Next Article in Journal
Conservation Assessment of the State Goat Farms by Using SNP Genotyping Data
Next Article in Special Issue
Cortical Granule Distribution and Expression Pattern of Genes Regulating Cellular Component Size, Morphogenesis, and Potential to Differentiation are Related to Oocyte Developmental Competence and Maturational Capacity In Vivo and In Vitro
Previous Article in Journal
Nucleophosmin 1 Mutations in Acute Myeloid Leukemia
 
 
Search for Articles:
Title / Keyword
Author / Affiliation / Email
Journal
Article Type
 
 
Advanced Search
 
Section
Special Issue
Volume
Issue
Number
Page
 
Journals
Genes
Volume 11
Issue 6
10.3390/genes11060651
genes-logo
Submit to this Journal Review for this Journal Propose a Special Issue
► Article Menu

Article Menu

share Share announcement Help format_quote Cite question_answer Discuss in SciProfiles thumb_up
...
Endorse textsms
...
Comment
first_page
settings
Order Article Reprints
Font Type:
Arial Georgia Verdana
Font Size:
Aa Aa Aa
Line Spacing:
Column Width:
Background:
Article

Transcription Analysis of the Chemerin Impact on Gene Expression Profile in the Luteal Cells of Gilts

by
Karol G. Makowczenko
1,
Jan P. Jastrzebski
2,3,
Karol Szeszko
1,
Nina Smolinska
1,
Lukasz Paukszto
2,3,
Kamil Dobrzyn
1,
Marta Kiezun
1,
Edyta Rytelewska
1,
Barbara Kaminska
1 and
Tadeusz Kaminski
1,*
1
Department of Animal Anatomy and Physiology, Faculty of Biology and Biotechnology, University of Warmia and Mazury in Olsztyn, Oczapowskiego 1A, 10-719 Olsztyn, Poland
2
Bioinformatics Core Facility, Faculty of Biology and Biotechnology, University of Warmia and Mazury in Olsztyn, Oczapowskiego 1A, 10-719 Olsztyn, Poland
3
Department of Plant Physiology, Genetics and Biotechnology, Faculty of Biology and Biotechnology, University of Warmia and Mazury in Olsztyn, Oczapowskiego 1A, 10-719 Olsztyn, Poland
*
Author to whom correspondence should be addressed.
Genes 2020, 11(6), 651; https://doi.org/10.3390/genes11060651
Submission received: 19 May 2020 / Revised: 9 June 2020 / Accepted: 10 June 2020 / Published: 12 June 2020
(This article belongs to the Special Issue Genomic Studies in the Mammalian Reproductive Tract)
Browse Figures
Versions Notes

Abstract

:
Chemerin is a recently discovered adipokine that participates in the regulation of many physiological and disorder-related processes in mammals, including metabolism, inflammatory reactions, obesity, and reproduction. We investigated how chemerin affects the transcriptome profile of porcine luteal cells. The luteal cells were acquired from mature gilts. After the in vitro culturing with and without chemerin, the total RNAs were isolated and high-throughput sequencing was performed. Obtained datasets were processed using bioinformatic tools. The study revealed 509 differentially expressed genes under the chemerin influence. Their products take part in many processes, important for the functions of the corpus luteum, such as steroids and prostaglandins synthesis, NF-κB and JAK/STAT signal transducing pathways, and apoptosis. The expression of the CASP3, HSD3B7, IL1B, and PTGS2 genes, due to their important role in the physiology of the corpus luteum, was validated using the quantitative real-time polymerase chain reaction (qPCR) method. The qPCR confirmed the changes of gene expression. Chemerin in physiological concentrations significantly affects the expression of many genes in luteal cells of pigs, which is likely to result in modification of physiological processes related to reproduction.

1. Introduction

Chemerin (CHEM) is an adipokine discovered more than 20 years ago, as a product of TIG2, later named as RARRES2. This substance was first identified during studies on the pathogenesis of psoriasis in 1997 as a product undergoing increased production under the influence of tazarotene [1]. To date, the occurrence of RARRES2 mRNA was found, e.g., in the ovaries of women [2], mice [3], and rats [4]. In accordance to the Du and Leung studies, the swine CHEM amino acid sequence has the highest level of identity with respect to the human sequence (84%) among all of tested model animals – cattle, rats, and mice [5].
To date, three CHEM membrane receptors have been identified [6]—CMKLR1 (also named as ChemR23 or GPCR-DEZ), GPR1 and CCRL2. The first two mentioned receptors—CMKLR1 and GPR1—show a high structural similarity and they are ‘classic’ chemokine receptors, associated with G-proteins, which initiate intracellular signal transduction. The expression of CMKLR1 was reported in human ovarian cells [2] and the production of GPR1 mRNA was detected in the murine corpus luteum (CL) [7]. The effect of action of the third membrane receptor of CHEM, CCRL2, is regulation of ligand molecules availability and creation of chemokine or non-chemokine ligands gradient in in vivo [8] and in vitro [9] conditions, determining the direction of inflammatory reactions. It has been found that CCRL2 gene expresses in the human ovaries [2].
Recently, attention of researchers was also paid to contribution of CHEM to the influence on human and animal reproduction [2,7,10,11,12,13]. Yao and his team observed an increased accumulation of reactive oxygen species and an increase in granulosa cells (GC) apoptosis in the ovaries of mice in which upregulation of the expression of CHEM and CMKLR1-encoding genes was induced by a high-fat diet [14]. In human, mouse, and bovine GC, the influence of CHEM on the inhibition of steroidogenesis was found [2,7,12]. In addition, CHEM in rats triggers follicular growth arrest [15]. To date, the influence of CHEM on luteal cells (LC) has not been studied. Moreover, most studies analyzing the impact of CHEM on various physiological processes are carried out in humans or rodents, and often do not consider farm animals, including pigs—model organism of major importance to the human farming economy.
Our recent studies have shown the presence of all three CHEM-associated receptors in selected structures of the pig hypothalamus [16] and ovary [17] during the estrous cycle and early pregnancy, which allowed us to conclude that CHEM has a direct effect on the hypothalamic–pituitary–gonadal regulatory axis (HPG) by modifying the functioning of its upstream structures. We hypothesized that CHEM may have endocrine effects on downstream structures of the HPG axis, in particular on CL producing steroid hormones, significantly modifying reproductive processes in mammals. The aim of this study was to investigate the influence of CHEM on the transcriptomic profile of swine in vitro cultured luteal cells collected during the mid-luteal phase of the estrous cycle.

2. Materials and Methods

2.1. Experimental Animals and Tissue Collection

Five mature gilts (Large White × Polish Landrace; 7–8 months of age; body weight of 120–130 kg) obtained from a private breeding farm were used in this study. The gilts were on days 10–12 of the estrous cycle. Females were observed daily for behavioral estrus in the presence of boar. The day of onset of the second estrus was designated as day 0 of the estrous cycle. The phase of the estrous cycle was additionally confirmed based on ovarian morphology [18]. Ovaries collected immediately after slaughter of gilts were placed in ice-cold PBS supplemented with 100 IU/mL penicillin and 100 µg/mL streptomycin and transported to the laboratory on ice within 1 h for in vitro cell cultures preparation. The experiments were carried out in accordance with the ethical standards of the Animal Ethics Committee at the University of Warmia and Mazury in Olsztyn.

2.2. Isolation of the Luteal Cells and in Vitro Cell Cultures

Luteal cells were isolated using the method described by Kaminski et al. [19]. Dissected from ovaries corpora lutea on days 10–12 of the cycle (the mid-luteal period of fully functional CL) were minced into small fragments and dispersed in F-12 medium containing BSA (1%) and antibiotics. Corpora lutea were enzymatically dissociated in 0.125% trypsin solution (4–6 times) at 38 °C, centrifuged (300× g, 10 min, 21 °C), and washed three times. Isolated LC were filtered through nylon mesh (75 µm) and resuspended in fresh F-12 medium. The cells were counted using a hemocytometer, and their viability (≈90%) was determined by 0.4% trypan blue dye exclusion.
Luteal cells (2 × 106/2 mL medium) were resuspended in F-12 medium enriched with FCS (20%), BSA (1%), and antibiotics, and pre-incubated for 48 h in a humidified incubator with 95% air and 5% CO2 atmosphere. The serum-containing medium was discarded, and the cells were washed using serum-free F-12 medium. After washing, LC were cultured for 24 h in F-12 medium with BSA (1%) and antibiotics, with or without recombinant human CHEM in concentration 200 ng/mL of medium. The concentration of the factor was selected on the basis of its relatively high level in women and porcine blood plasma [16,20].

