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Original Research ARTICLE

Front. Physiol., 12 February 2019 | https://doi.org/10.3389/fphys.2019.00080

KLF4-Induced Connexin40 Expression Contributes to Arterial Endothelial Quiescence

Jean-François Denis1, Mannekomba R. Diagbouga1, Filippo Molica1, Aurélie Hautefort1, Tanja Linnerz1, Masakatsu Watanabe2, Sylvain Lemeille1, Julien Y. Bertrand1 and Brenda R. Kwak1,3*
  • 1Department of Pathology and Immunology, University of Geneva, Geneva, Switzerland
  • 2Graduate School of Frontier Biosciences, Osaka University, Osaka, Japan
  • 3Department of Medical Specializations – Cardiology, University of Geneva, Geneva, Switzerland

Shear stress, a blood flow-induced frictional force, is essential in the control of endothelial cell (EC) homeostasis. High laminar shear stress (HLSS), as observed in straight parts of arteries, assures a quiescent non-activated endothelium through the induction of Krüppel-like transcription factors (KLFs). Connexin40 (Cx40)-mediated gap junctional communication is known to contribute to a healthy endothelium by propagating anti-inflammatory signals between ECs, however, the molecular basis of the transcriptional regulation of Cx40 as well as its downstream effectors remain poorly understood. Here, we show that flow-induced KLF4 regulated Cx40 expression in a mouse EC line. Chromatin immunoprecipitation in ECs revealed that KLF4 bound to three predicted KLF consensus binding sites in the Cx40 promoter. HLSS-dependent induction of Cx40 expression was confirmed in primary human ECs. The downstream effects of Cx40 modulation in ECs exposed to HLSS were elucidated by an unbiased transcriptomics approach. Cell cycle progression was identified as an important downstream target of Cx40 under HLSS. In agreement, an increase in the proportion of proliferating cell nuclear antigen (PCNA)-positive ECs and a decrease in the proportion of ECs in the G0/G1 phase were observed under HLSS after Cx40 silencing. Transfection of communication-incompetent HeLa cells with Cx40 demonstrated that the regulation of proliferation by Cx40 was not limited to ECs. Using a zebrafish model, we finally showed faster intersegmental vessel growth and branching into the dorsal longitudinal anastomotic vessel in embryos knock-out for the Cx40 orthologs Cx41.8 and Cx45.6. Most significant effects were observed in embryos with a mutant Cx41.8 encoding for a channel with reduced gap junctional function. Faster intersegmental vessel growth in Cx41.8 mutant embryos was associated with increased EC proliferation as assessed by PH3 immunostaining. Our data shows a novel evolutionary-conserved role of flow-driven KLF4-dependent Cx40 expression in endothelial quiescence that may be relevant for the control of atherosclerosis and diseases involving sprouting angiogenesis.

Introduction

Arteries are exposed to various biomechanical forces, which they sense via numerous mechanoreceptors (Kwak et al., 2014). On the luminal side, endothelial cells (ECs) sense shear stress, a blood flow-induced frictional force. This force varies in time, magnitude and direction according to the pulsatility of blood flow and vessel geometry, and is a critical regulator of endothelial function (Davies et al., 2013; Simmons et al., 2016). Atherosclerosis predominantly develops in regions of the arterial tree that are subjected to disturbed blood flow such as arterial bifurcations (Brown et al., 2016; Morbiducci et al., 2016). In contrast, straight parts of arteries experiencing a high laminar shear stress (HLSS) are protected from the disease. ECs in athero-susceptible regions are prone to pro-inflammatory activation and display an elevated permeability to lipoproteins compared to ECs at athero-protected sites (Kwak et al., 2014). Possibly as a response to injury, ECs at regions of disturbed flow regions display an increased turnover (Kwak et al., 2014).

Members of the Krüppel-like family of transcription factors, i.e., KLF2 and KLF4, are highly expressed in regions exposed to athero-protective flow (Tabas et al., 2015). They take part in the anti-inflammatory phenotype of ECs through induction of endothelial nitric oxide synthase expression and by attenuating the expression of the vascular cell adhesion molecule-1 and E-selectin, for example (SenBanerjee et al., 2004; Dekker et al., 2005). Although ECs display substantial heterogeneity in their individual response to receptor-mediated signaling (Huang et al., 2000; Pogoda et al., 2018), the presence of gap junctions between high and low responders enables a synchronized response with the endothelial syncytium.

Gap junction channels are comprised of connexins (Cxs), a family of transmembrane proteins with high homology among vertebrates, in particular in the N-terminal-, transmembrane- and extracellular loop domains (Eastman et al., 2006; Cruciani and Mikalsen, 2007). There are 20–21 Cxs in mammals and the zebrafish genome has been predicted to contain 39 Cx-encoding genes (Watanabe, 2017). This high number of Cxs can be attributed to gene duplication during fish evolution, but it is not known whether all the genes are expressed and functional (Watanabe, 2017). Six Cxs oligomerize to form a connexon, and two connexons from adjacent cells dock to establish a gap junction channel, enabling direct communication between neighboring cells through diffusion of ions and small metabolites (Leybaert et al., 2017). ECs in arteries express Cx37, Cx40, and Cx43 in a non-uniform manner (Molica et al., 2018). Cx43 is predominantly expressed in ECs at branching points or bifurcations of arteries exposed to disturbed blood flow (Gabriels and Paul, 1998), whereas Cx37 and Cx40 are expressed in ECs of straight arterial parts exposed to HLSS (Pfenniger et al., 2012; Denis et al., 2017). Interestingly, endothelial Cx40 interacts with IκBα, resulting in decreased activation of the NF-κB transcription factor thereby limiting the inflammatory response (Denis et al., 2017). In agreement, EC-specific deletion of Cx40 accelerates atherosclerosis in mice (Chadjichristos et al., 2010).

