Mengya Liang1†
Yi Zhang2†
Shuangjiao Gan2Yunqi Liu1
Huayang Li2
Quan Liu2Haoliang Liu2
Zhuoming Zhou2
Huawei Wu3Guangxian Chen1
Zhongkai Wu1*- 1Department of Cardiac Surgery, The First Affiliated Hospital, Sun Yat-Sen University, Guangzhou, China
- 2NHC Key Laboratory of Assisted Circulation, Sun Yat-Sen University, Guangzhou, China
- 3Department of Neurobiology, Physiology and Behavior, College of Biological Sciences, University of California, Davis, CA, United States
Long noncoding RNAs (lncRNAs) and microRNAs (miRNAs) are involved in the mechanism underlying cerebral dysfunction after deep hypothermic circulatory arrest (DHCA), although the exact details have not been elucidated. To explore the expression profiles of lncRNAs and miRNAs in DHCA cerebral injury, we determined the lncRNA, miRNA and mRNA expression profiles in the cerebral cortex of DHCA and sham rats. First, a rat model of DHCA was established, and high-throughput sequencing was performed to analyze the differentially expressed RNAs (DERNAs). Then, the principal functions of the significantly deregulated genes were identified using Gene Ontology (GO) and Kyoto Encyclopedia of Genes and Genomes (KEGG) pathway enrichment analyses. Expression networks (lncRNAs-miRNAs-mRNAs and transcription factors (TFs)-miRNAs-mRNAs) were also established. Finally, the expression of DERNAs was confirmed by quantitative real-time PCR (RT-qPCR). We identified 89 lncRNAs, 45 miRNAs and 59 mRNAs between the DHCA and sham groups and constructed a comprehensive competitive endogenous RNAs (ceRNAs) network. A TF-miRNA-mRNA regulatory network was also established. Finally, we predicted that Lcorl-miR-200a-3p-Ttr, BRD4-Ccl2 and Ep300-miR-200b-3p-Tmem72 may participate in the pathogenesis of DHCA cerebral injury.
1 Introduction
Deep hypothermia circulatory arrest (DHCA) surgery has been more widely used in clinical practice in recent decades (Griepp et al., 1975). Compared with cardiopulmonary bypass (CPB), DHCA reduces the core temperature to 18°C, which can reduce the body metabolic rate and tissue oxygen consumption and improve organ tolerance to ischemia, thereby substantially reducing the risk of surgery. Hence, DHCA has become an important manipulation during complex cardiac surgery, such as aortic arch surgery and complex congenital heart disease correction. However, because the brain is extremely sensitive to hypoxia and ischemia/reperfusion-induced pathological changes, neurological complications have become one of the major problems for surgeons to solve (Bartels et al., 2014; Cefarelli et al., 2017). Previous studies reported neurological dysfunction in 5.3–25% of patients after DHCA (Leshnower et al., 2010; Hu et al., 2014; Leshnower et al., 2015; Centofanti et al., 2016). In recent years, many studies have reported the effects of intraoperative cerebral perfusion strategies and temperature management for cerebral protection (Apostolakis and Shuhaiber, 2007; Fan et al., 2019); nevertheless, the mechanism of neurologic morbidities has not been fully elucidated, and further investigations are warranted.
Long noncoding RNAs (lncRNAs) are a class of RNAs whose length is greater than 200 nt, and they regulate a variety of biological processes at the transcriptional, posttranscriptional and epigenetic levels (Lalevée and Feil, 2015; Yu et al., 2018). Studies have reported that lncRNAs participate in multiple physiological functions, such as gene transcriptional regulation, chromatin modification, ontogenetic regulation, cell programming, and stem cell pluripotency maintenance in various ways (Clark et al., 2012). LncRNAs are specifically highly expressed in the central nervous system and regulate central nervous system development and neurodegenerative diseases (Ng et al., 2013). Studies have demonstrated that lncRNAs were differentially expressed in the ischemic brain after stroke, and that alteration to this expression was closely related with changes in gene expression, suggesting lncRNAs may regulate brain injury by altering the expressions of associated genes (Zhang et al., 2016; Liu et al., 2018). Feng et al. found that the expression of lncRNA ANRIL in patients with acute ischemic stroke (AIS) was lower than that in normal people, suggesting that ANRIL was closely related to the degree of cerebral inflammation after stroke (Feng et al., 2019). However, very few studies have reported the role of lncRNAs in DHCA.
MiRNAs are a class of ubiquitous, conserved, and endogenous noncoding single-stranded RNAs that are usually 19–25 nucleotides in length, and they specifically recognize and target mRNAs to promote their degradation and act as regulatory factors in the posttranscriptional stage of genes (Filipowicz et al., 2008; Zhang et al., 2019). An increasing number of noncoding RNAs have been found to be involved in physiological and pathological processes of the nervous system (Zhong et al., 2019). LncRNAs can serve as competitive endogenous RNAs (ceRNAs) to specifically bind with miRNAs, thus reducing mRNA degradation (Wang C. et al., 2020). For example, Gao’s group found that after DHCA, the lncRNA GAS5 was significantly increased in the hippocampus and could directly bind to miR-23a to promote the expression of the downstream PTEN gene. PTEN can decrease the levels of p-Akt and Bcl-2 through the dephosphorylation of PIP3, thereby inducing neuronal apoptosis (Gao et al., 2019). Ma et al. presented lncRNA-associated ceRNA profiles in an Alzheimer’s disease (AD) mouse brain and identified lncRNA-associated ceRNA networks (Ma et al., 2020). However, the roles and mechanisms of lncRNAs and the analysis of the lncRNA-associated ceRNA network in DHCA have not been comprehensively explored.
Transcription factors (TFs) are DNA-binding proteins that can play significant roles in the regulation of gene expression (Redell and Tweardy, 2006). MiRNA-TF coregulation is one of the most important feed-forward loop (FFL) types and represents a powerful method for investigating the underlying global relationships between molecular networks (Cai et al., 2021). Many studies have revealed that TFs regulate gene expression by interacting with miRNAs, for example, Mangalhara et al. revealed the zinc finger E-box binding homeobox 1(ZEB1) can downregulate miR-101 expression by regulating miR-101-1 promoter and induce Epithelial-Mesenchymal Transition (EMT) in breast cancer (Chandra Mangalhara et al., 2017). Understanding the interaction between these two regulators and their targets is crucial for revealing the complex molecular regulatory mechanisms of DHCA cerebral injury; however, detailed reports are not currently available on the TFs and TF-miRNA-mRNA network in DHCA.
In this study, we investigated the differentially expressed profiles of lncRNAs, miRNAs and mRNAs in the brain cortex of DHCA rats through high-throughput sequencing, quantitative real-time PCR (qRT-PCR) verification and bioinformatics analysis. Then, we analyzed the GO and KEGG pathways of DERNAs and established lncRNA-miRNA-mRNA and TF-miRNA-mRNA coregulatory networks. This study aims to provide insights into the mechanism of brain injury after DHCA and guidance for further steps in treatment strategies. The workflow chart and schematic diagram of the present study were showed in Figure 1.
FIGURE 1. The workflow and experimental protocol. Preop, Pre-operation; CPB, cardiopulmonary bypass; DHCA, deep hypothermic circulatory arrest.