2.3. RNA Isolation and High-Throughput Sequencing

Total RNA was extracted from in vitro cell cultures using RNeasy Mini Kit (Qiagen, Germantown, MD, USA) with DNase (RNase-free DNase Set, Qiagen, Germantown, MD, USA), according to manufacturer’s recommendations. The RNA quantity (wavelength 260 nm, A260) and purity (A260/A280) was assessed spectrophotometrically (Infinite M200 Pro, Tecan, Männedorf, Switzerland). Integrity of the total RNA was validated by electrophoresis on 1% agarose. Isolated RNA was stored at −80 °C for sequencing library preparation.
The sequencing library of template molecules suitable for following cluster generation was prepared using total RNA (from each sample) according to Shen et al. [21]. Firstly, the RNA solutions were purified from rRNA with use of Ribo-Zero rRNA Removal Kit (Illumina, San Diego, CA, USA). rRNA-depleted RNA was used to prepare strand-specific libraries using the TruSeq Stranded mRNA Library Prep Kit (Illumina, San Diego, CA, USA), following manufacturer’s protocol. Briefly, RNA was fragmented, ds-cDNA was synthesized replacing dTTPs with dUTPs in the reaction solution used in second strand cDNA synthesis. The obtained ds-cDNA fragments went through an end repair and A-tailing processes. Finally, specific adaptors were ligated to the obtained cDNA fragments. Polymerase chain reaction amplification was performed to enrich cDNA libraries.
The transcriptome high-throughput sequencing (RNA-Seq) of obtained cDNA libraries was performed on the NovaSeq 6000 platform (Illumina, San Diego, CA, USA) to generate 2 × 150 bp paired-end reads, with assumed minimal sequencing depth—100 million reads per sample.

2.4. In Silico Analyses

2.4.1. Row Reads Pre-Processing and Differentially Expressed Genes Processing

This stage of analysis was performed accordingly to Pertea et al. [22] with significant modifications (Figure 1). Row reads obtained from sequencing were subjected to quality control, using FastQC v0.11.8 software [23]. Adapters and low-quality regions of row reads were trimmed with use of Trimmomatic v0.38 program [24]. After re-checking the quality and adapter content of processed reads, they were mapped with the use of STAR mapper v2.6.1d [25] to the Sus scrofa v11.1.91 reference genome downloaded from Ensembl database [26]. The number of reads mapped to exonic, intronic, untranslated regions (UTRs), or intergenic regions was quantified using the CollectRnaSeqMetrics tool in the Picard v2.21.1 software [27]. Principal component analysis (PCA) and Euclidean distances between samples analysis were performed using ggplot2 library [28] and self-developed R script [29], to assess the overall similarity between transcriptomic profiles of RNA samples derived from CHEM-treated and non-CHEM-treated cells. StringTie aligner v1.3.5 [30] was used to enrich annotation of transcripts and prepare the Ballgown input files, with the fr-firststrand (--rf) enabled parameter. Counts per gene were computed on the basis of BAM files (alignments obtained from STAR) and GTF files (annotations from StringTie) using the prepDE python script with the Ballgown software [31]. Row reads were deposited in the European Nucleotide Archive database under the common project accession number—PRJEB35892.
Statistical analyses of differentially expressed genes (DEGs) for protein-coding RNA under the influence of CHEM was performed using Ballgown [31], dedicated Bioconductor v3.8 [32] package prepared for the R environment v3.5.2 [33], with the following operating parameters: q-value < 0.05 and |log2FC| ≥ 0.5.

2.4.2. Functional Annotation of Differentially Expressed Genes

Functional analyses (gene ontology and pathway enrichment) were performed with use of g:Profiler [34] and KO-Based Annotation System v3.0 (KOBAS) [35] web tools related to Kyoto Encyclopedia of Genes and Genomes (KEGG) [36], Gene Ontology (GO) [37,38], and The Reactome Knowledgebase [39] databases.

2.5. Quantitative Real-Time PCR Validations

Quantitative real-time PCR (qPCR) was proceeded by cDNA synthesis using the same RNA as in the RNA-Seq (all CHEM-treated and control samples). A total of 500 ng of each total RNA sample was transcribed using the Omniscript RT Kit (Qiagen, Germantown, MD, USA), a mix of dNTPs and 0.5 μg oligo(dT) (Roche, Penzberg, Germany) in a total volume of 10 µL. The reaction was conducted at 37 °C for 1 h and was terminated by incubation at 93 °C for 5 min. qPCR was performed in technical duplicate for each sample with use of the 7300 PCR System (Applied Biosystems, Foster, CA, USA). The protocol assumed to use constitutively expressed ACTB and GAPDH as reference genes. Primer sequences for reference and target genes (CASP3, HSD3B7, IL1B, and PTGS2) were developed using Primer Express Software 3 (Applied Biosystems, USA). Quantitative real-time PCR mixtures with a final volume of 20 μL consisted of cDNA (40 μg), 400 nM of the primers, 12.5 μL of the Power SYBR Green PCR Master Mix (Applied Biosystems, USA), and RNase-free water. The primer sequences of all tested genes are listed in Table 1. Quantitative real-time PCR were performed under the following conditions: preliminary cDNA denaturation and enzymes activation at 95 °C for 10 min, followed by 40 cycles of denaturation at 95 °C for 15 s, annealing at 60 °C for 1 min, and elongation at 72 °C for 1 min. For ACTB and HSD3B7 primers the annealing temperature was raised to 61 °C. Negative controls were prepared by replacing cDNA with water. All the samples were in duplicate. Calculation of the relative expression levels of validated genes was performed with use of the comparative cycle threshold method (ΔΔCT) and normalized using the geometrical means of the reference gene expression levels [40]. The results of qPCR were statistically processed in the R environment [33] with the use of one-factor ANOVA and were presented as mean values ± SEM. The results were regarded as statistically significant at p-value < 0.05.

3. Results

3.1. Overall Statistics of RNA-Seq Data and Mapping Results

The in vitro cultured LC sampled from five CHEM-treated groups and five control groups were used to create total cDNA libraries to explore the effect of CHEM treatment on the porcine LC transcriptome. The transcriptome high-throughput sequencing generated 1,154,494,264 raw paired-end reads. After pre-processing (minimum 90 bp length, Phred quality score > 30) and the removal of adapter sequences, 1,024,385,352 clean reads were obtained, of them 1,018,891,762 were mapped to the reference porcine genome (S. scrofa v11.1.91). On average, 96.52% of trimmed reads were uniquely mapped, 3.48% were mapped to multiple loci (Table 2).
In all libraries, 56.63% of processed reads were mapped to coding DNA sequence (CDS) regions, 22.08% were aligned to UTRs, 2.59% to introns, and 18.69% to intergenic locations (Figure 2). A total of 16,612 transcriptionally active regions (TARs) were identified in LC in at least half of the samples.
Principal component analysis revealed a high degree of differentiation in gene expression profiles between research and control samples (Figure 3A). The calculated Euclidean distances showed high consistency of the expression profiles, both within the control group and the experimental group (Figure 3B).

3.2. Differentially Expressed Genes

Ballgown-based analysis revealed that 509 genes (721 transcripts) showed statistically significant differences in expression between CHEM-treated and control samples (Table S1). The significant changes in gene expression profiles of in vitro cultured LC treated with CHEM are visualized in Figure 4. The 98 DEGs involved in metabolic pathways relevant for physiological functions of the corpus luteum (described below) are presented in a heatmap (Figure 5). Among all DEGs, 301 were upregulated and 208 were downregulated in the CHEM-treated group (Supplementary Table S1), and log2FC values ranged from 5.45 (IL1B) to −2.17 (PANK1). The 10 most upregulated genes were IL1B, CSF3, CCL3L1, CXCL8, CCL20, CXCL2, ENSSSCG00000008954, AMCF-II, ACOD1, and IL23A. The 10 most downregulated genes were PANK1, SLA-DMA, ENSSSCG00000031640, SLA-DMB, ENSSSCG00000016725, PTGFR, FMNL2, ANKRD1, LYZ, and KCNK3 (Table S1).