Little is known regarding the signal transduction pathways involved in HLSS-dependent regulation of Cx40 levels. A low level of laminar shear stress (LLSS) has been shown to induce a long-term expression of Cx40 in human umbilical vein ECs with PI3K activity being required for basal Cx40 expression and Akt activity taking part in its shear stress-dependent induction (Vorderwulbecke et al., 2012). However, the transcriptional regulation of Cx40 induction by arterial HLSS levels remains to be investigated. Moreover, no large-scale analysis to elucidate the downstream signaling and function of Cx40 under arterial shear stress levels has been performed to date.

Materials and Methods

Cell Culture

Different cell lines were used: (a) a mouse EC line (bEnd.3) (Kwak et al., 2001), (b) a communication-incompetent sub-clone of human HeLa cells (ATCC), and (c) the afore-mentioned HeLa cells stably transfected with murine Cx40 (Elfgang et al., 1995). Cells were grown in DMEM (41966-029, Gibco) supplemented with 10% fetal bovine serum (FBS; Sigma), 5000 U/L penicillin and 5 mg/mL streptomycin (Gibco). The medium of the stably Cx40-transfected HeLa cells was supplemented with 0.5 μg/mL puromycin (Sigma-Aldrich). bEnd.3 cells were grown on coverslips, dishes or Ibidi μ-Slide VI0.4 coated with 1.5% gelatin (Sigma-Aldrich).

Silencing of KLF4 or Cx40 in bEnd.3 cells was done using short interfering RNA (siRNA) SMARTpool ON-TARGETplus Mouse KLF4 siRNA or Mouse Gja5 siRNA (Dharmacon). The ON-TARGETplus Non-targeting (NT) Pool (Dharmacon) was used as negative control. The transfections were performed under serum-free conditions with 25 nmol/L siRNA and 5 mg/L DharmaFECT4 (Dharmacon). The efficiency of the KLF4 silencing was determined by quantitative real-time PCR (qPCR).

Human umbilical vein endothelial cells (HUVECs) from two different donors were purchased from Lonza and grown in EGM-2 medium (Promocell) at 37°C in a humidified atmosphere containing 5% CO2. Cells were passaged by trypsin–EDTA (Gibco) treatment and used at passages 4–6 for each donor.

Flow Experiments

Sixty thousand bEnd.3 cells were seeded per Ibidi μ-Slide VI0.4 channel and grown till confluence. Thereafter, siRNA for Cx40 or KLF4 was applied for 24 h as detailed above. A non-targeting pool of siRNA (siNT) was used as a control. Thereafter, cells were exposed for 48 h to defined flow conditions, i.e., HLSS: 20 dynes/cm2, LLSS: 5 dynes/cm2 or oscillatory shear stress (OSS): 5 dynes/cm2, 1 Hz, using the Ibidi pump system. Control cells were kept under no flow (static) conditions.

Alternatively, bEnd.3 cells or HUVECs were seeded in 6-well plates and grown to confluence. Thereafter, the 6-well plates were placed onto an orbital rotating platform (Grant Instruments) housed inside a cell culture incubator, and ECs were cultured for an additional 48 h. The radius of orbit of the orbital shaker was 10 mm and the rotation rate was set to 210 rpm, which induced swirling of the 3 mL culture medium over the cell surface and exposed the ECs to a wall shear stress of a defined magnitude and direction at the base, as described previously (Warboys et al., 2014). ECs exposed to undisturbed flow (HLSS; at the periphery) and disturbed flow (OSS; in the center) were compared to static conditions.

Immunofluorescence Staining

Immunofluorescent staining on bEnd.3 cells was performed as previously described (Kwak et al., 2001). In short, confluent bEnd.3 cultures were fixed with 100% methanol at -20°C for 5 min. Subsequently, the samples were permeabilized with 0.2% Triton X-100 in PBS for 30 min, charges neutralized with 0.5 mol/L NH4Cl in PBS for 15 min and blocked with 2% bovine serum albumin (BSA; AppliChem) or with 10% normal goat serum (Vector Laboratories) in PBS for 30 min. Next, the primary antibody against Cx40 (Alpha-Diagnostics; 1/200) or anti-proliferating cell nuclear antigen (PCNA; Thermo Fisher Scientific; 1/25) in blocking solution was applied and incubated overnight at 4°C. Finally, an Alexa Fluor 488-conjugated goat anti-rabbit antibody (Thermo Fisher Scientific, 1/2000) was used for signal detection. The nuclei and cells were counterstained with 4,6-diamidino-2-fenylindool (DAPI) and 0.003% Evans Blue, respectively. Samples on coverslips were mounted with Vectashield (Vector Laboratories) or with Ibidi mounting medium for Ibidi μ-Slides and imaged with an epifluorescent Zeiss Axiocam fluo microscope (Zeiss Axio Imager Z1) equipped with an AxioCam 506 mono camera (Carl Zeiss AG) and analyzed using the Zeiss Zen 2.3 software.

