Cryopreservation is known for its marked deleterious effects on embryonic health. Bovine compact morulae were vitrified or slow-frozen, and post-warm morulae were cultured to the expanded blastocyst stage. Blastocysts developed from vitrified and slow-frozen morulae were subjected to microarray analysis and compared with blastocysts developed from unfrozen control morulae for differential gene expression. Morula to blastocyst conversion rate was higher (P < 0.05) in control (72%) and vitrified (77%) than in slow-frozen (34%) morulae. Total 20 genes were upregulated and 44 genes were downregulated in blastocysts developed from vitrified morulae (fold change ≥ ± 2, P < 0.05) in comparison with blastocysts developed from control morulae. In blastocysts developed from slow-frozen morulae, 102 genes were upregulated and 63 genes were downregulated (fold change ≥ ± 1.5, P < 0.05). Blastocysts developed from vitrified morulae exhibited significant changes in gene expression mainly involving embryo implantation (PTGS2, CALB1), lipid peroxidation and reactive oxygen species generation (HSD3B1, AKR1B1, APOA1) and cell differentiation (KRT19, CLDN23). However, blastocysts developed from slow-frozen morulae showed changes in the expression of genes related to cell signaling (SPP1), cell structure and differentiation (DCLK2, JAM2 and VIM), and lipid metabolism (PLA2R1 and SMPD3). In silico comparison between blastocysts developed form vitrified and slow-frozen morulae revealed similar changes in gene expression as between blastocysts developed from vitrified and control morulae. In conclusion, blastocysts developed form vitrified morulae demonstrated better post-warming survival than blastocysts developed from slow-frozen morulae but their gene expression related to lipid metabolism, steroidogenesis, cell differentiation and placentation changed significantly (≥ 2 fold). Slow freezing method killed more morulae than vitrification but those which survived up to blastocyst stage did not express ≥ 2 fold change in their gene expression as compared with blastocysts from control morulae.
Citation: Gupta A, Singh J, Dufort I, Robert C, Dias FCF, Anzar M (2017) Transcriptomic difference in bovine blastocysts following vitrification and slow freezing at morula stage. PLoS ONE 12(11): e0187268. https://doi.org/10.1371/journal.pone.0187268
Editor: Christine Wrenzycki, Justus Liebig Universitat Giessen, GERMANY
Received: March 6, 2017; Accepted: October 17, 2017; Published: November 2, 2017
Copyright: © 2017 Gupta et al. This is an open access article distributed under the terms of the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original author and source are credited.
Data Availability: Microarray data have been deposited in NCBI’s Gene Expression Omnibus accessible through GEO SuperSeries accession number GSE95382.
Funding: This study was funded by Natural Sciences and Engineering Research Council of Canada (NSERC), and Agriculture and Agri-food Canada to MA. The funders had no role in study design, data collection and analysis, decision to publish, or preparation of the manuscript.
Competing interests: The authors have declared that no competing interests exist.
Cryopreservation of bovine embryos is widely used for trade of genetically superior animals and conservation of genetic diversity. Bovine embryos are commonly frozen with either slow freezing or vitrification method . Both techniques differ in concentration of cryoprotectants and cooling rates . Slow freezing is currently a gold standard method for cryopreservation of bovine embryos. However, it damages mammalian embryos due to intracellular ice formation and toxic effect of the permeating cryoprotectants (~1–2 M). The intracellular ice formation is dependent on cooling rate and surface area/volume of cells . Cryopreservation leaves deleterious effects on oocytes and embryos at developmental, morphological and biochemical levels [4,5]. Over the years, the attempts have been made to minimize damage to morulae/blastocysts caused by cryoprotectant-associated toxicity and intracellular ice formation during cryopreservation [1,6]. Vitrification includes the use of highly viscous solution of cryoprotectants (~7–8 M) to achieve a glass-like state with ultra-rapid cooling rates (>5000°C/min) avoiding the intracellular ice formation [7,8]. Following vitrification, bovine embryos undergo extra- and intra-cellular glass-like state instead of ice crystal formation [9,10]. The vitrified bovine embryos have improved or equivalent survival , blastocyst hatching and pregnancy rates [10,12] as compared with slow-frozen embryos. It is anticipated that vitrification will gradually replace slow freezing for embryo cryopreservation . Vitrification may be a suitable cryopreservation method for in vitro produced embryos which do not survive very well following slow freezing method, compared to in vivo produced embryos . Both, vitrification and slow freezing cause intracellular/extracellular fractures in freezing planes, acute shrinkage in cell volume and organelle damage in mammalian embryos [1,14,15].