2 Materials and Methods
2.1 Animal Model of Deep Hypothermic Circulatory Arrest
All procedures performed on the animals were approved by the Institutional Animal Care Committee of Sun Yat-sen University and conducted in compliance with Guidelines for Animal Experimentation of Sun Yat-sen University (Approval No. SYSU-IACUC-2021-000181). Twenty age-matched male Sprague–Dawley rats (age, 12–16 weeks; weight, 350–450 g) were provided by the Sun-yat Sen University Animal Center and randomly allocated into a DHCA group and a sham group, as previously described (Tu et al., 2019). In short, the rats were anesthetized with pentobarbital sodium (intraperitoneal) and orotracheally intubated with a 14G cannula, ventilated with a tidal volume of 10 ml/kg and a respiratory rate of 60–65 beats min−1 and given systemic heparinization (200 IU). Then, the left and right carotid arteries were cannulated and a multistaged venous return cannula was placed next to the junction of the inferior vena cava and right atrium through the right external jugular vein. The CPB circuit included a venous reservoir, a peristaltic pump and a custom-designed small-volume oxygenator. CPB was instituted at a flow rate of 80–100 ml kg−1 min−1, and the flow rate was decreased during the 30-min cooling process. By using a heat exchanger, a cooling blanket and ice bags, rats were cooled to a rectal temperature of 18°C within 30 min. Thereafter, the CPB was stopped and venous blood was drained into the reservoir. The animals were subjected to DHCA for another 30 min, which was confirmed by electrocardiography. Forty minutes later, the CPB was restarted. The rats were rewarmed to a rectal temperature of 34°C over 40 min, and then CPB was discontinued. Then, these rats were ventilated for an additional 60 min and gradually rewarmed to a rectal temperature of 36–37°C. Rats in the sham group only received anesthesia, cannulation, and heparin management. Sixty min later, the rats were euthanized and the brain tissue was harvested immediately for high-throughput sequencing analysis. Information on body temperature, blood pressure, heart rate, pH and PCO2 value was collected at 4 time points: just before CPB (T0), after cooling for 20 min (T1), after rewarming for 20 min (T2) and at the end of DHCA (T3).
2.2 Hematoxylin-Eosin and Nissl’s Staining
Rats (three for each group) were anesthetized and sacrificed by cervical dislocation, and the brain tissue was immediately extracted and placed on ice. The brain tissue was fixed overnight with 4% paraformaldehyde, embedded in paraffin, and sliced into serial sections with a thickness of 3–4 μm consecutively. For HE staining, the sections were deparaffinized, debenzolized, rinsed with water, and stained with hematoxylin for 8 min. The sections were then washed in running water for 5 min and stained with eosin for 2 min. For Nissl’s staining, the tissues were dewaxed to distilled water, stained with 1% toluidine blue solution at 60°C for 40 min, washed with distilled water for 3 min, then decolorized in gradient alcohol for about 3 min. Finally, sections were routinely dehydrated, cleared and resin-sealed. The morphological changes of cells were observed under a light microscope and the neuronal Nissl bodies were stained blue and purple.
2.3 RNA Isolation
Total RNA was extracted by Trizol reagent (Invitrogen, CA, United States), RNA degradation and contamination were monitored on 1% agarose gels, RNA purity was checked using the NanoPhotometer® spectrophotometer (IMPLEN, CA, United States), RNA concentration was measured using Qubit® RNA Assay Kit in Qubit® 2.0 Flurometer (Life Technologies, CA, United States), and RNA integrity was assessed using the RNA Nano 6000 Assay Kit of the Agilent Bioanalyzer 2100 system (Agilent Technologies, CA, United States).
2.4 Library Preparation, Clustering and Sequencing for RNA
A total amount of 3 μg total RNA per sample was used as input material for the small RNA library. Sequencing libraries were generated using NEBNext® Multiplex Small RNA Library Prep Set for Illumina® (NEB, United States of America) following manufacturer’s recommendations and index codes were added to attribute sequences to each sample. At last, library quality was assessed on the Agilent Bioanalyzer 2100 system using DNA High Sensitivity Chips. The clustering of the index-coded samples was performed on a cBot Cluster Generation System using TruSeq SR Cluster Kit v3-cBot-HS (Illumia) according to the manufacturer’s instructions. After cluster generation, the library preparations were sequenced on an Illumina Hiseq 2500/2000 platform and 50 bp single-end reads were generated. A total amount of 3 µg RNA per sample was used as input material for the RNA sample preparations. Sequencing libraries were generated using NEBNext® UltraTM RNA Library Prep Kit for Illumina® (NEB, United States of America) following manufacturer’s recommendations and index codes were added to attribute sequences to each sample. At last, PCR products were purified (AMPure XP system) and library quality was assessed on the Agilent Bioanalyzer 2100 system. The clustering of the index-coded samples was performed on a cBot Cluster Generation System using TruSeq PE Cluster Kit v3-cBot-HS (Illumia) according to the manufacturer’s instructions. After cluster generation, the library preparations were sequenced on an Illumina Hiseq platform and 125/150 bp paired-end reads were generated.
2.5 Quality Control and Quantification of Gene Expression Level
Raw data of fastq format were firstly processed through custom perl and python scripts. In this step, for small RNA, clean data were obtained by removing reads containing ploy-N, with 5′ adapter contaminants, without 3’ adapter or the insert tag, containing ploy A or T or G or C and low-quality reads from raw data. For Transcriptome sequencing, clean data were obtained by removing reads containing adapter, reads containing ploy-N and low-quality reads from raw data. At the same time, Q20, Q30, and GC content of the clean data were calculated. The small RNA tags were mapped to reference sequence by Bowtie without mismatch to analyze their expression and distribution on the reference (Langmead et al., 2009). MiRNA expression levels were estimated by TPM (transcript per million) through the following criteria: Normalization formula: Normalized expression = mapped readcount/Total reads*1000000. For Transcriptome sequencing, Reference genome and gene model annotation files were downloaded from genome website directly. Index of the reference genome was built using STAR and paired-end clean reads were aligned to the reference genome using STAR (v2.5.1b). HTSeq v0.6.0 was used to count the reads numbers mapped to each gene. And then FPKM of each gene was calculated based on the length of the gene and reads count mapped to this gene. The row data has been successfully deposited in GenBank, and the accession number is PRJNA739516.
2.6 Data Analysis
A DERNA analysis of the high-throughput sequencing data was performed using the edgeR R package (3.12.1) (Robinson et al., 2010). The resulting p-value were adjusted using the Benjamini and Hochberg’s approach for controlling the false discovery rate (FDR). The cutoff values for differentially expressed lncRNAs (DELs) and mRNAs (DEGs) were |log2 Fold Change| ≥2 and FDR<0.05, and for miRNAs (DEmiRNAs), |log2 Fold Change| ≥1.5 and p < 0.05. Volcano plots of DERNAs were generated using the ggplots2 R package, and a hierarchical clustering analysis was conducted using the pheatmap R package.
2.7 Construction the CeRNA Network
The DEL-associated ceRNA networks were constructed based on the competing endogenous RNA (ceRNA) hypothesis. The target miRNAs of lncRNAs were predicted based on the results of using miRanda (Enright et al., 2003), and the lncRNAs and their paired miRNAs exhibiting negatively correlated expressions were considered as lncRNA-miRNA pairs. By coexpression theory, the expressive correlation between DELs and DEGs was evaluated using the Pearson correlation coefficient (PCC), pairs with PCC > 0.95 were selected as lncRNA-mRNA pairs. The TargetScan (Agarwal et al., 2015), miRanda (Enright et al., 2003), and RNAhybrid (Rehmsmeier et al., 2004) databases were used to predict the biological targets of DEmiRNAs, the overlapping results between the targets of DEmiRNAs and DEGs were selected as miRNA-mRNA pairs. The ceRNA networks were visualized with DELs, DEmiRNAs and DEGs by using Cytoscape (version 3.8.2).
2.8 GO and KEGG Enrichment Analysis
GO and KEGG functional and pathway enrichment analyses of differentially expressed lncRNAs were implemented by the clusterProfiler R package (Yu et al., 2012), in which the gene length bias was corrected base on Wallenius non-central hyper-geometric distribution. Enriched biological process (BP), cellular component (CC), molecular function (MF) categories and KEGG pathways were used to analyze the DELs. A p-value < 0.05 was defined as statistically significant.