Fluorescence-Activated Cell Sorting (FACS)

Cell cycle status was determined in bEnd.3 cells using Hoechst 33342 (Thermo Fisher Scientific), a non-toxic specific vital stain for DNA, at a concentration of 10 μg/mL in Ibidi slides. Thereafter, cells were detached with trypsin (Gibco) for 5 min and their distribution was measured using a BDLSR Fortessa FACS (Becton Dickinson) equipped with a BD HTS unit (Becton Dickinson). Analysis of the cell populations in the different cell cycle compartments was performed using FlowJo software.

Western Blot

Cell cultures were rinsed with PBS, pH = 7.4, and lysed in RIPA buffer as previously described (Pfenniger et al., 2012). After protein concentration quantification with a Micro BCA protein assay kit (Thermo Scientific), 5 μg (HUVECs) or 10 μg (bEnd.3) of protein was separated by SDS-PAGE and transferred to PVDF-membrane (Immobilon, Millipore). After 2 h blocking with 5% milk and 1% Tween in PBS, the membrane was exposed to anti-Cx40 (Alpha-Diagnostics, 1/500) or anti-β-actin (Sigma, 1/10000) primary antibodies in blocking solution. Revelation was performed by incubating the membrane for 1 h at RT with secondary horseradish peroxidase-conjugated antibodies (Jackson ImmunoResearch; 1/5000) and followed by ECL detection (Millipore) using ImageQuant LAS 4000 software. Band intensities were thereafter quantified using ImageJ software. Cx40 results were normalized to β-actin.

Quantitative Real-Time PCR

Total RNA was extracted from bEnd.3 cells using the NucleoSpin RNA II kit (Macherey-Nagel) according to the manufacturers’ instructions. After extraction, RNA concentration was determined using a Nanodrop 2000c (Thermo Fisher Scientific) and equal amounts of RNA were used to obtain cDNA with the reverse transcriptase reaction kit (QuantiTect Reverse Transcription Kit, Qiagen). PCR was performed using the ABI StepOne Plus detection system with Taqman gene expression assays (Applied Biosystems) according to the manufacturers’ protocol. All reactions were normalized to GAPDH.

Chromatin Immunoprecipitation (ChIP)

bEnd.3 cells were grown until confluence in P100 dishes. The Simple Chip Enzymatic Chromatin IP kit with magnetic beads (Cell Signaling Technology) was used according to the manufacturers’ protocol. In short, chromatin was cross-linked with formaldehyde (Thermo Fisher Scientific) to a final concentration of 1% for 10 min and the reaction was stopped by adding glycine. Next, the cells were lysed and nuclei extracted. Micrococcal nuclease and sonication were used to fragment DNA (fragmentation between 150 and 900 bp) and cross-linked chromatin was extracted. The efficiency of the chromatin digestion was determined by electrophoresis on a 1% agarose gel. Ten micrograms of digested, cross-linked chromatin was immunoprecipitated using 2 μg anti-KLF4 antibody (R&D systems) and protein magnetic beads. As positive control a monoclonal rabbit anti-Histone H3 antibody (Cell Signaling Technology) was used and as negative control a rabbit IgG (Cell Signaling Technology). Finally, after elution and the reversal of the cross-linking, DNA was purified and efficiency of the procedure was assessed by qPCR. Putative KLF consensus binding sites in the promoter region of Cx40 [CACCC elements and other probable transcription factor binding sites (TFBS)] were predicted using the MatInspector online software1. Primers for the Cx40 promoter region were designed using the Primer3 version 0.4.0 online software. Primer sequences, named according to the location of the TFBS with respect to the transcription start site, are as follows:

- 2477 forward: AGCTTCTTTGCAGTGCCATT,

- 2477 reverse: TGCCATGCTCTCTCCTTCTT;

- 2599 forward: CCATCTCACCAGCCCTAAAG,

- 2599 reverse: TGGGCACACTTCACAATGTT;

- 4196 forward: TCTCAACCAGCAGAAACGTG,

- 4196 reverse: ATGGCAACACGTGCAAGTAA.

As KLF4 positive control, primers against a previously known TFBS on the fibroblast-specific protein 1 (FSP1) promoter region were used (Cuttano et al., 2016). Quantification of the ChIP efficiency was performed by qPCR with Power Up SYBR Green Master Mix (Applied Biosystems).

Library Preparation, Sequencing, Read Mapping to the Reference Genome and Gene Coverage Reporting

Following the above-described flow conditions, total RNA was isolated for the four conditions using the NucleoSpin RNA II kit (Macherey-Nagel) according to the manufacturers’ instructions. Quality of the three samples per condition was verified using the Agilent 2100 Bioanalyzer with the Agilent RNA 6000 Nano Kit (Agilent Technologies). cDNA libraries were constructed by the Genomic platform of the University of Geneva using the Illumina TruSeq RNA sample Preparation Kit according to the manufacturers’ protocol. Libraries were sequenced using single-end (50 nt-long) on Illumina HiSeq2000. FastQ reads were mapped to the ENSEMBL reference genome (GRCm38.80) using STAR version 2.4.0j (Dobin et al., 2013) with standard settings, except that any reads mapping to more than one location of the genome (ambiguous reads) were discarded (m = 1). Sequence data have been submitted to the GEO database under accession number GSE118717. A unique gene model was used to quantify reads per gene. In short, the model considers all annotated exons of all annotated protein coding isoforms of a gene to create a unique gene where the genomic region of all exons are considered as coming from the same RNA molecule and merged together.