3.3. Functional Genes Analysis

The GO enrichment analysis demonstrated that in the group of all DEGs, a total of 457 were associated with three aspects: biological process (BP), molecular function (MF), and cellular component (CC) GO terms (Figure 6). The BP aspect encompassed DEGs enriched to 407 statistically significant GO terms (padj < 0.05), for example: ‘cellular response to stimulus’, ‘regulation of signal transduction’, ‘immune system process’, ‘programmed cell death’, ‘response to cytokine’, ‘cytokine production’, and ‘I-kappaB kinase/NF-kappaB signaling’. Within the MF aspect, DEGs were enriched to 18 functions, for example ‘cytokine receptor binding’, ‘receptor regulator activity’, ‘growth factor receptor binding’, and ‘CCR chemokine receptor binding’. In the CC aspect, there were 15 significant GO terms, for example ‘extracellular region’, ‘cell surface’, ‘cytoplasm’, and ‘cell-cell junction’.
A subsequent KEGG enrichment classification revealed that 286 DEGs significantly affected by CHEM, had a statistically significant (padj < 0.05) impact on 51 biological pathways. Among all selected metabolic pathways, 32 were directly related to pathological processes such as carcinogenesis, autoimmune diseases, bacterial, viral infections, and those initiated by prions and protists. Due to the lack of relation with the studied tissue and the aim of understanding the physiological influence of CHEM on LC, these pathways were not analyzed. We investigated the impact of DEGs on the following signal pathways: ‘TNF signaling pathway’, ‘Cytokine-cytokine receptor interaction’, ‘NF-kappa B signaling pathway’, ‘Chemokine signaling pathway’, ‘MAPK signaling pathway’, ‘Cell adhesion molecules (CAMs)’, and ‘Apoptosis’ (Figures S1–S7). Additionally, following pathways, important for the CL functioning, that did not reach statistical significance during KEGG enrichment, were examined: ‘Steroid hormone biosynthesis’, ‘Ovarian steroidogenesis’, ‘Arachidonic acid metabolism’, and ‘JAK-STAT signaling pathway’ (Figures S8–S11).
The Reactome Knowledgebase enrichment analysis showed a significant contribution of 261 DEGs from the set obtained during this study in 19 molecular pathways, for example ‘Cytokine signaling in immune system’, ‘Programmed cell death’, ‘TAK1 activates NFkB by phosphorylation and activation of IKKs complex’, ‘Interleukin-1 signaling’, and ‘Chemokine receptors bind chemokines’.

3.4. Quantitative Real-Time PCR Validations

To validate the obtained RNA-Seq results, four DEGs were selected for qPCR. The qPCR expression patterns of HSD3B7, IL1B, PTGS2 were in agreement with RNA-Seq results. Changes in levels of CASP3 expression between CHEM-treated and control samples did not reach the statistical significance threshold (p-value = 0.06), but nevertheless indicated the trend that had been previously revealed during the analysis of RNA-Seq data. Results of qPCR mostly confirmed the veracity of the high-throughput methods used in the present study (Figure 7).

4. Discussion

The transcriptome high-throughput sequencing was applied to identify the global transcriptome profile of treated and non-treated in vitro-cultured porcine luteal cells, acquired on days 10–12 of the estrous cycle. During this study, we observed the statistically significant impact of CHEM on changes of expression levels of 509 genes, whose products are involved in several processes important for functioning of porcine LC, and thus CL.
Previous studies evidenced a significant impact of CHEM on the ovarian cells of other species, such as humans [2,43], mice [7], rats [44], and cattle [12]. Nevertheless, the cited studies did not analyze the effects of CHEM on the LC at the transcriptional level, using deep sequencing techniques that allow certain relationships to be found with greater probability and sensitivity. The authors would like to point out that in accordance to the literature data, gene expression affects at least 40% [45,46] of the variability of protein produced in mammalian cells. However, as stated by Li and co-workers [47], taking into account experimental errors, changes at the mRNA level explain up to 84% of the variance at the protein level.
Nuclear factor κB, the subunits’ production of which is strongly modified by CHEM in the porcine LC, is a protein complex controlling transcription of proteins, which contribute to the inflammatory response, through triggering synthesis of proinflammatory factors, regulating inflammatory reaction course, leukocyte recruitment, and apoptosis or cell survival [48]. Signal transduction can be carried out by ‘canonical’ pathway, activated by TNFα and IL1 or by ‘alternative’ pathway, in which the signal is activated by, among others, a CD40 membrane receptor [48]. Despite the lack of statistically significant change in the expression of TNFα-coding genes under the influence of CHEM, the level of TNFAIP3 mRNA produced by LC increased significantly (FC = 4.6). Furthermore, TNIP1 was 2.1-fold upregulated. TNF-receptor associated factor proteins are involved in the initial signal transduction in the ‘alternative’ NF-κB pathway. The expression of TRAF2 (FC = 2.6) was also modified by CHEM. Zmijewska and colleagues proved that IL1B in CL is secreted not only by macrophages but also by LC [49]. In CHEM-treated samples, we observed a 43.6-fold increase in the production of IL1B transcripts, an 8.1-fold increase in the production of IL1A transcripts, and a 2.0-fold increase in the production of IL1RAP transcripts, in comparison to control samples. Moreover, IRAK2 mediates the process of the NF-κB pathway activation by IL1 molecules [50], and its mRNA was produced in increased quantities under the influence of CHEM (FC = 1.7). Some of the proteins constructing the NF-κB complex, such as NFKB1 (FC = 1.8), NFKB2 (FC = 2.3), RELB (FC = 2.5), NFKBIA (FC = 4.2), NFKBIB (FC = 1.6), NFKBIE (FC = 2.0), and NFKBIZ (FC = 2.8) were upregulated. Proteins encoded by NFKB1 and NFKBIA participates in the ‘canonical’ pathway, whereas RELB and NFKB2 take a part in the ‘alternative’ NF-κB pathway. Interestingly, Xia and co-workers suggested that the ‘canonical’ pathway of the NF-κB can be inhibited by RELB protein, which is able to regulate the stability of protein encoded by the NFKBIA gene [51]. The effect of activating the ‘canonical’ pathway is an increase in the expression of many genes, such as mentioned IL1A, IL1B and IL18, PTGS2, PTGES, BIRC3, MCL1, and CFLAR, discussed in detail below [52]. As a result of previous studies conducted by Luo and colleagues [53], and Przygrodzka and colleagues [54], it was found that activation of the NF-κB pathway occurs in LC at a late luteal stage of the estrous cycle and is associated with the acquisition of luteolytic sensitivity by CL. This implies the participation of CHEM in the process of early acquisition of luteolysis capacity by LC. On the other hand, Vince and co-workers showed that TRAF2 must recruit proteins encoded by CIAP2 (also named as BIRC3 or HIAP1; FC = 1.7) to properly activate the NF-κB pathway and to create resistance to apoptosis induction [55]. Overexpression of genes encoding both proteins in LC transcriptomes treated with CHEM allows to assume also anti-apoptotic action of the described pathway.
The JAK/STAT pathway takes part in the transduction of signals associated with cell differentiation, proliferation, migration, or apoptosis [56]. It consists of only a few components, such as membrane receptors with a characteristic domain capable of binding JAK proteins, JAKs capable of phosphorylation STAT proteins, and a group of STATs, which activated and homodimerized may act as transcription factors [57]. The results revealed 2.3-fold upregulation of the STAT1 gene. More than 20 years ago, it was proven that STAT1 is an essential factor for the constitutive expression of, inter alia, CASP3 described below [58]. It was previously stated that homodimerization of STAT1 proteins is induced by IFNγ [59]. We did not identify any statistically significant increase in IFNγ-coding gene expression, but we did notice the upregulation of one of its receptors—IFNGR2 (FC = 1.8). Moreover, the expression of IL18, also known as IFNγ inducing factor-coding gene, and its receptor-coding gene (IL18R1) were, respectively, 2.1-fold and 1.5-fold upregulated. Tsuji and his colleagues discovered the production of IL18 and IL18R proteins directly by mouse LC, linking their observations to the paracrine and autocrine activity of these cells [60]. This may be an argument for probably more effective IFNγ action in the studied cells, despite the lack of a significant increase in the content of mRNAs. Furthermore, it has been confirmed that IFNγ may control porcine CL functions, including progesterone (P4) production [61,62]. Gene expression profiles also revealed differences in the content of SOCS3 (1.7-fold upregulation under CHEM influence) mRNA produced. SOCS3 is a known regulator of JAK/STAT pathway, induced by this pathway activation [56].
The corpus luteum is the primary endocrine gland that directly regulates the functioning of the uterus and modulates its transformation during the estrous cycle. Corpora lutea perform their function mainly by producing P4, a steroid hormone that prepares the endometrium for embryo implantation and is responsible for maintenance of gestation. The key steroidogenic enzyme involved in the production of P4 by LC is 3β-HSD. We observed a significant decrease in the content of HSD3B mRNA produced under the influence of CHEM (FC = 0.60), and we confirmed the expression of HSD3B by qPCR. Surprisingly, Rytelewska and co-workers [63] observed an induction of P4 secretion by CHEM-treated in vitro-cultured porcine LC obtained on days 10–12 of the estrous cycle. The difference between the observed amount of HSD3B mRNA in porcine LC and the level of P4 secretion may result from the negative feedback loop. The HSD3B feedback regulation by P4 was previously mentioned in rat ovaries by de Galarreta and co-workers [64], and Tanaka and colleagues [65]. Similarly, downregulation of HSD3B was noticed in testicular Leydig cells under the influence of androgens [66,67]. As a result of this mechanism, a large amount of P4 produced by LC may directly inhibit the expression of HSD3B. Furthermore, Rytelewska and colleagues [63] conducted analyses using in vitro LC cultures (identical to those used in this study) of the CHEM effect on basal and luteinizing hormone or follicle-stimulating hormone and/or insulin-induced secretion of other essential steroid hormones, such as androstenedione (A4), testosterone (T), estrone (E1), and estradiol (E2). The mentioned study revealed that CHEM inhibits basal and induced E2 secretion, and exerts both stimulatory and inhibitory effects on basal and induced secretion of A4, T, and E1 (depending on the phase of the estrous cycle). According to Rytelewska and co-workers [63], CHEM appears to be an important factor that modulates ovarian steroidogenesis in pigs, whereas its stimulatory or inhibitory effects on the secretion of steroid hormones may be due to the heterogeneity of factors regulating ovarian functions, possible interactions between these factors, and specific processes related to the ovarian physiology during different phases of the estrous cycle.
We found upregulation of cPLA2 (also named PLA2G4B; 1.9-fold increase), PTGS2 (also named COX2; 3.2-fold increase), and PTGES (2.3-fold increase). Enzymes encoded by these genes create the complete metabolic pathway, during which the arachidonic acid substrate is transformed into the final product, which is luteoprotective PGE2 [68]. In mammals, PGE2 is mainly responsible for the ovulation process and the subsequent luteinization of the ovarian follicle [69], which is also related to an increase in the production of HSD3B mRNA [70] and further in P4 secretion [71]. This assumption coincides with the observations of Zmijewska and co-workers [49] on the influence of IL1B on the expression of PTGS2 and PTGES genes, and thus PGE2 secretion. It is also probable that such a high increase in observed IL1B gene expression is the result of positive feedback loop via the NF-κB signal transduction pathway and upregulation of PTGS2 in swine LC, as was previously observed in human intervertebral disc cells [72]. Interestingly, it was affirmed that expression of the PTGES gene in swine CL does not directly correspond with intraluteal level of PGE2 due to its transport to ovary from conceptuses and the uterus, in order to rescue luteal function during the maternal recognition of pregnancy [73]. We observed 7.3-fold upregulation of PKIB. The protein encoded by this gene is an inhibitor of PKA enzymes family involved in the transduction of signals induced among others by PGE2. This observation may be a direct symptom of a strong influence of CHEM on PGE2 generation by porcine LC.
Programmed death of LC is one of the integral elements of CL lifespan and is directly related to the process of structural regression of CL [74]. During this research, we noticed increased expression of genes encoding apoptosis initiator caspase (CASP10 (FC = 1.6)) and executioner caspases (CASP3 (FC = 1.4) and CASP7 (FC = 1.6)) in samples treated with CHEM, which usually indicates the beginning of apoptotic processes in the studied cells. Increased quantity of produced CASP3 protein or mRNA, a key executioner protease, could indicate an ongoing process of cellular apoptosis by both intrinsic and extrinsic pathways, which has been observed under the influence of CHEM in the ovarian cells of other mammals [7,14,15]. Validation of RNA-Seq results by qPCR confirmed a tendency to increase the quantity of CASP3 mRNA produced in CHEM-treated samples in comparison to control samples. Due to the fact that obtained p-value was just above the assumed threshold of statistical significance, such a result cannot be considered as conclusive. Encoded by upregulated BAK1 (FC = 1.7) and PMAIP1 (also named Noxa protein; FC = 2.1) genes pro-apoptotic proteins, belonging to BCL2 family members, may form specific, for intrinsic apoptosis mitochondrial membrane, ‘permeability transition pores’ [75]. These pores may enable exit from mitochondria to cytosol molecules, that induce DNA defragmentation, formation of apoptosomes activating CASP9 (which in turn triggers CASP3), and formation of complexes suppressing the activity of apoptosis inhibitory proteins [74,76].
Nonetheless, cellular mechanisms to counteract programmed cell death are also significantly strengthened, as can be seen from the increase in the amount of produced CFLAR (also named C-FLIP; FC = 1.6), MCL1, CIAP2 mRNAs. C-FLIP protein binding FADD and CASP8 and/or CASP10 proteins prevents formation and activation of the caspase cascade [77]. Long isoforms of MCL1 protein are able to bind many proteins from the BCL2 family, preventing the formation of mitochondrial ‘permeability transition pores’. The CIAP2 protein has the ability to regulate apoptosis by binding caspases, but also to modulate inflammatory signaling by ubiquitination of proteins involved in the NF-κB signal pathway [78]. Gene encoding PFKFB3 protein was 2.5-fold upregulated in CHEM-treated samples. This gene acts as a regulator of glucose metabolism within cells and has been associated with prevention of apoptosis [79]. Modifications of expression of the genes mentioned in this paragraph, induced by CHEM treatment on the mid-luteal LC, suggest that despite the occurrence of strong pro-apoptotic signals in cells there are also parallel mechanisms of opposite effect—pro-survival. We assume that despite the visible preparation of LC for programmed death, a multitude of anti-apoptotic processes inhibit the action of executive factors. It is possible that this phenomenon is directly related to the phase of the estrous cycle and the lack of fully developed luteolytic activity by the cells.