2.9 Establishing the TF-miRNA-mRNA and TF-lncRNA-mRNA Network
TransmiR v2.0 (http://www.cuilab.cn/transmir) (Tong et al., 2019) dataset was used to analyze the TF-miRNA, and ChIP-Atlas (http://chip-atlas.org/) (Oki et al., 2018) was used to analyze the TF-lncRNA and TF-mRNA, the threshold for statistical significance values calculated by peak-caller MACS2 was 50, and the distance range from the Transcription Start Sites (TSS) was between -1000 and +1000 bp. According to the above findings, the overlapping results were selected to established TF-miRNA-mRNA and TF-lncRNA-mRNA regulatory networks using Cytoscape (version 3.8.2) software to visualize their interactions.
2.10 Quantitative Real-Time Polymerase Chain Reaction
Total RNA was isolated using TRIzol reagent (Invitrogen, CA, United States). For lncRNAs and mRNAs, the extracted RNA was reverse transcribed into cDNA using Color Reverse Transcription kit (EZBioscience, Roseville, United States), and for miRNAs, the extracted RNA was reverse transcribed into cDNA using microRNA Reverse Transcription kit (EZBioscience, Roseville, United States) according to the manufacturer’s instructions. Quantitative real-time polymerase chain reaction (qRT-PCR) was performed to select mRNAs (Ttr, Tfpi2, Ccl2, Lhx5 and Cxcl1) and lncRNAs (Rph3a, Smim13, AABR07066379.1, LINC2085 and Lcorl) using SYBR Green qPCR Master Mix (EZBioscience, Roseville, United States) and to select miRNAs (miR-450b-3p, miR-200b-3p, miR-200a-3p and miR-429) using EZ-Probe qPCR Master Mix for microRNA (EZBioscience, Roseville, United States) according to the manufacturer’s instructions. Relative expression levels were normalized to GAPDH and U6 as internal standard controls for selected DERNAs, and they were calculated by the 2−ΔΔCt method. Specific primers were designed as shown in Table 1.
TABLE 1. Primers for the quantitative real-time PCR (qRT-PCR) assay of selected DERNAs.
2.11 Detection of Tumor Necrosis Factor-α and Western Blot
After 2 h of reperfusion, 5 rats in each group were killed by decapitation. The brain cortex of rat was harvested. Proteins were extracted from tissues in cold lysis buffer. Tumor necrosis factor (TNF)-α levels in brain cortex samples were detected using commercially available ELISA Kits (Elabscience, Wuhan, China) with the recommended protocol by the manufacturer. Protein expression levels of TNFR, NF-κB p65, IL-6, TLR1 and TLR2 were further determined with western blot analysis by using polyclonal antibodies against them (1:1000 dilution; Affinity Biosciences, United States). Western blotting was performed as standard protocol. Signals were detected with an enhanced chemiluminescence system (Millipore, Billerica, MA, United States). The protein expressions were analyzed with National Institute of Health (NIH) Image (Research Services Branch, National Institutes of Health, Bethesda, Maryland) and quantified as a relative fold to the control group after normalization with GAPDH.
2.12 Statistical Analysis
Statistical analysis was performed using SPSS (version 25; IBM, Armonk, NY, United States) and presented graphically using GraphPad Prism 8.0 (GraphPad, La Jolla, CA, United States). Numerical data are presented as the mean ± standard deviation. Differences between means were analyzed using Student’s t-test. A p-value less than 0.05 was considered statistically significant.
3 Results
3.1 Characteristics of the DHCA and Sham Rats
Detailed characteristics of the DHCA and sham rats are shown in Figure 2. For validation, significant differences were observed in the rectal temperature (Figure 2A), heart rate (Figure 2B), arterial pressure (Figure 2C), pH (Figure 2D) and PCO2 (Figure 2E) value between the DHCA and sham groups (all p < 0.05). In the sham groups, the neurons in brain tissue were normal, the nucleus were obvious and the mesenchyme was uniform (Figures 3A–C). In the DHCA groups, obvious swelling, distortion, nuclear pyknosis and nuclear disappearance were observed (Figures 3D–F). For Nissl’s staining, the sham group showed that neuronal Nissl bodies were stained blue (Figures 4A–C), however the number of blue Nissl body decreased significantly in the DHCA group (Figures 4D–F).
FIGURE 2. Characteristics of the DHCA and sham rats at four time points in DHCA. (A) Rectal temperature. (B) Heart rate. (C) Arterial pressure. (D) pH value. (E) PCO2. n = 5 per group. *p < 0.05 vs T0. Just before CPB (T0), after cooling down for 20 min (T1), after rewarming for 20 min (T2), and at the end of DHCA (T3).
FIGURE 3. Neurologic damages in the cortex induced by DHCA (n = 3, each picture represents a rat). (A–C) Sham groups. The neurons were normal in shape with obvious nucleus and uniform mesenchyme. (D–F) DHCA groups. Obvious swelling, deformation and nuclear pyknosis of neurons (Indicated by the arrow).
FIGURE 4. The Nissl’s staining showed pathological changes of cortex tissues (n = 3, each picture represents a rat). (A–C) Nissl’s body staining in cortex of sham group. (D–F) Nissl’s body staining in cortex of DHCA group.
3.2 Differential Expression of DERNAs in the DHCA and Sham Groups
High-throughput sequencing analysis was conducted to detect differential lncRNA, miRNA and mRNA expression between the DHCA and sham groups. All the DELs, DEmiRNAs and DEGs are presented by hierarchical clustering heat maps and volcano plots in Figure 5. After data normalization, a total of 89 DELs were revealed, and they included 35 upregulated and 54 downregulated lncRNAs (Figures 5A,B). Twenty-five miRNAs were found to be significantly increased, and 20 miRNAs were significantly decreased (Figures 5C,D). Among the DEGs, thirty-six were upregulated and 23 were downregulated in the DHCA group compared with the sham group (Figures 5E,F). The results of DERNAs were shown in Tables 2–4.
FIGURE 5. Differentially expressed RNAs between DHCA and sham rats. Volcano plots and heat map of the lncRNA (A,B), miRNA (C,D) and mRNA (E,F) expression profiles between the DHCA and sham groups. The vertical lines represented a p-value of 0.05 in log10 scale, the horizontal lines represented up and down regulation with 2 fold-change. The red points represented the upregulated genes, the green points represented the downregulated genes, and the gray points represented genes that were not significantly differentially expressed.
TABLE 2. The RNA-seq result of the differentially expressive mRNAs.
TABLE 3. The RNA-seq results of the differentially expressive miRNAs.
TABLE 4. The RNA-seq results of the differentially expressive lncRNAs.
3.3 Validation of the Candidate Differential Genes
The qRT-PCR was performed to verify the expression level changes gained from the RNA-seq analysis. We randomly selected 5 lncRNAs (Figure 6A), 4 miRNAs (Figure 6B) and 5 mRNAs (Figure 6C) with high fold changes to validate the RNA-seq results. These results were consistent with the high-throughput sequencing results and therefore were indicative of reliable high-throughput sequencing data. The results of fold change of these selected DERNAs were shown in Supplementary Figure S1.
FIGURE 6. qPCR validation. Comparison between the RNA-seq and qPCR results of selected differentially expressed lncRNAs (AABR07066379.1, Rph3a, Smim13, LINC2085 and Lcorl) (A), miRNAs (miR-450b-3p, miR-200b-3p, miR-200a-3p and miR-429) (B) and mRNAs (Tfpi2, Ccl2, Cxcl1, Ttr, and Lhx5) (C). The qPCR analysis results were consistent with the RNA-seq data. All reactions were repeated three times for each mRNA and IncRNA, GAPDH and U6 were used as an internal control, n = 5.