RNAseq Analysis

All reads overlapping the exons of each unique gene model were reported using featureCounts version 1.4.6-p1 (Quinlan and Hall, 2010). Gene expressions were reported as raw counts and normalized in reads per kilobase per million (RPKM) in order to filter out genes with low expression value (<1 RPKM) before calling for differentially expressed genes. Library size normalizations and differential gene expression calculations were performed using the package edgeR (Robinson et al., 2010) designed for R software (Team, 2008). Only genes having significant fold-change (Benjamini-Hochberg corrected p-value <0.01) were considered for the rest of the RNAseq analysis. Differentially expressed genes were categorized on basis of their involvement in atherosclerosis-related processes such as inflammation, angiogenesis, permeability, vascular tone, extracellular matrix (ECM) interaction, metabolic processes or immune response. In each condition, approximately 50% of differentially expressed genes did match to these categories.

Gene Set Enrichment Analysis (GSEA)

All annotated pathways for Homo sapiens, Mus musculus, Rattus norvegicus and Danio rerio available on WikiPathways database2 were used to generate gene sets, as well as the KEGG metabolic pathways (KEGG3) relative to GRCm38.80. Genes were ranked by calculated fold-changes (decreasing ranking). A gene set analysis using the GSEA package Version 2.2 (Mootha et al., 2003; Subramanian et al., 2005) from the Broad Institute (MIT, Cambridge, MA, United States) was used to analyze the pattern of differential gene expression between the two groups. Gene set permutations were performed 1,000 times for each analysis. The Normalized Enrichment Score (NES) was calculated for each gene set. GSEA results with a nominal fold discovery rate (FDR) < 0.05 and abs(NES) > 1 were considered significant. In order to identify the subset of genes that are involved in several biological processes, a leading-edge analysis was performed. All leading-edge subsets of each significant regulated pathway [FDR < 0.05 and abs(NES) > 1] were extracted and the number of times each gene appears was reported. Then, per pathway, the mean of gene occurrences was calculated and, in order to simplify the picture, pathways with a mean lower than 10% of the total number of regulated pathways were removed from the analysis. Next, the counts of each gene were re-calculated and leading-edge genes as well as remaining pathways were hierarchically clustered on an heatmap. Only genes with a total number of occurrences higher than 2 appear on the heatmap. Per comparison, pathways involving up- or down-regulated genes were analyzed separately.

Zebrafish Strains, Husbandry, and Genotyping

AB zebrafish strains, along with transgenic and leopard mutant strains, were kept in a 14/10 h light/dark cycle at 28°C. Embryos were obtained as described previously (Westerfield, 2000). We used the following strains: Tg(flk1:eGFP)s843 (Jin et al., 2005), sihtc300b (Chen et al., 1996), leot1/t1 (hereafter called: Cx41.8t1/t1) (Watanabe et al., 2006), leotq270/tq270 (hereafter called: Cx41.8tq/tq) (Watanabe et al., 2006), Cx41.8t1/t1Cx45.6-/-, Tg(flk1:eGFP)Cx41.8t1/t1, Tg(flk1:eGFP)Cx41.8tq/tq, and Tg(flk1:eGFP)Cx41.8t1/t1Cx45.6-/-. The Cx45.6 knock-out mutant was generated by Transcription Activator-Like Effector Nucleases (TALENs) technique using a similar procedure as previously described (Misu et al., 2016). The target sequence for the Cx45.6 knock-out was 5-TGTCTGTTATGACCGAGCTTTccccattgctcatatccGCTACTGGGTGCTGCAGA-3 (TALEN binding sequences are shown in upper case and spacer sequence in lower case).

For genotyping genomic DNA was extracted from fin clips and used for PCR using the following primer pairs:

forward Cx41.8t1: AGATCAGAGAAGGTGTAGAC,

reverse Cx41.8t1: AGGTTAATTGGGCAAATTAGG;

forward Cx41.8tq: TGCTGCAAACATACGTCCTC,

reverse Cx41.8tq: TTTGCAGAGTTCTGCTGGTG;

forward Cx45.6: GGTGAGGAGTATGGGGGACT,

reverse Cx45.6: AGGGTGTCGATACGAAGACG.

The t1 and tq270 mutations in the Cx41.8 gene were detected by sequencing of the PCR fragments. Of note, the C>T t1 mutation results in premature stop codon and a knock-out phenotype. The A>T tq270 mutation results in a reduced channel function (Watanabe et al., 2006, 2016). Cx45.6 PCR fragments were digested with BsrDI resulting in 221 bp and 54 bp fragments for the wild-type allele and a 268 bp fragment for the mutant allele.

Cell Sorting and qPCR

Zebrafish embryos [24–48 h-post-fertilization (hpf)] were incubated in 0.5 mg/mL Liberase (Roche) solution for 90 min at 33°C, then dissociated and resuspended in 0.9X PBS-1% FBS. We excluded dead cells by SYTOX-red (Life Technologies) staining. Cell sorting for eGFP was performed using an Aria II (BD Biosciences).