5. Conclusions

This study was the first experiment to demonstrate the impact of CHEM on the transcriptome profile of porcine LC during the mid-luteal phase of the estrous cycle. During this study we showed, for the first time, the impact of CHEM on NF-κB and JAK/STAT signal transduction pathways in mammalian LC. We observed changes in expression of apoptosis-associated genes which products may in a cell-specific manner affect the activation of both pro-survival and pro-apoptotic signaling pathways.
It is highly probable that CHEM at the physiological concentration may influence the sophisticated metabolic processes associated with gilt reproduction by regulation of P4 generation, increased production of pro-inflammatory factors, and preparation for luteal regression. As a result, deregulation of the ovarian–uterine interactions may result in prevention of embryo implantation, loss of pregnancy, or significant reduction in fertility. This research may be a prelude to further studies of the effect of CHEM on the swine reproductive system, as an important farm animal and as a model organism with a physiology like that of humans.

Supplementary Materials

The following are available online at https://www.mdpi.com/2073-4425/11/6/651/s1, Table S1: Differentially expressed protein coding genes identified in porcine luteal cells after in vitro chemerin treatment, Figure S1: TNF signaling pathway with mapped expression data, Figure S2: Cytokine–cytokine receptor interaction with mapped expression data, Figure S3: NF-kappa B signaling pathway with mapped expression data, Figure S4: Chemokine signaling pathway with mapped expression data, Figure S5: MAPK signaling pathway with mapped expression data, Figure S6: Cell adhesion molecules with mapped expression data, Figure S7: Apoptosis pathways with mapped expression data, Figure S8: Steroid hormone biosynthesis pathways with mapped expression data, Figure S9: Ovarian steroidogenesis pathways with mapped expression data, Figure S10: Arachidonic acid metabolism pathway with mapped expression data, Figure S11: JAK/STAT signaling pathway with mapped expression data

Author Contributions

Conceptualization: N.S., T.K.; methodology, K.G.M., N.S., L.P., M.K., K.D., E.R., and B.K.; software, K.G.M., J.P.J. and L.P.; validation, K.S.; formal analysis, K.G.M., E.R., M.K. and K.D.; investigation, K.G.M., N.S., M.K. and K.D.; resources, K.G.M., L.P., M.K., K.D., E.R., and B.K.; data curation, K.G.M., J.P.J., L.P. and E.R.; writing—original draft preparation, K.G.M.; writing—review and editing, K.G.M., T.K., N.S., and J.P.J.; supervision, T.K. and J.P.J.; project administration, N.S., T.K.; funding acquisition, N.S., T.K. All authors have read and agreed to the published version of the manuscript.

Funding

This research was supported by the National Science Centre (Project no.: 2015/17/B/NZ9/03595).

Conflicts of Interest

The authors declare no conflict of interest regarding the publication of this paper.