3.4 GO Annotation and KEGG Pathway Analysis
GO analyses were performed to investigate the functions of the DELs, including biological process (BP), cellular component (CC) and molecular function (MF), which may reveal the roles of the significantly differentially regulated genes. Furthermore, we found that some of the enriched functions and pathways were associated with DHCA. Figure 7A showed that the top 5 significant BP terms were extracellular stimulus, glucocorticoid stimulus, corticosteroid stimulus, cellular response to interleukin-6, and aging. The top 5 enriched CCs were implicated in extracellular space, hemoglobin complex, extracellular region part, extracellular region and C-fiber, while the significant MFs were oxygen transporter activity, oxygen binding, myosin tail binding, oxidoreduction-driven active transmembrane transporter activity and chemokine activity. Figure 7B showed the top 20 pathways revealed by the KEGG pathway analysis. The main significant pathways were related to tumor necrosis factor (TNF) signaling pathway, Malaria, NOD-like receptor signaling pathway, nuclear factor (NF) -kappa B signaling pathway and Toll-like receptor (TLR) signaling pathway. Simultaneously, the expressions of genes associated with these pathways, such as TNF-α, TNFR, NF-κ B, IL-6, IL-1β, TLR1, and TLR2, were increased after DHCA in cerebral cortex, as well as protein levels (Figure 8). Specific primers were designed as shown in Table 1.
FIGURE 7. GO and KEGG pathway analysis of differentially expressed lncRNAs in DHCA. (A) Enriched lncRNAs were functionally classified according to the biological process (BP), cellular component (CC) and molecular function (MF) categories. (B) Top 20 significantly enriched KEGG pathway terms were shown.
FIGURE 8. (A) The expressions of genes associated with the main pathways were validated by qRT-PCR. All reactions were repeated three times for each gene, GAPDH was used as an internal control, n = 5. (B) Compared with sham group, the TNF-α level in the cortex after DHCA was increased, n = 5. (C,D) The protein levels of genes associated with the main pathways after DHCA markedly increased compared with sham group, n = 5. **p < 0.01, ***p < 0.001, compared with sham group.
3.5 Construction of the CeRNA Network
To further explore the potential lncRNA-miRNA-mRNA regulatory network, a coexpression analysis of differentially expressed lncRNA and mRNAs was conducted. We then identified lncRNA and miRNA interactions and miRNA and mRNA interactions. The last constructed lncRNA-miRNA-mRNA gene pairs included lncRNA as the decoy, miRNA as the core and mRNA as the target. A total of 223 lncRNA-mRNA pairs were obtained (PCC > 0.95 and p < 0.05), and 523 lncRNA-miRNA-mRNA targeted pairs were generated. The ceRNA network was shown in Figure 9A. For example, lncRNA Lcorl regulated Ttr by competing miRNA response elements of rno-miR-200a-3p.
FIGURE 9. lncRNA-miRNA-mRNA coexpression network and TF-miRNA-mRNA network in DHCA. (A) The network displayed the correlations between the differentially expressed lncRNA-associate ceRNA profiles. The triangle nodes represent the lncRNAs, circle nodes represent the miRNAs, and rectangle nodes represent the mRNAs. The size of the node represents the degree centrality of the gene in the network. (B,C) The networks were built according to the TF-miRNA, TF-lncRNA, TF-mRNA, lncRNA-mRNA and miRNA-mRNA interactions. The blue nodes represent TFs, the green triangles represent lncRNAs, the green rectangles represent miRNAs and pink circles represent mRNAs. The size of the node represents the degree centrality of the gene in the network.
3.6 Construction of the TF Regulatory Network
The regulatory networks of TF-miRNA-mRNA and TF-lncRNA-mRNA were established, as shown in Figures 9B,C, and it involved 7 TFs (Nr3c1, Ep300, Nr1h4, Med1, Mlxipl, Hnf4a, and BRD4), 9 lncRNAs (LOC363337, LOC100361645, LOC100366054, cdk7, RGD1560108, Rph3a, Tigd2, Lcorl, Smim13), 7 miRNAs (rno-miR-146a-5p, rno-miR-210-5p, rno-miR-200b-3p, rno-miR-34c-5p, rno-miR-34c-3p, rno-miR-632, and rno-miR-144-3p), and 15 mRNAs (Map3k8, Ttr, Atf3, Sostdc1, Dclk2, Myh9, Srp68, Lhx5, Wbp11, Clic6, Ush1c, Tmem72, Ccl2, Mta1, and Tfpi2). The regulatory network for rno-miR-200b-3p included 3 transcription factors: Hnf4a, Mlxipl, and Med1. Tmem72 was the common target gene that was coregulated by rno-miR-200b-3p and the four TFs Ep300, Hnf4a, BRD4, and Mlxipl. Here, rno-miR-210-5p and Hnf4a were found to coregulate the target gene Mta1.
4 Discussion
Although the mortality and morbidity after cardiovascular surgeries have been substantially improved, the utilization of DHCA can cause damage to multiple systems, including but not limited to the cardiovascular, kidney, and nervous systems (Cooper et al., 2000; Algra et al., 2014; Bartels et al., 2014; Fang et al., 2019). Stroke and temporary neurologic deficit were observed in 2 and 5.1% of patients undergoing aortic arch surgery using DHCA, respectively (Shi et al., 2020). The safe time range of DHCA is 20–30 min, and with the extension of DHCA time, the incidence of transient or persistent neurological dysfunction after DHCA surgery will significantly increase (Wei et al., 2015; Weber et al., 2019; Shi et al., 2020).
Many studies have suggested that the noncoding RNA family represented by lncRNAs and miRNAs plays a key regulatory role in the growth and differentiation of neurons, the development of the nervous system and the occurrence of neurological diseases (Liu et al., 2018; Mirzaei et al., 2018). Wei et al. found that miR-29 could reduce neuronal apoptosis and intracellular reactive oxygen species (ROS) by inhibiting the expression of the PUMA gene (Wei et al., 2018). miR-194-5p can directly inhibit the expression of the SUMO gene and promote the death of neurons (Datwyler et al., 2011). Zhang et al. reported that overexpression of the lncRNA Malat1 can reduce autophagy in vascular endothelial cells, thus reducing ischemic stroke injury (Zhang et al., 2017). However, studies on the regulatory role of ncRNAs in DHCA-induced organ injury have mainly focused on cardiovascular and renal aspects and less on the nervous system.
High-throughput sequencing is a second-generation sequencing method that can detect the expression of coding and noncoding RNAs in tissues (Chen et al., 2021). Its application is of great significance for understanding the regulation of basic biological systems and pathophysiological conditions and developing new treatments for many diseases (Khorkova et al., 2015). To date, few studies have focused on sequencing the expression profiles of the entire transcriptome and constructing a ceRNA regulator network to identify the core regulatory factors related to cerebral cortex injury following DHCA. Therefore, we performed RNA-seq for DHCA in a rat model to explore the key mechanisms underlying DHCA.
In this study, we screened the differential expression profiles between the DHCA and sham groups, and the results suggested 89 lncRNAs, 45 miRNAs and 59 mRNAs exhibit differential expressions. A total of 80 lncRNAs, 42 miRNAs and 18 mRNAs were found in the ceRNA networks. Through the GO enrichment analysis of DE profiles, the DELs were found to be mainly concentrated on responses to interleukin-6, regulation of nitric oxide biosynthetic processes and cellular responses to reactive oxygen species. These processes, which were reported in the previous literatures focused on cerebral ischemic insult, are mainly involved in cerebral inflammation and up-regulation of oxidative stress following ischemia-reperfusion injury (Wang et al., 2015; Wei et al., 2018). The current results of DELs were in line with our previous study, in which we found that Toll-like receptor 4 (TLR4), a key modulator of the pathway of TLR/NF-κB/MMP-9, could initialize the cascade of inflammatory molecules and cytokines, which results in degradation of tight junction proteins, therefore disrupts permeability of the BBB during DHCA (Tang et al., 2014). Furthermore, annotation of the DELs associated with the most significant KEGG pathways indicated the vital upstream pathways that regulate the inflammation and oxidative stress participate in the mechanism of the cerebral injury, such as the TNF signaling, Toll-like receptor signaling pathway and NF-κB signaling pathways. These involved pathways were partially verified by qRT-PCR results indicating the increased expression of related cytokines such as TNF-α, TNFR, NF-κB, IL-6 in the mouse DHCA model (Figure 8). There are growing evidences suggesting the noncoding RNAs are associated with molecular mechanisms of the inflammatory progress of the cerebral diseases (Jing et al., 2019), however, their roles in the inflammatory response during DHCA remains to be clarified (Yao et al., 2020).