RNA from eGFP+ and eGFP- populations was extracted using the NucleoSpin RNA II kit (Macherey-Nagel) and reverse transcribed into cDNA using the QuantiTect Reverse Transcription Kit (Qiagen). qPCR was performed using the ABI StepOne Plus detection system with SYBR green gene expression assays (KAPA SYBR FAST, Kapa Biosystems) supplemented with ROX high detection solution according to the manufacturers’ protocol using the following primers:

forward Cx41.8: ACCGAGGTTGAATGCTCC,

reverse Cx41.8: TGGTTTCAATCAGGCTCC;

forward Cx45.6: CTAAGCCTGCGCTTGTCTCT,

reverse Cx45.6: GGCTCGGGTTCGAAGTGAAA;

forward Ef1α: GGTAGTATTTGCTGGTCTCG,

reverse Ef1α: GAGAAGTTCGAGAAGGAAGC.

Each qPCR experiment was performed using biological triplicates. Experiments were repeated three times and fold-change averages from each experiment were obtained.

Zebrafish Embryo Imaging

Transgenic fluorescent embryos were dechorionated with pronase (Sigma-Aldrich) at 24 hpf and held in E3 buffer containing 0.003% tricaine methanesulfonate (Sigma-Aldrich) for imaging. Imaging was performed at 24, 28 or 48 hpf using an Olympus IX83 microscope and processed using CellSens Dimensions software.

The developmental stage of intersegmental vessels (ISVs) was quantified on the 10 proximal ISVs of the dorsal aorta (DA) in each individual fish at 28 hpf. A blinded observer classified the ISVs as: (1) partial ISV sprouts, (2) complete (full-length) ISVs, or (3) ISVs with complete branching forming the dorsal longitudinal anastomotic vessel (DLAV). Scoring distribution was compared with Fisher’s exact test.

Zebrafish embryos at 24 hpf were overnight stained with rabbit anti-PH3 (Abcam; 1/250) and chicken anti-eGFP (Life Technologies; 1/1400) after a 4-h fixation with 4% PFA at 4°C. Embryos were thereafter washed with 0.02% Triton X-100 in PBS and blocked for 1 h at 4°C in the same solution containing 4% BSA and 0.02% NaN3. Embryos were then incubated overnight at 4°C. After washing with 0.01% Triton X-100 in PBS, embryos were incubated with appropriate secondary antibodies [Alexa Fluor 488-conjugated anti-chicken (Life Technologies, 1/1000) and AlexaFluor594-conjugated anti-rabbit (Life Technologies, 1/1000)] and washed again before imaging with an Olympus IX83 microscope and processed using CellSens Dimensions software. A blinded observer counted the PH3+ nuclei in the proximal 10 ISVs of each embryo.

Statistics

Unless otherwise specified, results are presented as mean ± SEM. Unpaired Student’s t-tests (equal variance), Mann–Whitney U tests (unequal variance) or one-way ANOVAs were used to compare differences between groups. Differences with a P < 0.05 were considered statistically significant; P < 0.05; ∗∗P < 0.01; ∗∗∗P < 0.001; ∗∗∗∗P < 0.0001.

Results

KLF4 Regulates Flow-Dependent Cx40 Expression

The KLF2 and KLF4 transcription factors have been shown to act as critical regulators of multiple genes involved in endothelial homeostasis under HLSS (Davies et al., 2013). Although Cx37 expression is regulated by KLF2, this transcription factor seems not involved in the regulation of endothelial Cx40 expression (Pfenniger et al., 2012). To identify the transcription factor involved in flow-dependent Cx40 expression, we used the mouse EC line bEnd.3 known to express all three endothelial connexins (Kwak et al., 2001). Confluent cultures of bEnd.3 cells were exposed to LLSS (5 dynes/cm2) or HLSS (20 dynes/cm2) for 24 h or kept under static conditions. As expected, KLF4 mRNA levels increased gradually with the level of shear stress with a doubling under LLSS and a threefold increase in response to HLSS (Figure 1A). Compared to static conditions, LLSS and HLSS induced Cx40 transcript by about 10-fold (Figure 1B). In addition, a gradual increase in Cx40 protein was observed in ECs in response to increasing levels of laminar shear stress (Figure 1C). Shear stress-dependent regulation of Cx40 was also investigated using an orbital rotating platform. As detailed elsewhere (Warboys et al., 2014), on a rotating platform ECs at the periphery of the culture well are exposed to HLSS and cells in the center to OSS (Figure 1D). As shown in Figure 1E, HLSS enhanced Cx40 expression compared to static conditions. As expected (Denis et al., 2017), Cx40 expression in bEnd.3 cells was low under OSS and not different from static conditions (data not shown). Finally, we confirmed shear stress-dependent regulation of Cx40 expression in primary human ECs. As expected, HUVECs aligned in the direction of the flow at the periphery of the rotating culture well and were cobblestone-shaped under static conditions (Figure 1F). Moreover, HLSS enhanced Cx40 expression, similar to the effect observed in bEnd.3 cells (Figures 1G,H).

FIGURE 1
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Figure 1. Cx40 expression is gradually regulated by shear stress. (A) KLF4 expression in bEnd.3 cells under static conditions (St) or exposed to 24 h of LLSS and HLSS was assessed by qPCR. N = 3. (B) Cx40 expression in bEnd.3 cells under static conditions (St) or exposed to 24 h of LLSS and HLSS was assessed by qPCR. N = 3. (C) Representative images of Cx40 expression (green) in bEnd.3 cells under static conditions (St) or exposed to LLSS and HLSS for 24 h. Arrow indicates the direction of flow. Nuclei were stained with DAPI (blue). Scale bar represents 10 μm. (D) Schematic representation of flow regions in cell cultures induced by orbital rotation; green = HLSS and red = OSS. (E) Cx40 expression in bEnd.3 cells under static conditions (St) or exposed to 48 h of HLSS was assessed by Western blotting. N = 5. (F) Phase-contrast images of HUVECs under static conditions or exposed for 48 h of HLSS. (G,H) Cx40 expression in HUVECs under static conditions (St) or exposed to 48 h of HLSS was assessed by Western blotting (G) or qPCR (H; N = 6).