References

  1. Nagpal, S.; Patel, S.; Jacobe, H.; Disepio, D.; Ghosn, C.; Malhotra, M.; Teng, M.; Duvic, M.; Chandraratna, R.A. Tazarotene-induced Gene 2 (TIG2), a Novel Retinoid-Responsive Gene in Skin. J. Investig. Dermatol. 1997, 109, 91–95. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  2. Reverchon, M.; Cornuau, M.; Rame, C.; Guerif, F.; Royère, D.; Dupont, J. Chemerin inhibits IGF-1-induced progesterone and estradiol secretion in human granulosa cells. Hum. Reprod. 2012, 27, 1790–1800. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  3. Goralski, K.B.; McCarthy, T.C.; Hanniman, E.A.; Zabel, B.A.; Butcher, E.C.; Parlee, S.D.; Muruganandan, S.; Sinal, C.J. Chemerin, a Novel Adipokine That Regulates Adipogenesis and Adipocyte Metabolism. J. Boil. Chem. 2007, 282, 28175–28188. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  4. Wang, Q.; Kim, J.Y.; Xue, K.; Liu, J.-Y.; Leader, A.; Tsang, B.K. Chemerin, a Novel Regulator of Follicular Steroidogenesis and Its Potential Involvement in Polycystic Ovarian Syndrome. Endocrinology 2012, 153, 5600–5611. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  5. Du, X.-Y.; Leung, L.L. Proteolytic regulatory mechanism of chemerin bioactivity. Acta Biochim. Biophys. Sin. 2009, 41, 973–979. [Google Scholar] [CrossRef] [Green Version]
  6. De Henau, O.; De Groot, G.-N.; Imbault, V.; Robert, V.; De Poorter, C.; Mcheik, S.; Gales, C.; Parmentier, M.; Springael, J.-Y. Signaling Properties of Chemerin Receptors CMKLR1, GPR1 and CCRL2. PLoS ONE 2016, 11, e0164179. [Google Scholar] [CrossRef]
  7. Yang, Y.-L.; Ren, L.-R.; Sun, L.-F.; Huang, C.; Xiao, T.-X.; Wang, B.-B.; Chen, J.; Zabel, B.A.; Ren, P.; Zhang, J. The role of GPR1 signaling in mice corpus luteum. J. Endocrinol. 2016, 230, 55–65. [Google Scholar] [CrossRef] [Green Version]
  8. Monnier, J.; Lewén, S.; O’Hara, E.; Huang, K.; Tu, H.; Butcher, E.C.; Zabel, B.A. Expression, regulation, and function of atypical chemerin receptor CCRL2 on endothelial cells. J. Immunol. 2012, 189, 956–967. [Google Scholar] [CrossRef] [Green Version]
  9. Mazzotti, C.; Gagliostro, V.; Bosisio, D.; Del Prete, A.; Tiberio, L.; Thelen, M.; Sozzani, S. The Atypical Receptor CCRL2 (C-C Chemokine Receptor-Like 2) Does Not Act as a Decoy Receptor in Endothelial Cells. Front. Immunol. 2017, 8. [Google Scholar] [CrossRef] [Green Version]
  10. Mazaki-Tovi, S.; Kasher-Meron, M.; Hemi, R.; Haas, J.; Gat, I.; Lantsberg, D.; Hendler, I.; Kanety, H. Chemerin is present in human cord blood and is positively correlated with birthweight. Am. J. Obstet. Gynecol. 2012, 207, 412.e1–412.e10. [Google Scholar] [CrossRef]
  11. Garces, M.; Sánchez, E.; Acosta, B.; Angel, E.; Ruiz, A.; Rubio-Romero, J.; Diéguez, C.; Nogueiras, R.; Caminos, J. Expression and regulation of chemerin during rat pregnancy. Placenta 2012, 33, 373–378. [Google Scholar] [CrossRef] [PubMed]
  12. Reverchon, M.; Bertoldo, M.J.; Ramé, C.; Froment, P.; Dupont, J. CHEMERIN (RARRES2) Decreases In Vitro Granulosa Cell Steroidogenesis and Blocks Oocyte Meiotic Progression in Bovine Species1. Boil. Reprod. 2014, 90, 102. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  13. Margioris, A.N.; Katrinaki, M.; Tsatsanis, C.; Giwercman, A.; Bobjer, J.; Dermitzaki, E.; Katrinaki, M.; Dermitzaki, E.; Margioris, A.N.; Giwercman, A.; et al. Serum chemerin levels are negatively associated with male fertility and reproductive hormones. Hum. Reprod. 2018, 33, 2168–2174. [Google Scholar]
  14. Yao, J.; Li, Z.; Fu, Y.; Wu, R.; Wang, Y.; Liu, C.; Yang, L.; Zhang, H.-W. Involvement of obesity-associated upregulation of chemerin/chemokine-like receptor 1 in oxidative stress and apoptosis in ovaries and granulosa cells. Biochem. Biophys. Res. Commun. 2019, 510, 449–455. [Google Scholar] [CrossRef]
  15. Kim, J.Y.; Xue, K.; Cao, M.; Wang, Q.; Liu, J.-Y.; Leader, A.; Han, J.Y.; Tsang, B.K. Chemerin Suppresses Ovarian Follicular Development and Its Potential Involvement in Follicular Arrest in Rats Treated Chronically With Dihydrotestosterone. Endocrinology 2013, 154, 2912–2923. [Google Scholar] [CrossRef] [Green Version]
  16. Smolinska, N.; Kiezun, M.; Dobrzyn, K.; Rytelewska, E.; Kisielewska, K.; Gudelska, M.; Zaobidna, E.; Bogus-Nowakowska, K.; Wyrebek, J.; Bors, K.; et al. Expression of Chemerin and Its Receptors in the Porcine Hypothalamus and Plasma Chemerin Levels during the Oestrous Cycle and Early Pregnancy. Int. J. Mol. Sci. 2019, 20, 3887. [Google Scholar] [CrossRef] [Green Version]
  17. Rytelewska, E.; Kisielewska, K.; Kiezun, M.; Dobrzyn, K.; Gudelska, M.; Rak-Mardyla, A.; Dupont, J.; Kaminska, B.; Kaminski, T.; Smolinska, N. Expression of chemerin and its receptors in the ovaries of prepubertal and mature gilts. Mol. Reprod. Dev. 2020. accepted. [Google Scholar] [CrossRef]
  18. Akins, E.L.; Morrissette, M.C. Gross ovarian changes during estrous cycle of swine. Am. J. Veter Res. 1968, 29. [Google Scholar]
  19. Kaminski, T.; Siawrys, G.; Okrasa, S.; Przala, J. Action of the opioid agonist FK 33-824 on porcine small and large luteal cells from the mid-luteal phase: Effect on progesterone, cAMP, cGMP and inositol phosphate release. Anim. Reprod. Sci. 1999, 56, 245–257. [Google Scholar] [CrossRef]
  20. Bozaoglu, K.; Curran, J.E.; Stocker, C.J.; Zaibi, M.S.; Segal, D.; Konstantopoulos, N.; Morrison, S.; Carless, M.; Dyer, T.D.; Cole, S.A.; et al. Chemerin, a novel adipokine in the regulation of angiogenesis. J. Clin. Endocrinol. Metab. 2010, 95, 2476–2485. [Google Scholar] [CrossRef] [Green Version]
  21. Shen, Y.; Mao, H.; Huang, M.; Chen, L.; Chen, J.; Cai, Z.; Wang, Y.; Xu, N. Long Noncoding RNA and mRNA Expression Profiles in the Thyroid Gland of Two Phenotypically Extreme Pig Breeds Using Ribo-Zero RNA Sequencing. Genes 2016, 7, 34. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  22. Pertea, M.; Kim, D.; Pertea, G.M.; Leek, J.T.; Salzberg, S.L. Transcript-level expression analysis of RNA-seq experiments with HISAT, StringTie and Ballgown. Nat. Protoc. 2016, 11, 1650–1667. [Google Scholar] [CrossRef] [PubMed]
  23. Andrews, S. FastQC: A Quality Control Tool for High Throughput Sequence Data. Available online: http://www.bioinformatics.babraham.ac.uk/projects/fastqc (accessed on 10 June 2020).
  24. Bolger, A.M.; Lohse, M.; Usadel, B. Trimmomatic: A flexible trimmer for Illumina sequence data. Bioinformatics 2014, 30, 2114–2120. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  25. Dobin, A.; Davis, C.A.; Schlesinger, F.; Drenkow, J.; Zaleski, C.; Jha, S.; Batut, P.; Chaisson, M.; Gingeras, T.R. STAR: Ultrafast universal RNA-seq aligner. Bioinformatics 2012, 29, 15–21. [Google Scholar] [CrossRef]
  26. Zerbino, D.R.; Achuthan, P.; Akanni, W.; Amode, M.R.; Barrell, D.; Bhai, J.; Billis, K.; Cummins, C.; Gall, A.; Girón, C.G.; et al. Ensembl 2018. Nucleic Acids Res. 2018, 46, 754–761. [Google Scholar] [CrossRef]
  27. Broad Institute. Picard Tools. Available online: http://broadinstitute.github.io/picard/ (accessed on 10 June 2020).
  28. Wickham, H. ggplot2: Elegant Graphics for Data Analysis; Springer: New York, NY, USA, 2016; ISBN 978-3-319-24277-4. [Google Scholar]
  29. Paukszto, L.; Mikolajczyk, A.; Szeszko, K.; Smolinska, N.; Jastrzebski, J.P.; Kaminski, T. Transcription analysis of the response of the porcine adrenal cortex to a single subclinical dose of lipopolysaccharide from Salmonella Enteritidis. Int. J. Boil. Macromol. 2019, 141, 1228–1245. [Google Scholar] [CrossRef]
  30. Pertea, M.; Pertea, G.M.; Antonescu, C.M.; Chang, T.-C.; Mendell, J.T.; Salzberg, S.L. StringTie enables improved reconstruction of a transcriptome from RNA-seq reads. Nat. Biotechnol. 2015, 33, 290–295. [Google Scholar] [CrossRef] [Green Version]
  31. Frazee, A.C.; Pertea, G.; Jaffe, A.E.; Langmead, B.; Salzberg, S.L.; Leek, J.T. Flexible analysis of transcriptome assemblies with Ballgown. BioRxiv 2014, 003665. [Google Scholar]
  32. Ramos, M.; Schiffer, L.; Re, A.; Azhar, R.; Basunia, A.; Rodriguez, C.; Chan, T.; Chapman, P.; Davis, S.R.; Gomez-Cabrero, D.; et al. Software for the Integration of Multiomics Experiments in Bioconductor. Cancer Res. 2017, 77, e39–e42. [Google Scholar] [CrossRef] [Green Version]
  33. Ihaka, R.; Gentleman, R.R. A Language for Data Analysis and Graphics. J. Comput. Graph. Stat. 1996, 5, 299–314. [Google Scholar]
  34. Reimand, J.; Arak, T.; Adler, P.; Kolberg, L.; Reisberg, S.; Peterson, H.; Vilo, J. g: Profiler-a web server for functional interpretation of gene lists (2016 update). Nucleic Acids Res. 2016, 44, 83–89. [Google Scholar] [CrossRef] [PubMed]
  35. Wu, J.; Mao, X.; Cai, T.; Luo, J.; Wei, L. KOBAS server: A web-based platform for automated annotation and pathway identification. Nucleic Acids Res. 2006, 34, 720–724. [Google Scholar] [CrossRef] [PubMed]
  36. Kanehisa, M.; Furumichi, M.; Tanabe, M.; Sato, Y.; Morishima, K. KEGG: New perspectives on genomes, pathways, diseases and drugs. Nucleic Acids Res. 2016, 45, 353–361. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  37. Ashburner, M.; Ball, C.A.; A Blake, J.; Botstein, D.; Butler, H.; Cherry, J.M.; Davis, A.P.; Dolinski, K.; Dwight, S.S.; Eppig, J.T.; et al. Gene Ontology: Tool for the unification of biology. Nat. Genet. 2000, 25, 25–29. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  38. The Gene Ontology Consortium. Expansion of the Gene Ontology knowledgebase and resources. Nucleic Acids Res. 2016, 45, D331–D338. [Google Scholar] [CrossRef] [Green Version]