The gene expression in bovine oocytes at different development stages and in pre-implantation embryos has been studied [16–18]. The gene expression in oocytes, granulosa cells and pre-implantation embryos changed during extreme stress conditions such as heat shock  and hormonal imbalance [20–22]. Vitrification of in vitro produced bovine blastocysts up-regulated genes involved in stress response . Vitrification of mouse embryos exhibited differential apoptotic and DNA methylation gene expression . TUNEL-based assays on embryos showed low DNA-integrity indices after slow freezing and vitrification in mouse, human and bovine species [25,26]. Vitrification skewed inner cell mass to trophoblast ratio and generated reactive oxygen species in mouse embryos . On contrary, slow-frozen bovine embryos exhibited higher pro-apoptotic gene expression compared to vitrified embryos . These studies have examined individual genes in isolation. In order to fully understand the effects of vitrification and slow freezing on cellular and molecular pathways, there is a need to compare the global gene expression in in vitro produced bovine embryos. Such cryopreservation-related subtle but cumulative changes may influence the embryo development at a morphological level and may have long-term effects. The objectives of this study were to examine blastocyst development in vitrified, slow-frozen and unfrozen control bovine morulae, and to investigate their differential gene expression, using microarray analysis.
Material and methods
Chemicals and culture media
All chemicals were purchase from Sigma-Aldrich® (Oakville, ON, Canada), unless otherwise specified. Calf serum (CS; Cat#12484–010), Dulbecco’s Phosphate Buffer Saline (DPBS Ca2+-Mg2+ plus; Cat# 21300–025) and Tissue Culture Medium-199 (TCM-199 (Cat# 12340–030) were purchased from Invitrogen Inc. (Burlington, ON, Canada). Lutropin-V (LH; Cat # 1215094) and Folltropin-V (FSH; Cat # PHD075) were obtained from Bioniche® Animal Health, Inc. (Belleville, ON, Canada). Cryotops for vitrification and 0.25-ml straws for slow freezing were purchased from Kitazato® Co. (Fuzi, Shizuoka, Japan) and IMV® Tech. (Woodstock, ON, Canada), respectively.
Cumulus oocyte complex (COC) collection
Cow ovaries were collected from a commercial slaughterhouse (Cargill®, Calgary) and transported to Saskatoon at 20–25°C within 12–18 h. Ovaries, after trimming extra tissue, were washed with normal saline at room temperature. Follicular fluid containing cumulus oocyte complexes (COCs) was aspirated from <4mm ovarian follicles using an 18-gauge needle attached to 5-ml syringe, and pooled among ovaries for further processing.
In vitro embryo (morulae) production
The pooled follicular fluid was searched for COCs under stereomicroscope. COCs were washed in holding solution (HS; 5% CS in 1X DPBS) and graded as described earlier . First and second grade COCs were washed (3X) in maturation medium [TCM-199 supplemented with 5% CS, LH (5 μg/ml), FSH (0.5 μg/ml) and gentamicin (0.05 μg/ml)]. For in vitro maturation, groups of ~20 oocytes were placed in 100 μl droplets of maturation medium under mineral oil, and incubated at 38.5°C, 5% CO2 in air and saturated humidity, for 22–24 h.
For in vitro fertilization (IVF), two semen straws from a fertile bull were thawed at 37°C for 1 min. Semen was pooled and washed through Percoll gradient (45% and 90%) . After washing, sperm were diluted in Brackett-Oliphant (BO) fertilization medium to a final concentration 3x106/ml  [BO stock A + BO stock B + sodium pyruvate (1.3% w/v) + gentamicin (0.05 μg/ml)]. Following IVM, groups of 20 mature COCs were washed (3X) in BO medium supplemented with 10% (w/v) bovine serum albumin and added to 100 μl droplets of sperm in BO medium, under mineral oil, and incubated at 38.5°C, 5% CO2 in air and saturated humidity. After 18–22 h co-incubation of sperm and COCs, zygotes were washed and cultured in vitro (IVC) in CR1aa medium  supplemented with 5% (v/v) CS at 38.5°C, 5% CO2, 5% O2 and 90% N2 in air, and saturated humidity. On d7 post-IVF, compact morulae were collected, washed in HS and randomly divided in control, vitrification or slow freezing groups. Control morulae were incubated in IVC medium for 24–48 h. The remaining morulae underwent cryopreservation (vitrification or slow freezing) as follows.