Given the central positions the Inflammation related molecules occupy in the mechanism of the DHCA cerebral injury, we focused on screening candidate noncoding RNAs in the aggregate of current DELs. Of the up-regulating DELs, what interests us most is an inflammation related lncRNA Lcorl, which was reported to be linked to genes with known connections to AD pathophysiology and other neurodegenerative diseases (Scelsi et al., 2018), its attribution to inflammatory injury following DHCA is yet to be elucidated. Another previous study indicated that downregulated miR-200a could protect neural stem cells from cerebral infarction injury, possibly by regulating the STAT and MAPK/c-MYC signaling pathways (Ma et al., 2017). Additionally, miR-200a-3p and miR-200b-3p were implicated in the pathology of AD by suppressing the expression of β-amyloid protein precursor cleaving enzyme 1 and protein kinase A (Liu et al., 2015; Wang et al., 2019). In this study, T4 transporter transthyretin (Ttr) was predicted to be a common target of Lcorl and miR-200a-3p, was also reported to be strongly associated with amyloidosis and proteotoxicity(Tu et al., 2019). Azevedo et al. revealed that Ttr could activate microglia, leading to the secretion of TNF-α, IL-6 and nitric oxide, thus triggered neuronal damage (Azevedo et al., 2013). Therefore, we further selected the Lcorl-miR-200a-3p-Ttr pair of ceRNA for relative expression qRT-PCR verification. The result was consistent with the RNA-seq results, potentially indicated that Lcorl may regulate Ttr expression via sponging miR-200a-3p, in which further investigations are needed to elucidate the details of the regulatory networks.
Another noteworthy mRNA molecule which we found in the DEGs with highest fold change of expression is C-C motif chemokine ligand 2 (Ccl2). A previous study revealed that Ccl2 exhibited the highest levels of both mRNA and protein in an MCAO rat model and ameliorated ischemic lesions through binding the corresponding receptor CCR2 (Huang et al., 2018). Furthermore, Ccl2 was found to be associated with postischemic inflammatory responses, including transendothelial migration of monocytes and BBB disruption (Mahad et al., 2006; Roberts et al., 2012). However, the expression of Ccl2 and its mechanism in DHCA brain injury have not been reported. Among the TF-mRNA regulatory networks, bromodomain-containing protein 4 (BRD4), a member of the Bromo and Extra-Terminal (BET) family, was predicted to play a role in DHCA by binding to Ccl2. BRD4 expression was correlated with glial activation and cerebral I/R injury after MCAO in mice, and BRD4 suppression decreased the expression of pro-inflammatory factors by blocking NF-κB signaling, inflammasome activation and pyroptosis (Zhou et al., 2019). Therefore, our analysis further proved the upregulation of Ccl2 expression in the DHCA cerebral cortex, which is consistent with the study by Huang et al., and predicted that the pair of BRD4-Ccl2 may be a novel therapeutic target for DHCA brain injury. Based on the aforementioned analysis, the RNA-seq results of this study facilitated a comprehensive insight into these regulating networks in DHCA brain injury and provided evidence for potential molecular target of cerebral protection in DHCA.
Finally, we identified TF-regulatory networks composed of 7 TFs: BRD4, Ep300, Nr3c1, Mlxipl, Hnf4a, Nr1h4 and MED 1. As a transcription factor, MED1 is an important part of mega transcription factor-bound in trans enhancers, which can promote estrogen (E2)-mediated improvements in the transcriptional efficiency of downstream genes through ERα, thus promoting the growth of cancer cells (Liu et al., 2014). Estrogen can attenuate traumatic brain injury by inhibiting the activation of microglia and astrocyte-mediated inflammatory responses (Wang J. et al., 2020). In a previous study, Anet al. revealed that E-cadherin transcriptional activator (Ep300) could mediate brain-derived neurotrophic factor (BDNF) activation by targeting acetylated histones H3 and H4 on the BDNF promoter during the neuropathic pain associated with chronic constriction injury (Tan et al., 2020). According to the analysis results, we found that Ep300-miR-200b-3p-Tmem72 might play important role in DHCA cerebral injury, but the interactions among the aforementioned miRNAs, mRNAs and TFs warrants further exploration.
A large number of previous studies have found that there were differences in lncRNA expression in cerebrospinal fluid (CSF) and blood during the early phaseof diseases (Kraus et al., 2017; Taghizadeh et al., 2021). A study by Zhang et al. demonstrated that lncRNA RPL34-AS1 potentially serve as a valuable diagnostic and prognostic biomarker and therapeutic target in patients with brain glioma (Zhang et al., 2021). Measurement of lncRNAs levels in cerebrospinal fluid and leukocyte samples can be used as an ideal biomarker in different stages of Parkinson’s disease (PD) (Lv et al., 2020). Additionally, in a recent study Cai et al. showed downregulated lncRNA UCA1 ameliorates the damage of dopaminergic neurons in PD rats through the inhibition of the PI3K/Akt signaling pathway, which suggested that UCA1 might be a promising therapeutic target for PD (Cai et al., 2019). Based on the above findings, the clinical applications of lncRNA as novel tools for prediction and early diagnosis of cerebral diseases have gradually become a research spot lighting in recent years. Moreover, further investigation of molecular mechanism of lncRNAs is able to contribute to providing valuable clues of targets of treatment. Therefore, tracking lncRNAs in the central nervous system of patients with neurological dysfunction is of great value for prognosis, diagnosis and development of drugs.
Our study has some limitations. First, the transcriptome results in the current study reflect only the genetic changes in the acute phase of DHCA, and the transcriptome in a chronic model of DHCA may be quite different from the current results. Second, laboratory experiments to further verify these novel genes are lacking. Finally, using p-value instead of FDR inevitably cause slight loss of specificity and increase of false positive rate in the results of miRNAs.
In this study, the transcriptome related to cerebral injury in rats after DHCA was analyzed using high-throughput sequencing technology, and lncRNA-miRNA-mRNA and TF-miRNA-mRNA regulatory networks were constructed. Meanwhile we predicted that Lcorl-miR-200a-3p-Ttr, BRD4-Ccl2 and Ep300-miR-200b-3p-Tmem72 may participate in the pathogenesis of DHCA cerebral injury through multiple proinflammatory pathways. In summary, this study provides a direction for further investigation of changes in transcriptome of DHCA cerebral injury and clues of potential molecular targets for pharmaceutical research in the future.
Data Availability Statement
The datasets presented in this study can be found in online repositories. The names of the repository/repositories and accession number(s) can be found below: https://www.ncbi.nlm.nih.gov/genbank/, PRJNA739516.
Ethics Statement
The animal study was reviewed and approved by the Sun Yat-Sen University and ethically approved by the Institutional Animal Care and Use Committee (IACUC), Sun Yat-Sen University.
Author Contributions
ML and ZW conceived the main idea. YZ and SG drafted the manuscript. ML, YL, GC, and ZW reviewed drafts of the paper and improved the manuscript. YZ, HYL, and QL collected the data and performed the statistical analysis. ZZ and HW provided statistical advice. YZ, SG, and HL analyzed the data. ML, GC, and ZW supervised the study and provided funding. All authors read and commented on the manuscript.
Funding
This article was funded by the National Natural Science Foundation of China, grant numbers 81770319, 81570039, and 82070297; and the Natural Science Funds of Guangdong Province of China, grant number 2019A1515010218.
Conflict of Interest
The authors declare that the research was conducted in the absence of any commercial or financial relationships that could be construed as a potential conflict of interest.
Publisher’s Note
All claims expressed in this article are solely those of the authors and do not necessarily represent those of their affiliated organizations, or those of the publisher, the editors and the reviewers. Any product that may be evaluated in this article, or claim that may be made by its manufacturer, is not guaranteed or endorsed by the publisher.