  39. Fabregat, A.; Jupe, S.; Matthews, L.; Sidiropoulos, K.; Gillespie, M.; Garapati, P.; Haw, R.; Jassal, B.; Korninger, F.; May, B.; et al. The Reactome Pathway Knowledgebase. Nucleic Acids Res. 2018, 46, D649–D655. [Google Scholar] [CrossRef]
  40. Livak, K.J.; Schmittgen, T.D. Analysis of Relative Gene Expression Data Using Real-Time Quantitative PCR and the 2−ΔΔCT Method. Methods 2001, 25, 402–408. [Google Scholar] [CrossRef]
  41. Spagnuolo-Weaver, M.; Fuerst, R.; Campbell, S.T.; Meehan, B.M.; McNeilly, F.; Adair, B.; Allan, G. A fluorimeter-based RT-PCR method for the detection and quantitation of porcine cytokines. J. Immunol. Methods 1999, 230, 19–27. [Google Scholar] [CrossRef]
  42. Nitkiewicz, A.; Smolinska, N.; Przala, J.; Kaminski, T. Expression of orexin receptors 1 (OX1R) and 2 (OX2R) in the porcine ovary during the oestrous cycle. Regul. Pept. 2010, 165, 186–190. [Google Scholar] [CrossRef]
  43. Li, X.; Zhu, Q.; Wang, W.; Qi, J.; He, Y.; Wang, Y.; Lu, Y.; Wu, H.; Ding, Y.; Sun, Y. Elevated Chemerin Induces Insulin Resistance in Human Granulosa-Lutein Cells from Polycystic Ovary Syndrome Patients. SSRN Electron. J. 2018. [Google Scholar] [CrossRef]
  44. Wang, Q.; Leader, A.; Tsang, B.K. Inhibitory Roles of Prohibitin and Chemerin in FSH-Induced Rat Granulosa Cell Steroidogenesis. Endocrinology 2013, 154, 956–967. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  45. Abreu, R.D.S.; Penalva, L.O.; Salemi, M.; Vogel, C. Global signatures of protein and mRNA expression levels. Mol. BioSyst. 2009, 5, 1512–1526. [Google Scholar] [CrossRef] [Green Version]
  46. Schwanhäusser, B.; Busse, D.; Li, N.; Dittmar, G.; Schuchhardt, J.; Wolf, J.; Chen, W.; Selbach, M. Global quantification of mammalian gene expression control. Nature 2011, 473, 337–342. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  47. Li, J.J.; Bickel, P.J.; Biggin, M.D. System wide analyses have underestimated protein abundances and the importance of transcription in mammals. Peer J. 2014, 2, e270. [Google Scholar] [CrossRef] [Green Version]
  48. Lawrence, T. The Nuclear Factor NF-kB Pathway in Inflammation. Cold Spring Harb. Perspect. Biol. 2009, 1, a001651. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  49. Zmijewska, A.; Franczak, A.; Kotwica, G. Role of interleukin-1β in the regulation of porcine corpora lutea during the late luteal phase of the cycle and during pregnancy. Acta Veter Hung. 2012, 60, 395–407. [Google Scholar] [CrossRef] [Green Version]
  50. Lin, S.-C.; Lo, Y.-C.; Wu, H. Helical assembly in the MyD88–IRAK4–IRAK2 complex in TLR/IL-1R signalling. Nature 2010, 465, 885–890. [Google Scholar] [CrossRef] [Green Version]
  51. Xia, Y.; Chen, S.; Wang, Y.; Mackman, N.; Ku, G.; Lo, D.; Feng, L. RelB Modulation of IκBα Stability as a Mechanism of Transcription Suppression of Interleukin-1α (IL-1α), IL-1β, and Tumor Necrosis Factor Alpha in Fibroblasts. Mol. Cell. Boil. 1999, 19, 7688–7696. [Google Scholar] [CrossRef] [Green Version]
  52. Hayden, M.; West, A.P.; Ghosh, S. NF-κB and the immune response. Oncogene 2006, 25, 6758–6780. [Google Scholar] [CrossRef] [Green Version]
  53. Luo, W.; Diaz, F.J.; Wiltbank, M.C. Induction of mRNA for chemokines and chemokine receptors by prostaglandin F2α is dependent upon stage of the porcine corpus luteum and intraluteal progesterone. Endocrinology 2011, 152, 2797–2805. [Google Scholar] [CrossRef] [Green Version]
  54. Przygrodzka, E.; Kaczmarek, M.M.; Kaczyński, P.; Ziecik, A.J.; Ski, P.K. Steroid hormones, prostanoids, and angiogenic systems during rescue of the corpus luteum in pigs. Reproduction 2016, 151, 135–147. [Google Scholar] [CrossRef] [PubMed]
  55. Vince, J.E.; Pantaki, D.; Feltham, R.; Mace, P.D.; Cordier, S.M.; Schmukle, A.C.; Davidson, A.J.; Callus, B.A.; Wong, W.W.-L.; E Gentle, I.; et al. TRAF2 Must Bind to Cellular Inhibitors of Apoptosis for Tumor Necrosis Factor (TNF) to Efficiently Activate NF-κB and to Prevent TNF-induced Apoptosis. J. Boil. Chem. 2009, 284, 35906–35915. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  56. Rawlings, J.S.; Rosler, K.M.; Harrison, D. The JAK/STAT signaling pathway. J. Cell Sci. 2004, 117, 1281–1283. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  57. Heinrich, P.C.; Behrmann, I.; Haan, S.; Hermanns, H.M.; Müller-Newen, G.; Schaper, F. Principles of interleukin (IL)-6-type cytokine signalling and its regulation. Biochem. J. 2003, 374, 1–20. [Google Scholar] [CrossRef] [Green Version]
  58. Kumar, A.; Commane, M.; Flickinger, T.W.; Horvath, C.M.; Stark, G.R. Defective TNF-α-Induced Apoptosis in STAT1-Null Cells Due to Low Constitutive Levels of Caspases. Science 1997, 278, 1630–1632. [Google Scholar] [CrossRef]
  59. Kaplan, D.H.; Shankaran, V.; Dighe, A.S.; Stockert, E.; Aguet, M.; Old, L.J.; Schreiber, R.D. Demonstration of an interferon γ-dependent tumor surveillance system in immunocompetent mice. Proc. Natl. Acad. Sci. USA 1998, 95, 7556–7561. [Google Scholar] [CrossRef] [Green Version]
  60. Tsuji, Y.; Adachi, S.; Iemoto, A.; Hasegawa, A.; Koyama, K.; Tamaoki, T.H.; Kashiwamura, S.-I.; Ueda, H.; Muranaka, J.; Furuyama, J.-I.; et al. Expression of interleukin-18 and its receptor in mouse ovary. Am. J. Reprod. Immunol. 2001, 46, 349–357. [Google Scholar] [CrossRef]
  61. Prakash, B.S.; Pedina, J.; Steiner, A.; Wuttke, W. Demonstration of luteotrophic responses of human recombinant γ interferon in porcine corpora lutea using an in-vivo microdialysis system. J. Steroid Biochem. Mol. Biol. 1997, 63, 189–194. [Google Scholar] [CrossRef]
  62. Przygrodzka, E.; Witek, K.J.; Kaczmarek, M.M.; Andronowska, A.; Ziecik, A.J. Expression of factors associated with apoptosis in the porcine corpus luteum throughout the luteal phase of the estrous cycle and early pregnancy: Their possible involvement in acquisition of luteolytic sensitivity. Theriogenology 2015, 83, 535–545. [Google Scholar] [CrossRef]
  63. Rytelewska, E.; Kiezun, M.; Kisielewska, K.; Gudelska, M.; Dobrzyn, K.; Kaminska, B.; Kaminski, T.; Smolinska, N. Chemerin as a modulator of ovarian steroidogenesis in pigs: An in vitro study. Theriogenology. under review.
  64. Ruiz de Galarreta, C.M.; Fanjul, L.F.; Hsueh, A.J.W. Progestin regulation of progesterone biosynthetic enzymes in cultured rat granulosa cells. Steroids 1985, 46, 987–1002. [Google Scholar] [CrossRef]
  65. Tanaka, N.; Iwamasa, J.; Matsuura, K.; Okamura, H. Effects of progesterone and anti-progesterone RU486 on ovarian 3β-hydroxysteroid dehydrogenase activity during ovulation in the gonadotrophin-primed immature rat. J. Reprod. Fertil. 1993, 97, 167–172. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  66. Ruiz de Galarreta, C.M.; Fanjul, L.F.; Meidan, R.; Hsueh, A.J.W. Regulation of 3β-hydroxysteroid dehydrogenase activity by human chorionic gonadotropin, androgens, and anti-androgens in cultured testicular cells. J. Biol. Chem. 1983, 438, 663–665. [Google Scholar] [CrossRef]
  67. Fanjul, L.F.; Quintana, J.; González, J.; Santana-Delgado, P.; Estévez, F.; De Galarreta, C.M.R. Testicular 3β-hydroxysteroid dehydrogenase/Δ5–4 isomerase in the hypophysectomized rat: Effect of treatment with 5α-dihydrotestosterone. J. Endocrinol. 1992, 133, 237–243. [Google Scholar] [CrossRef] [PubMed]
  68. Park, J.Y.; Pillinger, M.H.; Abramson, S.B. Prostaglandin E2 synthesis and secretion: The role of PGE2 synthases. Clin. Immunol. 2006, 119, 229–240. [Google Scholar] [CrossRef]
  69. Kim, S.O.; Harris, S.M.; Duffy, D.M. Prostaglandin E2 (EP) receptors mediate PGE2-specific events in ovulation and luteinization within primate ovarian follicles. Endocrinology 2014, 155, 1466–1475. [Google Scholar] [CrossRef]
  70. Li, X.M. Prostaglandins alter the abundance of messenger ribonucleic acid for steroidogenic enzymes in cultured porcine granulosa cells. Boil. Reprod. 1993, 48, 1360–1366. [Google Scholar] [CrossRef]
  71. Wiesak, T.; Hunter, M.G.; Foxcroft, G.R. Effect of prostaglandins on luteal function during early pregnancy in pigs. Reproduction 1992, 95, 831–840. [Google Scholar] [CrossRef] [Green Version]
  72. Jimbo, K.; Park, J.S.; Yokosuka, K.; Sato, K.; Nagata, K. Positive feedback loop of interleukin-1β upregulating production of inflammatory mediators in human intervertebral disc cells in vitro. J. Neurosurg. Spine 2005, 2, 589–595. [Google Scholar] [CrossRef]
  73. Ziecik, A.J.; Przygrodzka, E.; Kaczmarek, M.M. Corpus Luteum Regression and Early Pregnancy Maintenance in Pigs. In The Life Cycle of the Corpus Luteum; Springer International Publishing: Cham, Switzerland, 2017; pp. 227–248. ISBN 9783319432380. [Google Scholar]
  74. Maekawa, R.; Okuda, K. Species-related differences in the mechanism of apoptosis during structural luteolysis. J. Reprod. Dev. 2007, 53, 977–986. [Google Scholar] [CrossRef] [Green Version]
  75. Levine, B.; Sinha, S.C.; Kroemer, G. Bcl-2 family members: Dual regulators of apoptosis and autophagy. Autophagy 2008, 4, 600–606. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  76. Lavitrano, M.; Barazzoni, A.; Forni, M.; Costerbosa, G.L. In situ detection of apoptosis in regressing corpus luteum of pregnant sow: Evidence of an early presence of DNA fragmentation. Domest. Anim. Endocrinol. 1996, 13, 361–372. [Google Scholar] [CrossRef]