Cryopreservation of morulae
Vitrification was conducted as described earlier . Briefly, morulae were washed in HS and equilibrated in vitrification solution 1 [VS1; 7.5% Ethylene glycol (EG, v/v) + 7.5% dimethyl sulfoxide (DMSO, v/v) + 20% CS (v/v) in 1X DPBS] for 5 min at room temperature. Morulae (n = 3 to 4 in a given batch) were passed through three 20-μl droplets of vitrification solution 2 [VS2; 15% EG + 15% DMSO + 20% CS + 17.1% sucrose (w/v) in 1X DPBS] at 37°C within 1 min, placed on cryotop (Kitazato® Co., Fuzi, Shizuoka, Japan) in individual droplet with minimal volume of VS2, immediately plunged in liquid N2 and stored for at least 24 h before warming.
Slow freezing was done as described earlier . Briefly, morulae were washed (1X) and incubated in cryoprotectant freezing solution [1.5 M glycerol + 5% CS (v/v) in 1X DPBS] for 10 min at room temperature. Morulae were transferred to 0.25-ml plastic straws (IMV® Tech., Woodstock, ON, Canada), sealed and kept in the controlled rate freezer (Bio-Cool® III-80, FTS systems, SP Industries, Inc., Stone Ridge, NY, USA) already set at -7°C, for 5 min. Ice seeding was initiated by touching straws with an ultra-cold Q-tip immersed in liquid N2. The straws were placed back in freezer at -7°C for additional 10 min, cooled to -35°C at the rate of 0.5°C/min, quickly plunged in liquid N2 and stored for at least 24 h before warming.
Vitrified morulae on cryotop were transferred to warming solution [0.5 M sucrose (w/v) + 20% CS (v/v) in 1X DPBS] at 37°C and incubated for 5 min. Similarly, slow-frozen morulae in 0.25 ml plastic straws were held in air for 10 s and immersed in water bath at 37°C for 1 min. For glycerol removal, slow-frozen morulae were transferred to warming solution [0.7 M sucrose + 5% CS (v/v) in 1X DPBS] at 37°C and incubated for 5 min.
Morulae culture and blastocyst collection
Post-warm (vitrified and slow-frozen) morulae were washed with HS and cultured in CR1aa medium for 24–48 h to the expanded blastocyst stage. Blastocyst conversion rates (%) were calculated for each treatment group (control, vitrification and slow-freezing) as number of expanded blastocysts out of number of morulae used per group.
Expanded blastocysts (n = 5 to 7 per treatment per replicate) were pooled in 50–100 μl RNAse-free water in 0.5 ml cryovials (RNase-free; Neptune®, San Diego, CA). Expanded blastocysts were flash frozen by plunging cryovials in liquid N2 and shipped to Dép. des Sciences Animales, Université Laval, Quebec city, QC, for microarray analysis. Total five IVF/IVC/cryopreservation cycles (i.e. biological replicates) were conducted on separate dates. Four biological replicates were used in microarray analysis (i.e. one cryotube per treatment per cycle). Three biological replicates were used in quantitative real-time PCR (qRT-PCR) analysis. Two biological replicates (cycles) were common between microarray analysis and qRT-PCR. Different tubes containing blastocysts (within treatment and replicate) were used for microarray and qRT-PCR analyses.
All procedures for microarray experiment were conducted according to procedures described previously [22,35], with little modifications. Total RNA was extracted from blastocysts developed from vitrified, slow-frozen and control morulae (replicate-wise) using Arcturus Picopure® RNA isolation kit (Cat#KIT0204, Life Technologies, Burlington, ON). The samples were subjected to a DNAse I (Cat#79254, Qiagen® Inc., Toronto, ON) digestion on the column. Total RNA was eluted in 13 μl of elution buffer. The quality and quantity of RNA was analyzed using Agilent 2100 Bioanalyzer™ and Agilent RNA 6000® pico kit (Cat# 5067–1513, Agilent technologies, Santa Clara, CA) and stored at -80°C until microarray and qRT-PCR analyses. High quality RNA samples with RNA integrity number (RIN) over 7.0 were amplified using T7 RNA amplification procedure RiboAmp® HSPlus RNA Amplification Kit (Cat# KIT0525, Life™ technologies, Burlington, ON) and used for microarray hybridization.
