vitrification group). COCs matured in delipidated serum (non-vitrified group) exhibited similar expression levels of the four ER stress markers respect to the control whole serum group. These results demonstrate that vitrification induces ER stress in COCs when they are previously matured in vitro in medium deprived of lipids.

Fig 4. Expression of endoplasmic reticulum (ER) stress genes induced in cumulus oocytes complexes (COCs) submitted to in vitro maturation (IVM) in whole or delipidated serum with subsequent vitrification.

Total RNA was extracted from denuded COCs, and expression of ER stress marker genes (ATF4, GRP7878, ATF6 and CHOP10) was determined by qPCR. Gene expression of 5 experimental groups, interaction was found when COCs were matured in delipidated serum and subsequently vitrified. Within the same gene, different letters indicates significant differences (P< 0.05). Mean ± SEM is expressed as fold change compared with calibrator sample (control whole serum).


The current study demonstrates that COCs matured in vitro in medium supplemented with delipidated estrous sheep serum contain fewer cytoplasmic lipid droplets than those matured in medium supplemented with whole estrous serum. However, reduced numbers of cytoplasmic lipid droplets did not improve oocyte competence and embryo production in fresh and vitrified oocytes. While the vitrification process impairs oocyte developmental competence, the serum type (delipidated or whole) used during IVM did not appear to have any adverse effects. Notably, mRNA expression levels of ER stress genes increased significantly after vitrification of oocytes but only when maturation was performed with medium supplemented with delipidated serum.

We found that the standard method used for in vitro maturation of COCs with a medium supplemented with whole estrous sheep serum increased oocyte neutral lipid content in comparison with immature oocytes. This increase was prevented by serum delipidation, since oocytes subjected to IVM medium with partially delipidated serum had less lipid droplets than COCs matured in control whole serum. Lipid droplets are intracellular sites of neutral lipid storage, which have been shown to play an important role in the metabolism of lipids and cellular energy homeostasis [36]. During in vitro maturation, serum lipids are incorporated into the oocyte cytoplasm [37], with the presence of lipids in culture media causing an increase in the number of lipid droplets in the produced embryos [38]. Although lipid droplets play a pivotal role during oocyte maturation, since oxidative phosphorylation is the main pathway to produce ATP [7], high accumulation of lipid droplets content has been correlated with poorer cryosurvival rates and reduced development competence of oocytes.[39]. In this study, we demonstrate that in vitro maturation of COCs in medium containing whole estrous serum increase lipid accumulation in matured oocytes, a finding that could be important for oocyte cryotolerance and embryo development.

Studies show that high lipid content in IVM oocytes correlates with reduced cryotolerance, therefore different strategies have been used to reduce numbers of lipid droplets in oocytes. One way to regulate the lipid content is the use of serum free media, which contains restricted nutrients, during IVM [1]. However, efforts to reduce lipid content in the oocytes and embryos, have been met with limited success and resulted in lower oocyte competence [40], [41]. Unlike other approaches, the protocol described herein for delipidation of estrous sheep serum was effective in decreasing levels of Triglycerides, total Cholesterol, and NEFAs. To our knowledge this is the first study to use the Cleanascite HC method to generate estrous sheep serum yielding significantly reduced lipid levels. Subsequent use of the partially delipidated serum as supplemented in IVM media resulted in effective reduction of oocyte lipid content. The advantage of this method over other traditional methods (i.e. chloroform) includes increased feasibility and reduced toxicity and biosafety concerns [42]. Similar results have been found when oocyte delipidation is achieved by stimulating lipid metabolism (i.e. L-Carnitine) [43]. The approach of encouraging embryos and oocytes to deplete intracellular lipids to increase cryosurvival rates has been shown to be a more benign alternative to mechanical delipidation and safer for oocytes and embryos [1]. Furthermore, our protocol enables simultaneous delipidation of large numbers of oocytes and does not require micromanipulation, thereby increasing efficiency and improving viability of oocytes.

The current study shows that oocyte competence was affected by cryopreservation independently of the lipid environment in which the COCs were matured. Cryopreservation protocols are not well established for oocytes, especially in domestic animals due to their high lipid content.[44]. Ultra-rapid vitrification methods have made it possible to overcome some challenges associated with oocyte cryopreservation. Specifically, the use of Cryotop with minimum volume of vitrification (<0.1 μl) and high cooling rates (22.800°C min-1) has allowed human oocytes to obtain post-warming survival rates of >90% and blastocyst rates of roughly 50% [29]. Compared to human oocytes, oocytes from some species of domestic animals have high lipid content which increases their sensitivity to cooling processes and exacerbates outcomes after IVM [1]. Overall, species that have higher lipid content in their ooplasma have lower survival rates following cryopreservation [39]. As expected, we found that vitrified oocytes that had been in IVM medium containing whole serum showed reduced cleavage rates and embryo development compared to fresh control oocytes that were not subjected to vitrification. Interestingly, although incorporation of partially delipidated serum in the IVM medium resulted in lower lipid content in the matured oocytes, it did not improve outcomes after vitrification including cleavage rates and embryo development rates in comparison to IVM oocytes with control whole serum medium. Collectively, our results show that reducing lipid content during the COC maturation process prior to cryopreservation is not sufficient to improve oocyte competences following, suggesting that lipid content is one factor amongst many variables/factors that can lead to reduced tolerance to cryopreservation. Some studies attribute the lower cryotolerance of in vitro produced embryos to an imbalance of oxidation-reduction metabolism leading to greater accumulation of reactive oxygen species in the culture medium and reduced survival rates of embryos [45]. Our current results suggest that a negative correlation exists between lipid content and oocyte cryotolerance. It is well known that embryos derived from live animals have fewer lipid droplets compared to IVP embryos [46]. This difference in lipid neutral content may explain, in part, the differences in cryotolerance between in vivo versus in vitro embryos [1]. Some studies have reported similar differences in bovine and porcine oocytes matured in vivo vs. in vitro [47,48]. These observations support the idea that if IVM oocytes in delipidated systems could resemble in vivo matured oocytes in terms of lipid droplets content and that cryotolerance could be improved. However, despite the lower lipid droplet content found in those COCs subjected to IVM with partially delipidated serum, no differences in oocyte competence were found. It is likely that either the variations observed are insufficient to alter oocytes’ cryotolerance to vitrification, or that a reduction of lipid droplets using our experimental conditions is not a key factor to overcome damages associated with vitrification.