  77. Safa, A.R. Roles of c-FLIP in Apoptosis, Necroptosis, and Autophagy. J. Carcinog. Mutagen. 2013, 4, 1–10. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  78. Graber, T.E.; Holcik, M. Distinct roles for the cellular inhibitors of apoptosis proteins 1 and 2. Cell Death Dis. 2011, 2, e135. [Google Scholar] [CrossRef]
  79. Yalcin, A.; Clem, B.F.; Imbert-Fernandez, Y.; Ozcan, S.C.; Peker, S.; O’Neal, J.; Klarer, A.C.; Clem, A.L.; Telang, S.; Chesney, J. 6-Phosphofructo-2-kinase (PFKFB3) promotes cell cycle progression and suppresses apoptosis via Cdk1-mediated phosphorylation of p27. Cell Death Dis. 2014, 5, e1337. [Google Scholar] [CrossRef] [PubMed]
Genes 11 00651 g001 550
Figure 1. The course of in silico analyses. In the flowchart, blue blocks indicate used bioinformatic software, grey blocks represent databases (including the source of raw reads). Orange blocks symbolize input and output files necessary to run subsequent programs or tools. Green rectangles represent the result files that are the main effect of the entire data pipeline, which contain differentially expressed genes (DEGs). The red diamond symbolizes the decision-making process. Continuous arrows indicate the main direction of data flow, while intermittent arrows indicate the indirect influence on the analysis process.
Figure 1. The course of in silico analyses. In the flowchart, blue blocks indicate used bioinformatic software, grey blocks represent databases (including the source of raw reads). Orange blocks symbolize input and output files necessary to run subsequent programs or tools. Green rectangles represent the result files that are the main effect of the entire data pipeline, which contain differentially expressed genes (DEGs). The red diamond symbolizes the decision-making process. Continuous arrows indicate the main direction of data flow, while intermittent arrows indicate the indirect influence on the analysis process.
Genes 11 00651 g001
Genes 11 00651 g002 550
Figure 2. Percentage (%) of bases mapped to specific components of the pig reference genome among all samples: coding regions (CDS), untranslated regions (UTRs), intronic and intergenic regions.
Figure 2. Percentage (%) of bases mapped to specific components of the pig reference genome among all samples: coding regions (CDS), untranslated regions (UTRs), intronic and intergenic regions.
Genes 11 00651 g002
Genes 11 00651 g003 550
Figure 3. (A) Principal component analysis (PCA) of all differentially expressed genes. PCA plot was generated using the ggplot2 R library. (B) Sample-to-sample distance matrix. The color intensity means the distance, where dark blue is the lowest distance (the diagonal squares have distance 0) and the light blue (almost white) means high Euclidean distance. Heatmap showing the Euclidean distances between the samples was generated with use of the DESeq2 package.
Figure 3. (A) Principal component analysis (PCA) of all differentially expressed genes. PCA plot was generated using the ggplot2 R library. (B) Sample-to-sample distance matrix. The color intensity means the distance, where dark blue is the lowest distance (the diagonal squares have distance 0) and the light blue (almost white) means high Euclidean distance. Heatmap showing the Euclidean distances between the samples was generated with use of the DESeq2 package.
Genes 11 00651 g003
Genes 11 00651 g004 550
Figure 4. (A) MA plot shows the logarithmic values of fold changes (Y axis) and mean of logarithmic (fragments per kilobase per million reads mapped (FPKM) + 1) values (X axis) for comparing CHEM-treated and control libraries. (B) Volcano plot presents the logarithmic values of fold changes (X axis) plotted against negative logarithmic q-values (Y axis). On both plots each point is defaultly colored black, red dots represent differentially expressed genes (DEGs) upregulated under the CHEM treatment and green dots show downregulated DEGs with significant q-value < 0.05. Triangles symbolize DEGs above the visible range, and rhomboids symbolize DEGs to the right of the visible range. Purple dashed lines symbolize cut-off levels.
Figure 4. (A) MA plot shows the logarithmic values of fold changes (Y axis) and mean of logarithmic (fragments per kilobase per million reads mapped (FPKM) + 1) values (X axis) for comparing CHEM-treated and control libraries. (B) Volcano plot presents the logarithmic values of fold changes (X axis) plotted against negative logarithmic q-values (Y axis). On both plots each point is defaultly colored black, red dots represent differentially expressed genes (DEGs) upregulated under the CHEM treatment and green dots show downregulated DEGs with significant q-value < 0.05. Triangles symbolize DEGs above the visible range, and rhomboids symbolize DEGs to the right of the visible range. Purple dashed lines symbolize cut-off levels.
Genes 11 00651 g004
Genes 11 00651 g005 550
Figure 5. Heatmap of expression data for 98 differentially expressed genes and their participation in metabolic pathways from the Kyoto Encyclopedia of Genes and Genomes (KEGG) database. Genes were ordered according to the dendrogram (not shown) of similarity of their expression profiles calculated on the basis of the respective Z-scores. Samples marked with CTRL belong to the control group, while CHEM were treated with chemerin.
Figure 5. Heatmap of expression data for 98 differentially expressed genes and their participation in metabolic pathways from the Kyoto Encyclopedia of Genes and Genomes (KEGG) database. Genes were ordered according to the dendrogram (not shown) of similarity of their expression profiles calculated on the basis of the respective Z-scores. Samples marked with CTRL belong to the control group, while CHEM were treated with chemerin.
Genes 11 00651 g005
Genes 11 00651 g006 550
Figure 6. Lollipop chart with 15 best (with lowest p-value) Gene Ontology (GO) terms for every GO aspect (Biological Process—BP, Cellular Component—CC, Molecular Function—MF), sorted due to descending negative logarithmic adjusted p-value of enrichment analysis. Numbers in circles represent the number of differentially expressed genes matched to a specific term.
Figure 6. Lollipop chart with 15 best (with lowest p-value) Gene Ontology (GO) terms for every GO aspect (Biological Process—BP, Cellular Component—CC, Molecular Function—MF), sorted due to descending negative logarithmic adjusted p-value of enrichment analysis. Numbers in circles represent the number of differentially expressed genes matched to a specific term.
Genes 11 00651 g006
Genes 11 00651 g007 550
Figure 7. Quantitative real-time PCR validations of RNA-Seq results performed for selected differentially expressed genes—interleukin 1β (IL1B), prostaglandin-endoperoxide synthase 2 (PTGS2), hydroxy-δ-5-steroid dehydrogenase, 3 β- and steroid δ-isomerase 7 (HSD3B7) and caspase 3 (CASP3). Above the bars, precise p-values obtained from statistical analysis of the results are written. CTRL is a control group and CHEM is a chemerin-treated group.
Figure 7. Quantitative real-time PCR validations of RNA-Seq results performed for selected differentially expressed genes—interleukin 1β (IL1B), prostaglandin-endoperoxide synthase 2 (PTGS2), hydroxy-δ-5-steroid dehydrogenase, 3 β- and steroid δ-isomerase 7 (HSD3B7) and caspase 3 (CASP3). Above the bars, precise p-values obtained from statistical analysis of the results are written. CTRL is a control group and CHEM is a chemerin-treated group.
Genes 11 00651 g007
Table
Table 1. Primers used for the validation of RNA-Seq results.
Table 1. Primers used for the validation of RNA-Seq results.
Gene SymbolGene DescriptionPrimers SequencesProduct LengthReference
IL1BInterleukin 1βF: TTTGAAGAAGAGCCCATCATCC
R: CCAGCCAGCACTAGAGATTTG		119 bp[The present study]
CASP3Caspase 3F: GTGCTTCTAAGCCATGGTGAA
R: CGGCAGGCCTGAATTATGAA		143 bp[The present study]
PTGS2Prostaglandin-endoperoxide synthase 2F: ATGGGTGTGAAAGGGAGGAAA
R: AAACTGATGGGTGAAGTGCTG		141 bp[The present study]
HSD3B7Hydroxy-δ-5-steroid dehydrogenase, 3 β- and steroid δ-isomerase 7F: CTCGAAGCCAACGGAAGGA
R: CCACGTTACCCACGTAGACC		193 bp[The present study]
ACTBβ-actinF: ACATCAAGGAGAAGCTCTGCTACG
R: GAGGGGCGATGATCTTGATCTTCA		366 bp[41]
GAPDHGlyceraldehyde-3- phosphate dehydrogenaseF: CCTTCATTGACCTCCACTACATGG
R: CCACAACATACGTAGCACCAGCATC		183 bp[42]
Abbreviations: F—forward; R—reverse.
Table
Table 2. Summary of the results of RNA sequencing, preprocessing and mapping of reads to the porcine reference genome. All numerical values are expressed in millions. CTRL are samples from control group, and CHEM are samples from chemerin-treated group.
Table 2. Summary of the results of RNA sequencing, preprocessing and mapping of reads to the porcine reference genome. All numerical values are expressed in millions. CTRL are samples from control group, and CHEM are samples from chemerin-treated group.
Treatment CTRL CHEM
Samples1_LC2_LC3_LC4_LC5_LC1_LC2_LC3_LC4_LC5_LC
Row reads110.458125.606121.017115.746108.415109.209115.928112.795122.503112.816
Processed reads97.605111.356106.973102.61196.01097.413102.89599.857109.165100.500
Mapped reads97.057110.805106.363102.00995.5496.93102.24499.362108.61399.97
Uniquely mapped94.274106.514102.76698.57792.28493.33799.2295.599104.36596.408
% of uniquely mapped97.13%96.13%96.62%96.64%96.59%96.29%97.04%96.21%96.09%96.44%
Multi-mapped2.7834.2913.5973.4323.2563.5933.0243.7634.2483.562