The amplified RNA (aRNA) samples from control, vitrified and slow-frozen blastocysts (replicate wise) were labeled with DY-547/647 (Green–Cy3 and Red–Cy5) fluorescent dyes using Universal Labeling System (ULS™) Labeling Kit (Cat# EA-021, Kreatech® Diagnostics, Amsterdam, The Netherlands), as recommended by manufacturer. The unfrozen control group was used as reference for both vitrification and slow freezing groups, therefore 4 μg aRNA from control samples, and 2.5 μg aRNA from each vitrification and slow freezing samples were labeled with Cy3 or Cy5 dyes. Non-reacted residual dyes were filtered out using Picopure RNA isolation kit (Cat#KIT0204, Life™ Technologies, Burlington, ON) without DNAse I treatment. Pure labeled aRNA was eluted with 13 μl elution buffer. Labeling efficiency for both dyes was measured with NanoDrop™ ND-1000 spectrophotometer (Nanodrop Technologies, Wilmington, DE, USA) with a minimum 30 pmol/μg (dye concentration/aRNA concentration) for each sample.
Two custom-built bovine microarray slides (EmbryoGENE EMBV3 manufactured by Agilent® technologies GEO Accession #: GPL13226, Design ID-028298), were used . Each slide consisted of 4 arrays and each array contained 43,671 probes, including 21,139 unique genes and 9,322 novel transcribed regions (NTRs). One slide was used to compare control (reference) and vitrification groups, and other one to compare control (reference) and slow freezing groups. A hybridization mixture [containing 825 ng of each cyanine (Cy3 or Cy5) labeled aRNA, Agilent spikes, nuclease-free water, 10X blocking agent, and 25X fragmentation buffer], in total volume 55 μl, was pipetted onto the microarray slides. Four biological replicates in each comparison (control vs. vitrified or control vs. slow-frozen) were used in the experimental design, in dye-swap setup. Slides were incubated at 65°C for 17 h, washed with wash buffers, dried and scanned using Tecan PowerScanner™ (Tecan Group Ltd., Mannedorf, Switzerland) .
The quality of hybridization was determined from the distribution of signals generated by both channels, in addition to the negative and spike-in controls, as reported earlier . Repeatability and specificity of hybridization were visualized through the distribution across channels of repeated and control probes bearing an increasing number of mismatches, respectively. Within an experiment, the set of microarrays was compared through a correlation matrix that enabled the quick identification of poor and divergent replication.
The normalized and differential expression data from FlexArray® were uploaded and analyzed in Ingenuity® Pathway Analysis (IPA) software. Differential gene lists from vitrified vs. control (≥ ± 2-fold change and P < 0.05) and slow-frozen vs. control (≥ ± 1.5 fold change, P < 0.05), and vitrification vs. slow freezing (≥ ± 2 fold change, P < 0.05) were compared for functional analysis to obtain molecular, cellular and functional correlations.
Quantitative real-time PCR (qRT-PCR) analysis
Total RNA extraction from blastocysts developed from vitrified, slow-frozen and control morulae, and initial processing is described under microarray analysis. Total RNA was reverse transcribed to cDNA using qScript™ cDNA supermix (Cat#95048–100, Quanta Biosciences, Inc., MD, USA) following kit instructions. Total cDNA quantity was measured using Nanodrop spectrophotometer and stored in -80°C until further use. In addition, total RNA and cDNA were obtained from extra samples of pooled IVP bovine expanded blastocysts for primer optimization and standard curve generation.
Total 7 genes (AKR1B1, CLDN23, CYP11A1, KRT19, PLAU, SPP1 and TKTL1) and one housekeeping gene (conserved helix-loop-helix ubiquitous kinase, CHUK)  were selected for qRT-PCR analysis. Primer testing and optimization was done using end-point PCR implying Taq DNA polymerase (Cat#201203, Qiagen) kit. PCR products were visualized on 1% agarose gel, purified, quantified, and sequenced to confirm specificity and validity of primers. The list of selected genes and primers is presented in Table 1.
The cDNA equivalent to 0.2 embryos was used from each treatment group per replicate. Quantitative real-time PCR was done on Stratagene® Mx3005P fast thermal cycler (Agilent technologies, Santa Clara, CA) using QuantiFast® SYBR® green PCR kit (Qiagen). PCR protocol included initial step at 95°C for 5 min followed by 40 cycles of 95°C for 10 s and 60°C for 1 min.
Cycle threshold (CT) values were recorded for each selected gene for every treatment group. These CT values were used to calculate differential expression in blastocysts developed from vitrified and slow-frozen morulae vs. blastocysts developed from control morulae. At first, PCR efficiency was calculated using standard curve data for each gene and software used pair-wise fixed reallocation randomization test using Relative Expression Software Tool (REST® 2009, Qiagen). PCR efficiency ranging between 1.90 and 1.99 (i.e. 90% and 99%) was considered optimum for each gene.