To determine the possible causal relationship between flow-driven KLF4 and Cx40 expression, confluent cultures of bEnd.3 cells were transfected with siRNA directed against KLF4. Under static conditions, siKLF4 effectively reduced the expression of KLF4 mRNA by 50% compared to siNT (data not shown). Next, confluent ECs were treated with siKLF4 or siNT for 24 h followed by 48 h of HLSS or static conditions. In presence of siNT the ECs responded similarly to HLSS with a threefold induction of KLF4 transcript and a ninefold increase in Cx40 mRNA (compare Figures 2A,B vs. Figures 1A,B). However, a prior exposure to KLF4 siRNA blunted the HLSS-driven induction of both KLF4 and Cx40 by half (Figures 2A,B). Notably, the HLSS-driven induction of KLF2 and Cx37 was not affected by siKLF4 (Figures 2C,D). Moreover, Cx43 transcript was not significantly affected by HLSS or siKLF4 (Figure 2E). Together, these results indicate that KLF4 participates in the induction of Cx40 by HLSS in ECs.

FIGURE 2
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Figure 2. KLF4 regulates flow-dependent Cx40 expression. KLF4 (A), Cx40 (B), KLF2 (C), Cx37 (D) and Cx43 (E) expression in bEnd.3 cells transfected with KLF4 siRNA or NT siRNA and subsequently exposed to 48 h of HLSS or kept under static conditions. N = 6. (F) Representative ChIP results for bEnd.3 chromatin precipitated with antibodies against KLF4. Three different CACCC KLF-consensus sites (indicated in bp) were amplified for Cx40 (left) and one for FSP1 (right; positive control). Levels of DNA are normalized to input. N = 2.

The Cx40 promoter contains multiple CACCC elements, which are preferential binding sites of the KLF transcription factors. To investigate whether the regulation of Cx40 expression by KLF4 is direct or involves other pathways, we performed ChIP on bEnd.3 cells using an antibody directed against mouse KLF4. To ensure the efficacy of KLF4 immunoprecipitation, we first investigated the FSP1 promoter, which is known to be regulated by KLF4 through direct binding (Cuttano et al., 2016). Indeed, we observed an enrichment of the specific FSP1 promoter locus, thus validating this mouse KLF4 antibody for the ChIP procedure (Figure 2F). Similarly, three potential KLF4-binding sites were investigated in the Cx40 promoter region. We observed an enrichment of all three selected promoter loci with the region located 2,599 bp upstream from the transcription start site being mostly enriched compared to control IgG (Figure 2F). Altogether, these results indicate that KLF4 binds directly to at least three loci in the Cx40 promoter.

Cx40-Dependent Flow-Induced Differential Gene Expression

Although the importance of Cx40 for the maintenance of a healthy quiescent endothelium has become increasingly clear (Chadjichristos et al., 2010; Denis et al., 2017), no unbiased large-scale functional analysis to detail the participating signaling pathways has been performed until now. To shed light on the Cx40-dependent signaling pathways in the endothelium under various shear stress conditions, we performed RNAseq. First, we compared differential gene expression between HLSS and OSS under control conditions or after knock-down of Cx40. For each comparison between up- and down-regulated genes, genes with a fold-change and P-values thresholds higher than 2 and lower than 0.01, respectively, were considered as differentially expressed. Remarkably, comparing bEnd.3 cells exposed to similar shear stresses but silenced or not for Cx40 resulted in a significant differential expression of only one gene out of the approximately 10,450 tested, namely Gja5 (encoding Cx40) (Figures 3A,B). This not only illustrates the effective silencing of Cx40 but also validates the reproducibility of the experiment. As expected, under control conditions (siNT) OSS induced a considerable change in the gene expression profile with 18 genes being up-regulated and 68 genes down-regulated when compared to HLSS (Figure 3C and Supplementary Tables 1, 2). Further analyses of these differentially expressed genes revealed groups involved in various atherosclerosis-related processes such as inflammation (16), angiogenesis (15), metabolic processes (7), endothelial permeability (5), ECM interaction (4), vascular tone (3) and immune response (2), as shown in Figure 3E. After effective knock-down of Cx40, the total number of differentially expressed genes under OSS was rather similar, with 11 genes being up-regulated and 64 genes down-regulated when compared to HLSS (Figure 3D and Supplementary Tables 3, 4). However, the relative contribution of genes involved in inflammation increased from 31 to 43% and genes involved in endothelial permeability were no longer differentially expressed after silencing of Cx40 (Figure 3F). Finally, we observed a considerable overlap between the differentially expressed genes under OSS (as compared to HLSS) with or without Cx40 silencing. As shown in Figure 3G, 47 genes were commonly down-regulated and four genes commonly up-regulated, thus more than half of the OSS-induced differentially expressed genes were regulated independently from the Cx40 expression level.