Supplementary Material
The Supplementary Material for this article can be found online at: https://www.frontiersin.org/articles/10.3389/fgene.2021.746757/full#supplementary-material
Supplementary Figure 1 | The relative expression of differentially expressive RNAs. All reactions were repeated three times for each lncRNA (A), miRNA (B) and mRNA (C), GAPDH and U6 were used as an internal control, n = 5, * p < 0.05, ** p < 0.01, *** p < 0.001, compared with sham group.
References
Agarwal, V., Bell, G. W., Nam, J.-W., and Bartel, D. P. (2015). Predicting Effective microRNA Target Sites in Mammalian mRNAs. Elife 4. doi:10.7554/eLife.05005
Algra, S. O., Jansen, N. J. G., van der Tweel, I., Schouten, A. N. J., Groenendaal, F., Toet, M., et al. (2014). Neurological Injury after Neonatal Cardiac Surgery. Circulation 129 (2), 224–233. doi:10.1161/circulationaha.113.003312
Apostolakis, E., and Shuhaiber, J. H. (2007). Antegrade or Retrograde Cerebral Perfusion as an Adjunct during Hypothermic Circulatory Arrest for Aortic Arch Surgery. Expert Rev. Cardiovasc. Ther. 5 (6), 1147–1161. doi:10.1586/14779072.5.6.1147
Azevedo, E. P., Ledo, J. H., Barbosa, G., Sobrinho, M., Diniz, L., Fonseca, A. C. C., et al. (2013). Activated Microglia Mediate Synapse Loss and Short-Term Memory Deficits in a Mouse Model of Transthyretin-Related Oculoleptomeningeal Amyloidosis. Cell Death Dis 4, e789. doi:10.1038/cddis.2013.325
Bartels, K., Ma, Q., N. Venkatraman, T., R. Campos, C., Smith, L., E. Cannon, R., et al. (2014). Effects of Deep Hypothermic Circulatory Arrest on the Blood Brain Barrier in a Cardiopulmonary Bypass Model - A Pilot Study. Heart Lung Circ. 23 (10), 981–984. doi:10.1016/j.hlc.2014.04.131
Cai, C., Zeng, Q., Zhou, G., and Mu, X. (2021). Identification of Novel Transcription Factor-microRNA-mRNA Co-regulatory Networks in Pulmonary Large-Cell Neuroendocrine Carcinoma. Ann. Transl Med. 9 (2), 133. doi:10.21037/atm-20-7759
Cai, L., Tu, L., Li, T., Yang, X., Ren, Y., Gu, R., et al. (2019). Downregulation of lncRNA UCA1 Ameliorates the Damage of Dopaminergic Neurons, Reduces Oxidative Stress and Inflammation in Parkinson's Disease through the Inhibition of the PI3K/Akt Signaling Pathway. Int. Immunopharmacology 75, 105734. doi:10.1016/j.intimp.2019.105734
Cefarelli, M., Murana, G., Surace, G. G., Castrovinci, S., Jafrancesco, G., Kelder, J. C., et al. (2017). Elective Aortic Arch Repair: Factors Influencing Neurologic Outcome in 791 Patients. Ann. Thorac. Surg. 104 (6), 2016–2023. doi:10.1016/j.athoracsur.2017.05.009
Centofanti, P., Barbero, C., D'Agata, F., Caglio, M. M., Caroppo, P., Cicerale, A., et al. (2016). Neurologic and Cognitive Outcomes after Aortic Arch Operation with Hypothermic Circulatory Arrest. Surgery 160 (3), 796–804. doi:10.1016/j.surg.2016.02.008
Chandra Mangalhara, K., Manvati, S., Saini, S. K., Ponnusamy, K., Agarwal, G., Abraham, S. K., et al. (2017). ERK2-ZEB1-miR-101-1 axis Contributes to Epithelial-Mesenchymal Transition and Cell Migration in Cancer. Cancer Lett. 391, 59–73. doi:10.1016/j.canlet.2017.01.016
Chen, X., Lin, B., Luo, M., Chu, W., Li, P., Liu, H., et al. (2021). Identifying circRNA- and lncRNA-Associated-ceRNA Networks in the Hippocampi of Rats Exposed to PM2.5 Using RNA-Seq Analysis. Genomics 113 (1 Pt 1), 193–204. doi:10.1016/j.ygeno.2020.12.025
Clark, M. B., Johnston, R. L., Inostroza-Ponta, M., Fox, A. H., Fortini, E., Moscato, P., et al. (2012). Genome-wide Analysis of Long Noncoding RNA Stability. Genome Res. 22 (5), 885–898. doi:10.1101/gr.131037.111
Cooper, W. A., Duarte, I. G., Thourani, V. H., Nakamura, M., Wang, N.-P., Brown, W. M., et al. (2000). Hypothermic Circulatory Arrest Causes Multisystem Vascular Endothelial Dysfunction and Apoptosis. Ann. Thorac. Surg. 69 (3), 696–702. doi:10.1016/s0003-4975(99)01524-6
Datwyler, A. L., Lättig-Tünnemann, G., Yang, W., Paschen, W., Lee, S. L. L., Dirnagl, U., et al. (2011). SUMO2/3 Conjugation Is an Endogenous Neuroprotective Mechanism. J. Cereb. Blood Flow Metab. 31 (11), 2152–2159. doi:10.1038/jcbfm.2011.112
Enright, A. J., John, B., Gaul, U., Tuschl, T., and Marks, C. D. S. (2003). MicroRNA Targets in Drosophila. Genome Biol. 5 (1), R1–R14. doi:10.1186/gb-2003-5-1-r1
Fan, S., Li, H., Wang, D., Wu, C., Pan, Z., Li, Y., et al. (2019). Effects of Four Major Brain protection Strategies during Proximal Aortic Surgery: A Systematic Review and Network Meta-Analysis. Int. J. Surg. 63, 8–15. doi:10.1016/j.ijsu.2019.01.009
Fang, Z., Wang, G., Liu, Q., Zhou, H., Zhou, S., Lei, G., et al. (2019). Moderate and Deep Hypothermic Circulatory Arrest Has a Comparable Effect on Acute Kidney Injury after Total Arch Replacement with Frozen Elephant Trunk Procedure in Type A Aortic Dissection. Interact Cardiovasc. Thorac. Surg. 29 (1), 130–136. doi:10.1093/icvts/ivz092
Feng, L., Guo, J., and Ai, F. (2019). Circulating Long Noncoding RNA ANRIL Downregulation Correlates with Increased Risk, Higher Disease Severity and Elevated Pro-inflammatory Cytokines in Patients with Acute Ischemic Stroke. J. Clin. Lab. Anal. 33 (1), e22629. doi:10.1002/jcla.22629
Filipowicz, W., Bhattacharyya, S. N., and Sonenberg, N. (2008). Mechanisms of post-transcriptional Regulation by microRNAs: Are the Answers in Sight? Nat. Rev. Genet. 9 (2), 102–114. doi:10.1038/nrg2290
Gao, S., Gu, T., Shi, E., Tang, R., Liu, J., and Shi, J. (2020). Inhibition of Long Noncoding RNA Growth Arrest-specific 5 Attenuates Cerebral Injury Induced by Deep Hypothermic Circulatory Arrest in Rats. J. Thorac. Cardiovasc. Surg. 159, 50–59. doi:10.1016/j.jtcvs.2019.01.050
Griepp, R. B., Stinson, E. B., Hollingsworth, J. F., and Buehler, D. (1975). Prosthetic Replacement of the Aortic Arch. J. Thorac. Cardiovasc. Surg. 70 (6), 1051–1063. doi:10.1016/s0022-5223(19)39653-9