The relative levels of a transcript for each treatment group were calculated as cycle threshold (CT) normalized separately (ΔCT) for levels of transcripts for house-keeping (CHUK) gene. A lower CT (or Δ CT) of “1” indicates approximately a two-fold (21) higher concentration of RNA.
Data on blastocyst development rate were analyzed using link-function for binary distribution (yes/no response variable). Three groups (control, vitrification, slow freezing) were considered categorical fixed-effect explanatory variables and replicate was considered as a random factor. Data were analyzed using Proc Glimmix in SAS® Enterprise Guide 4.3 (SAS). Data were arranged in columns for replicate, treatment, outcome (each embryo was coded as 1 = successful development, 0 = no development). Following common SAS syntax model was used: Proc glimmix method = quad; class = replicate treatment; model outcome (event = “1”) = treatment/ dist = bin link = logit; random intercept/subject = Replicate; run. If the p-value for treatment was ≤0.05, then least square means were compared using Tukey’s test.
Microarray data were normalized and analyzed as described earlier . After laser scanning the slides, image files and median signal intensities from each spot were obtained using Array-Pro™ software (Media Cybernetics Inc., Rockville, MD, USA). The gene-spot intensity file was uploaded in MIAME-compliant ELMA (EmbryoGENE Laboratory Information Management System and Microarray Analysis) portal. Data quality control (probe specificity, and variance between biological replicates and between treatments) was monitored by in-built Gydle™ software (http://www.gydle.com). The background and spot median intensities were uploaded and analyzed in FlexArray® software Version 1.6.3. For background normalization, background signal intensity was subtracted from median grayscale signal intensity of spots to obtain required correct signal intensity. In case of higher background intensity for a spot than the signal intensity, negative value was replaced with 0.5 as a default (false spots). The median value for each target was transformed to the log2 value and normalized “within array” for dye bias using non-parametric regression (locally weighted scatter plot smoothing “lowess”), and subjected to between array normalization to unify intensities across the arrays using quantile normalization methodology (GEO #: GSE45381), respectively . Linear Models for Microarray (LIMMA) and RNA-Seq data simple statistical analyses were done in FlexArray and lists of upregulated and downregulated genes were obtained for each comparison [i.e. vitrification vs. control (reference) group and slow freezing vs. control (reference) group]. Statistically adjusted signal intensity data for vitrification and slow-frozen were derived from the previously acquired data for vitrification-control and slow freezing-control groups and then in silico FlexArray analysis was conducted between vitrification and slow freezing (reference) groups. A gene was considered differentially expressed if the fold change was ≥ ± 2 with a P < 0.05. As no genes were detected as differentially expressed at fold change ± 2 in the slow freezing vs. control comparison, and additional analysis was performed by lowering the fold change threshold to ≥ ± 1.5. Microarray data have been deposited in NCBI’s Gene Expression Omnibus accessible through GEO SuperSeries accession number GSE95382. The fold changes from microarray and qRT-PCR data were compared using a Student’s t-test in Microsoft® Excel, for each tested gene.
Morula to blastocyst development rate
The blastocyst development rate (number of expanded blastocysts/number of morulae used; %) did not differ between vitrification and control groups (P > 0.05). The slow freezing group had the lowest blastocyst development rate among all three groups (P < 0.05; Fig 1).
Differential gene expression profile
Using FlexArray software, total 64 genes differentially expressed in blastocysts developed from vitrified compared to control morulae (fold change ≥ 2; P < 0.05); and 1 and 165 genes differentially expressed in blastocysts developed from slow-frozen compared to control morulae at fold change ≥ ± 2 and ≥ ± 1.5, respectively (P < 0.05; Table 2). In silico comparison revealed 75 genes differentially expressed in blastocysts developed from vitrified compared to slow-frozen morulae at fold change ≥ 2 (Table 2). Top 5 upregulated and 5 downregulated genes in blastocysts developed from vitrified vs. control morulae, slow-frozen vs. control morulae, and vitrified vs. slow-frozen morulae, are presented in Table 3.
Transcripts with known functions and novel transcripts are listed separately.