FIGURE 3
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Figure 3. Cx40-dependent flow-induced differential gene expression. (A–D) Differential gene expression in bEnd.3 cells exposed to HLSS or OSS after treatment with siNT or Cx40 siRNA. Volcano plots show relationship between degree of gene expression change (log2 of fold-change; x-axis) and statistical significance of this change (–log10 of P-value; y-axis). Colored dots represent differentially expressed genes (P-value < 0.01) with fold-change >2 that are down-regulated (red) or up-regulated (blue). (A) Differential gene expression in ECs exposed to HLSS after treatment siCx40 compared to siNT. (B) Differential gene expression in ECs exposed to OSS after treatment with siCx40 compared to siNT. (C) Differential gene expression in siNT-treated (control) ECs exposed to HLSS compared to OSS. (D) Differential gene expression in siCx40-treated ECs exposed to HLSS compared to OSS. (E,F) Pie chart representation for differentially expressed genes organized for seven atherosclerosis-related processes, i.e., inflammation (dark blue), ECM interaction (orange), permeability (gray), angiogenesis (yellow), metabolic processes (light blue), vascular tone (green), and immune response (lilac). Differential expressed genes between siNT-treated (E) or siCx40-treated (F) cells exposed to HLSS compared to OSS. (G) Venn diagram representing gene overlap in OSS (as compared to HLSS) with or without Cx40 silencing. Highlighted are 47 and 4 genes that are commonly up- or down-regulated, respectively. (H) Gene set enrichment analysis of pathways in bEnd.3 cells exposed to HLSS after treatment with siNT or siCx40. Colored dots represent differentially regulated pathways (FDR < 0.05) with NES > 1 which involve genes that are down-regulated (red) or up-regulated (blue).

Next, we performed GSEA to identify essential pathways that are regulated by Cx40 under specific shear stress conditions. As Cx40 expression level in arterial regions exposed to OSS is rather low and Cx40 expression is down-regulated by OSS in vitro (Denis et al., 2017), we decided to focus on the HLSS conditions. Of the 483 pathways tested, 16 were up-regulated and 48 down-regulated when comparing ECs with a knock-down of Cx40 with control ECs under HLSS (Figure 3H and Supplementary Tables 5, 6). Whereas the top enriched up-regulated pathways in control ECs under HLSS show large diversity, the top enriched down-regulated pathways however point rather uniformly to signaling pathways involved in DNA repair and cell cycle control, suggesting a potential role for Cx40 in this process.

Cx40-Dependent Cell Proliferation

The role of Cxs in tumor growth has long been recognized (Aasen et al., 2016). In addition, ECs in straight parts of arteries display a quiescent state (Kwak et al., 2014). To obtain insight in candidate genes that might participate to the regulation of EC proliferation by Cx40, we performed leading-edge analysis of the GSEA results. Extraction of the core members of high scoring gene sets that contributed to the GSEA score identified the Replication proteins a1 and a3 (Rpa1, Rpa3), the proliferating cell nuclear antigen (Pcna) and DNA polymerases (Pold1, Pold2, and Pole) as genes with high number of occurrences (Figure 4A) among which Pcna displayed a high fold-change (Figure 4B). To investigate whether Cx40 plays a role in the inhibition of proliferation in ECs exposed to HLSS, we treated bEnd.3 cells with siCx40 and siNT for 24 h and subsequently exposed them to 24 h of HLSS. The ECs in which Cx40 was effectively silenced displayed an almost doubled proportion of PCNA-positive cells (Figures 4C,D), indicating an increased proliferation rate. Moreover, FACS-based cell cycle analysis revealed that the proportion of cells in the resting G0 or G1 phase was decreased by 9% in ECs with effective Cx40 silencing (Figure 4E).

FIGURE 4
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Figure 4. Cx40 controls EC proliferation. (A,B) Heat-maps visualizing leading-edge analysis of GSEA results, in which color intensity represents the number of occurrences (A) or the fold-change of each gene (B). Adjusted P-values were all <0.001. (C) Representative images of PCNA expression (green) in bEnd.3 cells after treatment with siNT or siCx40 and exposed to HLSS for 48 h. Nuclei were stained with DAPI (blue). Scale bar represents 50 μm. (D) Quantification of B. N = 4. (E) Cell cycle distribution (G0/G1, S, G2) in bEnd.3 cells exposed to 48 h of HLSS and analyzed by FACS after staining with Hoechst 33342. (F) Proportion of PCNA+ parental HeLa cells or HeLa cells expressing Cx40. N = 4.

To investigate whether the inhibitory effect of Cx40 on EC proliferation could be generalized to other cell types, we used Cx-deficient parental HeLa cells and HeLa cells stably transfected with Cx40. Transfected HeLa cells showed a high expression of Cx40 located at cell–cell contacts and efficient gap junctional coupling following microinjection of fluorescent dye, as reported previously (Denis et al., 2017). Interestingly, the proportion of PCNA-positive cells was reduced to half as compared to parental Cx-deficient HeLa cells (Figure 4F), pointing to a ubiquitous role of Cx40 in cell cycle control. Together, these results suggest that Cx40 regulation by HLSS may be involved in the maintenance of a quiescent endothelium.