Hu, Z., Wang, Z., Ren, Z., Wu, H., Zhang, M., Zhang, H., et al. (2014). Similar Cerebral Protective Effectiveness of Antegrade and Retrograde Cerebral Perfusion Combined with Deep Hypothermia Circulatory Arrest in Aortic Arch Surgery: a Meta-Analysis and Systematic Review of 5060 Patients. J. Thorac. Cardiovasc. Surg. 148 (2), 544–560. doi:10.1016/j.jtcvs.2013.10.036
Huang, Y., Wang, J., Cai, J., Qiu, Y., Zheng, H., Lai, X., et al. (2018). Targeted Homing of CCR2-Overexpressing Mesenchymal Stromal Cells to Ischemic Brain Enhances post-stroke Recovery Partially through PRDX4-Mediated Blood-Brain Barrier Preservation. Theranostics 8 (21), 5929–5944. doi:10.7150/thno.28029
Jing, H., Liu, L., Jia, Y., Yao, H., and Ma, F. (2019). Overexpression of the Long Non-coding RNA Oprm1 Alleviates Apoptosis from Cerebral Ischemia-Reperfusion Injury through the Oprm1/miR-155/GATA3 axis. Artif. Cell Nanomedicine, Biotechnol. 47 (1), 2431–2439. doi:10.1080/21691401.2019.1626408
Khorkova, O., Hsiao, J., and Wahlestedt, C. (2015). Basic Biology and Therapeutic Implications of lncRNA. Adv. Drug Deliv. Rev. 87, 15–24. doi:10.1016/j.addr.2015.05.012
Kraus, T. F. J., Haider, M., Spanner, J., Steinmaurer, M., Dietinger, V., and Kretzschmar, H. A. (2017). Altered Long Noncoding RNA Expression Precedes the Course of Parkinson's Disease-A Preliminary Report. Mol. Neurobiol. 54 (4), 2869–2877. doi:10.1007/s12035-016-9854-x
Lalevée, S., and Feil, R. (2015). Long Noncoding RNAs in Human Disease: Emerging Mechanisms and Therapeutic Strategies. Epigenomics 7 (6), 877–879. doi:10.2217/epi.15.55
Langmead, B., Trapnell, C., Pop, M., and Salzberg, S. L. (2009). Ultrafast and Memory-Efficient Alignment of Short DNA Sequences to the Human Genome. Genome Biol. 10 (3), R25. doi:10.1186/gb-2009-10-3-r25
Leshnower, B. G., Myung, R. J., Kilgo, P. D., Vassiliades, T. A., Vega, J. D., Thourani, V. H., et al. (2010). Moderate Hypothermia and Unilateral Selective Antegrade Cerebral Perfusion: a Contemporary Cerebral protection Strategy for Aortic Arch Surgery. Ann. Thorac. Surg. 90 (2), 547–554. doi:10.1016/j.athoracsur.2010.03.118
Leshnower, B. G., Thourani, V. H., Halkos, M. E., Sarin, E. L., Keeling, W. B., Lamias, M. J., et al. (2015). Moderate versus Deep Hypothermia with Unilateral Selective Antegrade Cerebral Perfusion for Acute Type A Dissection. Ann. Thorac. Surg. 100 (5), 1563–1568. doi:10.1016/j.athoracsur.2015.05.032
Liu, C., Yang, J., Zhang, C., Liu, M., Geng, X., Ji, X., et al. (2018). Analysis of Long Non-coding RNA Expression Profiles Following Focal Cerebral Ischemia in Mice. Neurosci. Lett. 665, 123–129. doi:10.1016/j.neulet.2017.11.058
Liu, H., Tian, T., Qin, S., Li, W., Zhang, X., Wang, X., et al. (2015). Folic Acid Deficiency Enhances Abeta Accumulation in APP/PS1 Mice Brain and Decreases Amyloid-Associated miRNAs Expression. J. Nutr. Biochem. 26 (12), 1502–1508. doi:10.1016/j.jnutbio.2015.07.020
Liu, Z., Merkurjev, D., Yang, F., Li, W., Oh, S., Friedman, M. J., et al. (2014). Enhancer Activation Requires Trans-recruitment of a Mega Transcription Factor Complex. Cell 159 (2), 358–373. doi:10.1016/j.cell.2014.08.027
Lv, Q., Wang, Z., Zhong, Z., and Huang, W. (2020). Role of Long Noncoding RNAs in Parkinson's Disease: Putative Biomarkers and Therapeutic Targets. Parkinson's Dis. 2020, 1–12. doi:10.1155/2020/5374307
Ma, J., Shui, S., Han, X., Guo, D., Li, T., and Yan, L. (2017). microRNA-200a Silencing Protects Neural Stem Cells against Cerebral Ischemia/reperfusion Injury. PLoS One 12 (2), e0172178. doi:10.1371/journal.pone.0172178
Ma, N., Tie, C., Yu, B., and Wan, W. J. (2020). Identifying lncRNA-miRNA-mRNA Networks to Investigate Alzheimer's Disease Pathogenesis and Therapy Strategy. Aging 12 (3), 2897–2920. doi:10.18632/aging.102785
Mahad, D., Callahan, M. K., Williams, K. A., Ubogu, E. E., Kivisäkk, P., Tucky, B., et al. (2006). Modulating CCR2 and CCL2 at the Blood-Brain Barrier: Relevance for Multiple Sclerosis Pathogenesis. Brain 129 (Pt 1), 212–223. doi:10.1093/brain/awh655
Mirzaei, H., Momeni, F., Saadatpour, L., Sahebkar, A., Goodarzi, M., Masoudifar, A., et al. (2018). MicroRNA: Relevance to Stroke Diagnosis, Prognosis, and Therapy. J. Cell Physiol 233 (2), 856–865. doi:10.1002/jcp.25787
Ng, S.-Y., Lin, L., Soh, B. S., and Stanton, L. W. (2013). Long Noncoding RNAs in Development and Disease of the central Nervous System. Trends Genet. 29 (8), 461–468. doi:10.1016/j.tig.2013.03.002
Oki, S., Ohta, T., Shioi, G., Hatanaka, H., Ogasawara, O., Okuda, Y., et al. (2018). Ch IP ‐Atlas: a Data‐mining Suite Powered by Full Integration of Public Ch IP ‐seq Data. EMBO Rep. 19 (12). doi:10.15252/embr.201846255
Redell, M. S., and Tweardy, D. J. (2006). Targeting Transcription Factors in Cancer: Challenges and Evolving Strategies. Drug Discov. Today Tech. 3 (3), 261–267. doi:10.1016/j.ddtec.2006.09.010
Rehmsmeier, M., Steffen, P., Höchsmann, M., and Giegerich, R. (2004). Fast and Effective Prediction of microRNA/target Duplexes. RNA 10 (10), 1507–1517. doi:10.1261/rna.5248604
Roberts, T. K., Eugenin, E. A., Lopez, L., Romero, I. A., Weksler, B. B., Couraud, P.-O., et al. (2012). CCL2 Disrupts the Adherens junction: Implications for Neuroinflammation. Lab. Invest. 92 (8), 1213–1233. doi:10.1038/labinvest.2012.80
Robinson, M. D., McCarthy, D. J., and Smyth, G. K. (2010). edgeR: a Bioconductor Package for Differential Expression Analysis of Digital Gene Expression Data. Bioinformatics 26 (1), 139–140. doi:10.1093/bioinformatics/btp616
Scelsi, M. A., Khan, R. R., Lorenzi, M., Christopher, L., Greicius, M. D., Schott, J. M., et al. (2018). Genetic Study of Multimodal Imaging Alzheimer's Disease Progression Score Implicates Novel Loci. Brain 141 (7), 2167–2180. doi:10.1093/brain/awy141
Shi, J., Jiang, X., Gao, S., Zhu, Y., Liu, J., Gu, T., et al. (2021). Gene-modified Exosomes Protect the Brain against Prolonged Deep Hypothermic Circulatory Arrest. Ann. Thorac. Surg. 111, 576–585. doi:10.1016/j.athoracsur.2020.05.075
Taghizadeh, E., Gheibihayat, S. M., Forough Taheri, , Afshani, S. M., Farahani, N., and Saberi, A. (2021). LncRNAs as Putative Biomarkers and Therapeutic Targets for Parkinson’s Disease. Neurol. Sci. 42 (10), 4007–4015. doi:10.1007/s10072-021-05408-7