To understand broader implications of gene expression changes in blastocysts developed from vitrified and slow-frozen morulae, a list of potentially “inhibited” or “activated” upstream regulators was generated using IPA software. The analysis was based on the activation score ≥ ± 2 and P < 0.05. Activation score represents the direction of change for the function. Compared to blastocysts developed from control morulae, blastocysts developed from vitrified morulae had two “inhibited” upstream regulators i.e. NFKB and Tretinoin (Table 4). To provide a better picture, other upstream regulators are also listed in Table 4. Three upstream regulators (NFKB, Tretinoin and EGF) were common between blastocysts developed form vitrified vs. control morulae and vitrified vs. slow-frozen morulae.
Functional annotation and pathway analysis
The differentially expressed genes from the FlexArray analysis for each treatment comparison were uploaded in IPA software and analyzed to determine the affected cellular, molecular, physiological and disease-related pathways. Top 10 affected pathways in blastocysts developed from vitrified and slow-frozen morulae as compared with blastocysts developed from control morulae are presented in Fig 2. Among these, cellular movement, small molecule biochemistry, carbohydrate metabolism, cellular function and maintenance, cellular growth and proliferation, and cellular development pathways were common between blastocysts developed from vitrified and slow-frozen morulae. Similarly, 10 pathways affected in blastocysts developed from vitrified as compared with slow-frozen morulae are presented in Fig 2. Genes involved in well-known canonical pathways were also examined, using the IPA software and top 10 affected canonical pathways in vitrified vs. control, slow-frozen vs. control and vitrified vs. slow-frozen are presented in Fig 3. A network of top differentially expressed genes (P < 0.05; fold change ≥ ± 2) in blastocysts developed from vitrified as compared with control morulae is presented in Fig 4.
Higher log values relate to higher significance of the functions. Top 10 cellular and molecular functions in each comparison are illustrated. Taller bars are more significant than shorter bars and the dotted line represents the cut-off value for P ≤ 0.05, -log-value = 1.3. Abbreviations: CON–control; SF–slow freezing; VIT–vitrification.
Score ratio (open circles) depicts the number of genes affected in the treatment versus the total number of genes involved in the pathway (y-axis on right side of each figure).
All genes involved in this network are part of the matrix-remodeling network. Genes are arranged horizontally in four cell compartments (nucleus, cytoplasm, plasma membrane and extracellular space), based on subcellular location of their gene products. The differences in color intensity of molecules show the degree of up- (red) and down- (green) regulation. The relationship lines between molecules and functions are supported by at least one reference derived from the literature, textbooks, and/or canonical pathways stored in Ingenuity® Knowledge Base.
Quantitative real-time PCR
Based on microarray data and function analysis, 6 differentially expressed genes (AKR1B1, CLDN23, CYP11A1, KRT19, PLAU and TKTL1) from vitrification group and 1 gene (SPP1) from slow freezing group were selected for validation with qRT-PCR. After quantification in three independent biological replicates from treatment (vitrification and slow freezing) and control groups, differential expression was validated in 7 genes (90% confidence level; P ≤ 0.01; Fig 5).
Black bars represent the differential level of expression of transcripts detected in the microarray analysis, while light grey bars represent the differential level of expression of the same transcripts obtained by qRT-PCR analysis. Asterisks (*) represent difference between gene expressions determined by microarray and qRT-PCR (P ≤ 0.01) analyses. NS = nonsignificant.
This is the first report, to our knowledge, on the comparison of differential gene expression in bovine blastocysts following vitrification and slow freezing at morula stage. In this study, vitrification of bovine morulae demonstrated better survival rate than slow freezing. However, this is the first report on the poor quality of surviving blastocysts developed from vitrified morulae at transcriptome level comparing with blastocysts developed from control morulae. Microarray data revealed that blastocysts developed from vitrified morulae may have impaired implantation and placentation in uterus. On the other side, the majority of morulae did not survive slow freezing method but those which survived to the blastocyst stage showed a similar transcriptome compared to blastocysts developed from control morulae.