Share and Cite

MDPI and ACS Style

Makowczenko, K.G.; Jastrzebski, J.P.; Szeszko, K.; Smolinska, N.; Paukszto, L.; Dobrzyn, K.; Kiezun, M.; Rytelewska, E.; Kaminska, B.; Kaminski, T. Transcription Analysis of the Chemerin Impact on Gene Expression Profile in the Luteal Cells of Gilts. Genes 2020, 11, 651. https://doi.org/10.3390/genes11060651

AMA Style

Makowczenko KG, Jastrzebski JP, Szeszko K, Smolinska N, Paukszto L, Dobrzyn K, Kiezun M, Rytelewska E, Kaminska B, Kaminski T. Transcription Analysis of the Chemerin Impact on Gene Expression Profile in the Luteal Cells of Gilts. Genes. 2020; 11(6):651. https://doi.org/10.3390/genes11060651

Chicago/Turabian Style

Makowczenko, Karol G., Jan P. Jastrzebski, Karol Szeszko, Nina Smolinska, Lukasz Paukszto, Kamil Dobrzyn, Marta Kiezun, Edyta Rytelewska, Barbara Kaminska, and Tadeusz Kaminski. 2020. "Transcription Analysis of the Chemerin Impact on Gene Expression Profile in the Luteal Cells of Gilts" Genes 11, no. 6: 651. https://doi.org/10.3390/genes11060651

Note that from the first issue of 2016, this journal uses article numbers instead of page numbers. See further details here.

Article Metrics

Back to TopTop