Finally, we demonstrate that vitrification induces greater expression of ER stress genes in COCs matured in a medium with reduced lipid content. The ER folding capacity can be disturbed by biological stimuli, resulting in an accumulation of misfolded and unfolded proteins in the ER lumen and ER stress [32]. ER stress triggers a homeostasis response, referred to as the unfolded protein response (UPR) [49], which involves the activation of ER transmembrane signaling molecules (PERK, IRE1 and ATF6). Activation of these three master regulators of UPR influence the transcription of several genes involved in UPR. IRE1α regulates the splicing of XBP1 promoting components of ER-associated protein degradation (ERAD) as Bip/GRP78. Activation of PERK favor translation of ATF4, which regulates genes involved in protein folding, degradation, and apoptosis, including CHOP. In this study, we have selected downstream regulators ATF4, CHOP, and GRP78 as representative genes of the PERK/IRE1 pathway to determine UPR activation [32]. Differences in the expression levels of UPR genes has been related with lipid droplet content in mice and expression of GRP78 is greater when oocytes are matured in vivo [50]. Lipid peroxidation has also been linked to induction of UPR in endothelial cells [51] and augmentation in the expression levels of XBP1 has been reported in vitrification-warmed mouse oocytes [12]. Our data revealed that GRP78 is expressed highly in immature sheep oocytes compared to COCs that were matured in vitro. No significant differences were found in the expression levels of ATF4, ATF6, GRP78, and CHOP10 in COCs that were matured in vitro—either in whole serum or in delipidated serum. Attenuation in the expression levels of GRP78 in in vitro matured COCs could be a consequence of FSH supplementation in the IVM media as reported previously for mice [52]. COCs that were matured in vitro in IVM media supplemented with delipidated serum and vitrification upregulated the expression of ATF4, ATF6, CHOP10, and GRP78. It has been previously suggested that lipid droplets may serve as a site of storage to sequester unfolded or excessive proteins, thereby alleviating ER stress [53]. Therefore, the amount of lipid droplets in COCs matured in whole serum and vitrified reduced their sensitivity to ER stress induction post-warming. Another possible explanation for our results, is that oocyte competence is regulated by adaptive machineries governed by ER stress. Various genes associated with ER stress were found in oocytes and preimplantation embryos of mice and pigs, as a normal part of preimplantation embryos adaptive machineries [54,55]. However, some studies oppose the notion that the UPR response promotes oocyte competence. The inhibition of the UPR response by different inhibitors (TUDCA or Salubrinal) was shown to enhance maturation of pig and mouse oocytes by preventing ER stress mediated apoptosis in vitro [24,55], suggesting that ER stress may negatively impact oocyte developmental competence. To our knowledge, this is the first time that expression of the ATF4, ATF6, CHOP10, and GRP78 genes has been evaluated in ovine oocytes. We demonstrate that vitrification can cause activation of UPR when oocytes are diminished in lipid droplets content.

In conclusion, this study demonstrates that partial delipidation of estrous sheep serum used for supplementation of IVM medium reduces the neutral lipid content and the presence of cytoplasmic lipid droplet in oocytes. However, the culture of oocytes in delipidated serum did not result in improved cryotolerance when in vitro matured oocytes were subjected to vitrification. COCs with reduced amounts of lipid droplets subjected to vitrification were observed to have higher expression of UPR genes. Overall, this study provides a feasible method to reduce lipid droplets in oocytes that are in vitro matured, and suggests the need of a revision of the idea that oocyte cryotolerance may be improved by lipid content depletion.


The authors thank Victoria de Brun and Marcela Díaz for their technical support. The authors would also like to thank Dr. Stephan du Plessis and Dr. Sumantha Bhatt for their help in preparing this manuscript. This study received financial support of Union Agriculture Group (UAG) and Agencia Nacional de Investigación e Innovación (ANII; POSNAC201311217). AM and MC are fellows of Sistema Nacional de Investigadores (SNI) and PEDECIBA.


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