In the present study, vitrification at morula stage affected the lipid metabolism and excretion mechanisms in in vitro produced bovine blastocysts. During slow freezing, the fluidic lipid portion of cell membrane changes into gel phase called ‘lipid phase transition’ . In vitrification, embryos are exposed to the permeating cryoprotectants in high concentration and undergo ultra-fast cooling rate by direct plunging in liquid nitrogen . In this procedure, embryos turn into glass-like solid phase, avoiding intracellular ice formation, as confirmed by synchrotron x-ray diffraction method . However, vitrification causes irreversible damage to cell membranes in bovine embryos . Membrane phospholipids [arachidonic acid and polyunsaturated fatty acids (PUFA)] are source for steroid metabolism. The current study revealed the downregulation of genes involved in steroid biosynthesis, pregnenolone biosynthesis and eicosanoid signaling (cytochrome P450 subunit 11 type A 1 (CYP11A1), 3-beta hydroxy steroid dehydrogenase delta-isomerase type 1 (HSD3B1), ATP-binding cassette subfamily C-2 (ABCC2) and prostaglandin synthase 2 (PTGS2) / cyclooxygenase 2 (COX2) in blastocysts developed from vitrified morulae. Earlier, the genes involved in purine metabolism and sphingolipid metabolism were upregulated in vitrified blastocysts . This difference in gene regulation could be due to the difference in embryonic stage (morula vs. blastocyst) at which vitrification was done. The lipid metabolism genes (CYP11A1, HSD3B1 and APOA1), involved in retinoids and their receptor (FXR/RXR) pathway were also downregulated in this study. FXR/RXR are expressed in inner cell mass (ICM) and trophectoderm (TE) cells and enhance blastocyst development and hatching in sheep and cattle [41,42].
In this study, CYP11A1, HSD3B1, PTGS2 and aldo-keto reductases family 1 B1 (AKR1B1) genes were downregulated. These genes are involved in steroid metabolism and are important for embryo implantation and placentation [43,44]. The impaired gene expression of CYP11A1 leads to inefficient lipid metabolism and defective placentation which are hallmarks of transcriptional deregulations in pre-eclamptic conditions . Therefore, it is suggested that vitrification downregulates the genes involving implantation of bovine blastocysts. This hypothesis will be further discussed in subsequent sections along with other genes and pathways.
Vitrification is known for cytotoxicity associated with high concentration of the permeating cryoprotectants (DMSO and EG). This study demonstrated the downregulation of genes associated with cellular uptake and efflux of cholesterol and fatty acids [apolipoprotein type A1 (APOA1) and ABCC2] from the external media and are actively involved in cellular detoxification through waste disposal (detoxification) during oxidative stress [46–48]. This is an important mechanism for the survival of semi-independent pre-implantation embryos. Similarly, AKR1B1 also performs detoxification that protects cells against lipid peroxidation products and toxic carbonyl-compounds produced during cell metabolism under stressful conditions .
The use of serum and/or bovine serum albumin in in vitro culture media renders bovine embryos susceptible to cryodamage due to increased cytoplasmic lipid content [50,51]. The downregulation of lipid metabolism and external uptake in stressful conditions may be responsible for better survival of vitrified than slow-frozen morulae to blastocyst stage. These findings support “quiet embryo” hypothesis i.e. embryo with relatively low metabolic activity survive better . The addition of phenazine ethosulfate, a metabolic inhibitor for fatty acid synthesis, reduced lipid accumulation and increased blastocyst re-expansion after vitrification .
An important aspect of bovine embryo development is the blastocyst formation from morula stage which involves differentiation of blastomeres into ICM and TE cells. Claudin family and actinγ2 (ACTG2) are involved in formation of tight cell junctions in placental development [54,55]. These tight junctions prevent leakage of fluid during blastocoel formation, and support blastocyst expansion and hatching processes . The downregulation of claudin and actin genes led us to develop a notion that vitrification delays the hatching of blastocysts. This supported previous findings that vitrification caused downregulation of tight junction and cell adhesion (tight junction protein and desmocollin2 genes in bovine blastocysts .
Cytokines (IFNT and IFNG) and growth factors (EGF, FGF, TGFB and IGFBPB) present in uterus, involved in cell growth, proliferation and differentiation, are important for transformation of morula to blastocyst and subsequent hatching. IFNT and IFNG play major roles in embryo signaling, maternal recognition of pregnancy, immune regulation and establishment of pregnancy [57,58]. IFNG secreted by the implanting embryos, inhibits the production of prostaglandin synthase (PGS) in bovine . Interestingly, the expression of CALB1, PTGS2, PLAU, KRT19 and CYP11A1 genes was downregulated in blastocysts developed from vitrified morulae in this study. Another study failed to detect such change in IFN expression levels . In the present study, keratin family (KRT19) and urokinase-based plasminogen activator (PLAU) genes were also downregulated in blastocysts developed from vitrified morulae. The PLAU is a key player in implantation and its downregulation has been associated with resorbed embryos in bovine . Taken together, the downregulation of keratin family and PLAU along with predicted decrease in upstream regulator IFNG suggests the possible impairment in early embryo recognition and implantation process in vitrified embryos.