Tan, M., Shen, L., and Hou, Y. (2020). Epigenetic Modification of BDNF Mediates Neuropathic Pain via miR-30a-3p/EP300 axis in CCI Rats. Biosci. Rep. 40 (11). doi:10.1042/BSR20194442
Tang, Z.-X., Chen, G.-X., Liang, M.-Y., Rong, J., Yao, J.-p., Yang, X., et al. (2014). Selective Antegrade Cerebral Perfusion Attenuating the TLR4/NF-Κb Pathway during Deep Hypothermia Circulatory Arrest in a Pig Model. Cardiology 128 (3), 243–250. doi:10.1159/000360694
Tong, Z., Cui, Q., Wang, J., and Zhou, Y. (2019). TransmiR v2.0: an Updated Transcription Factor-microRNA Regulation Database. Nucleic Acids Res. 47 (D1), D253–D258. doi:10.1093/nar/gky1023
Tu, L. N., Timms, A. E., Kibiryeva, N., Bittel, D., Pastuszko, A., Nigam, V., et al. (2019). Transcriptome Profiling Reveals Activation of Inflammation and Apoptosis in the Neonatal Striatum after Deep Hypothermic Circulatory Arrest. J. Thorac. Cardiovasc. Surg. 158 (3), 882–890. doi:10.1016/j.jtcvs.2019.02.091
Wang, C., Xu, X., Chen, J., Kang, Y., Guo, J., Duscher, D., et al. (2020a). The Construction and Analysis of lncRNA-miRNA-mRNA Competing Endogenous RNA Network of Schwann Cells in Diabetic Peripheral Neuropathy. Front. Bioeng. Biotechnol. 8, 490. doi:10.3389/fbioe.2020.00490
Wang, J., Hou, Y., Zhang, L., Liu, M., Zhao, J., Zhang, Z., et al. (2020b). Estrogen Attenuates Traumatic Brain Injury by Inhibiting the Activation of Microglia and Astrocyte-Mediated Neuroinflammatory Responses. Mol. Neurobiol. 58, 1052–1061. doi:10.1007/s12035-020-02171-2
Wang, L., Liu, J., Wang, Q., Jiang, H., Zeng, L., Li, Z., et al. (2019). MicroRNA-200a-3p Mediates Neuroprotection in Alzheimer-Related Deficits and Attenuates Amyloid-Beta Overproduction and Tau Hyperphosphorylation via Coregulating BACE1 and PRKACB. Front. Pharmacol. 10, 806. doi:10.3389/fphar.2019.00806
Wang, Y., Gu, T., Shi, E., Yu, L., Wang, C., Zhang, Y., et al. (2015). Inhibition of microRNA-29c Protects the Brain in a Rat Model of Prolonged Hypothermic Circulatory Arrest. J. Thorac. Cardiovasc. Surg. 150 (3), 675–684. doi:10.1016/j.jtcvs.2015.04.062
Weber, C., Jenke, A., Chobanova, V., Yazdanyar, M., Chekhoeva, A., Eghbalzadeh, K., et al. (2019). Targeting of Cell-free DNA by DNase I Diminishes Endothelial Dysfunction and Inflammation in a Rat Model of Cardiopulmonary Bypass. Sci. Rep. 9 (1), 19249. doi:10.1038/s41598-019-55863-8
Wei, R., Zhang, R., Li, H., Li, H., Zhang, S., Xie, Y., et al. (2018). MiR-29 Targets PUMA to Suppress Oxygen and Glucose Deprivation/Reperfusion (OGD/R)-induced Cell Death in Hippocampal Neurons. Cnr 15 (1), 47–54. doi:10.2174/1567202615666180403170902
Wei, R., Zhang, R., Xie, Y., Shen, L., and Chen, F. (2015). Hydrogen Suppresses Hypoxia/Reoxygenation-Induced Cell Death in Hippocampal Neurons through Reducing Oxidative Stress. Cell Physiol Biochem 36 (2), 585–598. doi:10.1159/000430122
Yao, P., Li, Y.-L., Chen, Y., Shen, W., Wu, K.-Y., and Xu, W.-h. (2020). Overexpression of Long Non-coding RNA Rian Attenuates Cell Apoptosis from Cerebral Ischemia-Reperfusion Injury via Rian/miR-144-3p/GATA3 Signaling. Gene 737, 144411. doi:10.1016/j.gene.2020.144411
Yu, G., Wang, L.-G., Han, Y., and He, Q.-Y. (2012). clusterProfiler: an R Package for Comparing Biological Themes Among Gene Clusters. OMICS: A J. Integr. Biol. 16 (5), 284–287. doi:10.1089/omi.2011.0118
Yu, S.-y., Tang, L., and Zhou, S.-h. (2018). Long Noncoding RNAs: New Players in Ischaemia-Reperfusion Injury. Heart Lung Circ. 27 (3), 322–332. doi:10.1016/j.hlc.2017.09.011
Zhang, D., Jiang, H., Ye, J., Gao, M., Wang, X., Lu, E., et al. (2021). A Novel lncRNA, RPL34-AS1, Promotes Proliferation and Angiogenesis in Glioma by Regulating VEGFA. J. Cancer 12 (20), 6189–6197. doi:10.7150/jca.59337
Zhang, J., Yuan, L., Zhang, X., Hamblin, M. H., Zhu, T., Meng, F., et al. (2016). Altered Long Non-coding RNA Transcriptomic Profiles in Brain Microvascular Endothelium after Cerebral Ischemia. Exp. Neurol. 277, 162–170. doi:10.1016/j.expneurol.2015.12.014
Zhang, X., Hamblin, M. H., and Yin, K.-J. (2019). Noncoding RNAs and Stroke. Neuroscientist 25 (1), 22–26. doi:10.1177/1073858418769556
Zhang, X., Tang, X., Liu, K., Hamblin, M. H., and Yin, K.-J. (2017). Long Noncoding RNA Malat1 Regulates Cerebrovascular Pathologies in Ischemic Stroke. J. Neurosci. 37 (7), 1797–1806. doi:10.1523/JNEUROSCI.3389-16.2017
Zhong, Y., Yu, C., and Qin, W. (2019). LncRNA SNHG14 Promotes Inflammatory Response Induced by Cerebral Ischemia/reperfusion Injury through Regulating miR-136-5p/ROCK1. Cancer Gene Ther. 26 (7-8), 234–247. doi:10.1038/s41417-018-0067-5
Keywords: deep hypothermic circulatory arrest (DHCA), high-throughput sequencing, long noncoding RNA (lncRNA), microRNA (miRNA), transcription factor (TF), transcription factor-miRNA coregulatory network (TF-miRNA coregulatory network)
Citation: Liang M, Zhang Y, Gan S, Liu Y, Li H, Liu Q, Liu H, Zhou Z, Wu H, Chen G and Wu Z (2021) Identifying lncRNA- and Transcription Factor-Associated Regulatory Networks in the Cortex of Rats With Deep Hypothermic Circulatory Arrest. Front. Genet. 12:746757. doi: 10.3389/fgene.2021.746757
Received: 24 July 2021; Accepted: 30 November 2021;
Published: 17 December 2021.
Edited by:
Zhexing Wen, Emory University, United StatesCopyright © 2021 Liang, Zhang, Gan, Liu, Li, Liu, Liu, Zhou, Wu, Chen and Wu. This is an open-access article distributed under the terms of the Creative Commons Attribution License (CC BY). The use, distribution or reproduction in other forums is permitted, provided the original author(s) and the copyright owner(s) are credited and that the original publication in this journal is cited, in accordance with accepted academic practice. No use, distribution or reproduction is permitted which does not comply with these terms.
*Correspondence: Zhongkai Wu, wuzhk@mail.sysu.edu.cn
†These authors have contributed equally to this work