In the current study, IPA analysis of differentially expressed genes indicated apoptosis (NFKB, CYP11A1, AKR1B1, CALB1 and PLAU) and necrosis (TGFB, IFNG, PLAU, KRT19, CYP11A1, ABCC2, and CCL17) pathways in blastocysts developed from vitrified morulae. Necrosis is a large scale cellular damage associated with membrane damage, nuclear disintegration and cellular swelling, thus may affect whole embryo survival . Apoptosis, a physiological process, is usually associated with single cell damage i.e. cytoplasmic shrinkage, chromatin condensation and DNA damage leaving adjacent cells intact. Apoptosis of individual blastomere is a part of strategy of embryo survival under stressful circumstances . This seems to be true for greater survival rate in vitrified morulae than slow-frozen.
Interestingly, the surviving blastocysts developed from slow-frozen morulae showed fewer changes in gene expression comparing with blastocysts developed from control morulae but differed significantly comparing with blastocysts developed from vitrified morulae. The upregulation of cell structure and morphology genes microtubule polymerization, doublecortin-like kinase 2 (DCLK2) and zinc finger MYM 6 (ZMYM6) compared to control group may be the compensatory mechanisms for cell structure damage. Vimentin (VIM) was also downregulated in blastocysts developed from slow-frozen morulae. VIM encodes a protein member of cellular intermediate filaments known to enhance cell elasticity, capacity to adapt stress and thus is important for normal bovine embryo development . Other upregulated genes in slow-frozen blastocysts related to membrane lipid metabolizing enzymes i.e. phospholipase A2 recepetor 1 (PLA2R1) and sphingomyelin phosphodiestrase 3 (SMPD3) depict the utilization of embryo’s internal resources for metabolism. These changes point towards the viability and better quality of blastocysts developed from slow-frozen which survived the transition from morula to blastocyst after warming.
Vitrification is becoming popular under field conditions due to high embryo survival rates as well as the ease of technique . Their study demonstrated higher morula to blastocyst rate in vitrified blastocysts (77%) than slow-frozen blastocysts (34%). Similar results were obtained in the present and earlier studies on bovine embryos [10,64,65]. Interestingly, in silico comparison between blastocysts developed from vitrified and slow-frozen morulae revealed similar changes in gene expression as between blastocysts from vitrified and control morulae. Similar pathways like lipid metabolism and cell movement and adhesion were affected. Inspite of better survival, a similar pregnancy rate (~45%) was observed after transfer of vitrified and slow-frozen bovine embryos, under field conditions . Studies conducted on rabbit morulae following vitrification demonstrated impaired trophoblast proliferation and differentiation, retarded fetal development and altered gene expression (ANXA3, EGFLAM and TNAIP6) compared to slow-frozen blastocysts [66,67]. Based on discussion in previous sections and considering the field pregnancy data in cattle, we anticipate that vitrified blastocysts compared to slow-frozen blastocysts have higher failure rate during maternal recognition of pregnancy and pre-implantation, resulting in similar pregnancy rates by 30-days of gestation. This hypothesis needs to be tested further.
Bovine embryos between compact morula- and blastocyst-stage, suitable for non-surgical embryo transfer, are frozen with great success . Morula/early blastocyst is a favourite stage for cryopreservation to avoid embryo manipulation like blastocoel collapse in the expanded blastocyst . In this study, compact morulae were cryopreserved so that post-warm transcriptomic changes could be expressed at later (blastocyst) stage. This study represented transcriptomic changes in bovine embryos cryopreserved at morula stage. It is anticipated that transcriptomic changes of bovine embryos may be different if cryopreserved at the expanded blastocyst stage.
Blastocysts developed from vitrified morulae showed downregulation of genes involved in lipid metabolism, cell differentiation and cell adhesion leading to impaired implantation. Although the survival rate of blastocysts developed from slow-frozen morulae was poor, the intensity of changes in gene expression was low comparing with blastocysts developed from unfrozen control morulae. Also, gene expression changes between blastocysts developed from vitrified vs. slow-frozen morulae were similar as between blastocysts developed from vitrified vs. control morulae. Generally, the cryosurvival of morulae is assessed at blastocyst, expanded blastocyst and/or hatched blastocyst stages. It will be important to study the developmental competence of cryopreserved embryos beyond blastocyst stage, like implantation, placentation and actual pregnancy.
This study was funded by Natural Sciences and Engineering Research Council of Canada (NSERC), and Agriculture and Agri-food Canada. Authors are thankful to Dr. Kosala Rajapaksha for his technical help in this study
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