Cx40 Contributes to EC Proliferation in vivo

During vascular development in zebrafish, small caliber ISVs sprout from the DA by angiogenesis and give rise to the DLAV, processes that require careful orchestration of cell behavior of adjacent ECs (see Figure 5A for examples). The arterial/venous identity of ECs in the developing zebrafish is determined before circulation begins (Lawson and Weinstein, 2002). To investigate the role of endothelial Cx40 on EC proliferation in vivo, we used zebrafish with knock-out mutations in Cx41.8 (t1) and Cx45.6 genes as well as with a Cx41.8 (tq) mutation that leads to reduced gap junction channel function (Figure 5B) (Watanabe et al., 2006). These zebrafish Cx40 orthologs both show a high degree of homology to mammalian Cx40 (Supplementary Table 7). We first determined the expression of the Cx40 orthologs in Tg(flk1:eGFP) embryos. Thus, cells were dissociated from 24 hpf embryos and FACS-sorted, and the expression of Cx41.8 and Cx45.6 was assessed in eGFP+ and eGPF- populations by qPCR. We found that Cx41.8 and Cx45.6 transcripts were, respectively, 32 and 13 times enriched in eGFP+ cells, indicating considerable expression of these Cxs in the endothelium of zebrafish embryos (Figures 5C,D). Next, we compared the progress of ISV formation at 28 hpf in Tg(flk1:eGFP), Tg(flk1:eGFP)Cx41.8t1/t1, Tg(flk1:eGFP)Cx41.8tq/tq and Tg(flk1:eGFP)Cx41.8t1/t1Cx45.6-/- embryos. Whereas only 11% of ISVs in Tg(flk1:eGFP) control embryos displayed completed branching for DLAV formation, this was enhanced to over 50% in all Cx41.8/Cx45.6 mutant embryos (Figures 5E,F). Interestingly, the Cx41.8tq/tq mutant showed most advanced vascular development at 28 hpf (Figures 5E,F), suggesting that channel-dependent rather than channel-independent effects are involved in the mechanism linking Cx40 to cell proliferation. Of note, compensatory upregulation of Cx45.6 expression in Cx41.8t1/t1 and Cx41.8tq/tq mutants was excluded as their mRNA level for this Cx was not different from Tg(flk1:eGFP) controls (Figure 5G). To investigate the effects of Cx40 channel-dependent intercellular communication on cell proliferation in vivo, we performed immunostainings for the proliferation marker PH3 in Tg(flk1:eGFP) and Tg(flk1:eGFP)Cx41.8tq/tq embryos (Figure 5H). The number of PH3-positive cells was significantly higher in the ISVs of Tg(flk1:eGFP)Cx41.8tq/tq embryos than in Tg(flk1:eGFP) controls, suggesting that the enhanced speed of ISV formation in Tg(flk1:eGFP)Cx41.8tq/tq embryos is, at least in part, due to increased proliferation of ECs (Figure 5I). Overall, our study demonstrates that Cx40 is a critical regulator of EC proliferation in vitro and in vivo, a function that appears preserved during evolution.

FIGURE 5
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Figure 5. Cx40 contributes to EC proliferation in vivo. (A) Vascular development in Tg(flk1:eGFP) zebrafish embryos at 24 and 48 hpf. Intersegmental vessels (ISVs) sprout from the dorsal aorta (DA) and give rise to the dorsal longitudinal anastomotic vessel (DLAV). (B) Schematic representation of location of leot1 and leotq mutation in Cx41.8. (C,D) Cx41.8 and Cx45.6 expression in eGFP+ and eGFP- cells isolated from Tg(flk1:eGFP) zebrafish embryos at 24 hpf was assessed by qPCR. N = 3. (E) Progress of ISV formation at 28 hpf in Tg(flk1:eGFP) (control; N = 7), Tg(flk1:eGFP)Cx41.8tq/tq (N = 6), Tg(flk1:eGFP)Cx41.8t1/t1 (N = 6) and Tg(flk1:eGFP)Cx41.8t1/t1Cx45.6-/- (N = 7) embryos. (F) Scores are: partial ISV sprouts (in black), complete ISVs (in gray) and ISVs with complete DLAV branching (in white). (G) Cx45.6 expression in eGFP+ cells isolated from Tg(flk1:eGFP), Tg(flk1:eGFP)Cx41.8tq/tq and Tg(flk1:eGFP)Cx41.8t1/t1 embryos at 24 hpf was assessed by qPCR. N = 3. (H) Examples of PH3 staining (in red) during ISV formation at 24 hpf in Tg(flk1:eGFP) and Tg(flk1:eGFP)Cx41.8tq/tq embryos. Arrows indicate PH3+ cells. (I) PH3 positive nuclei in proximal ISVs of Tg(flk1:eGFP) (control N = 23) and Tg(flk1:eGFP)Cx41.8tq/tq (N = 23) embryos at 24 hpf.

Discussion

Using in vitro experiments and a large-scale functional analysis, we confirm here that Cx40 expression is regulated by shear stress, being gradually up-regulated by laminar shear stress. We demonstrated that flow-induced Cx40 expression is directly controlled by the transcription factor KLF4. Using RNAseq and GSEA, cell cycle progression was identified as an important downstream target of Cx40 under HLSS. The functional role of Cx40 in the control of cell proliferation was supported by further in vitro studies and in a zebrafish model. Overall, our study demonstrates that Cx40 is a critical regulator of EC proliferation in vitro and in vivo, thereby likely contributing to endothelial quiescence in healthy arteries and restraining vascular development.

KLF2 and KLF4 are key controllers of endothelial homeostasis in large arteries (Atkins and Jain, 2007). Endothelial-specific ablation of both Klf2 and Klf4 genes in adult mice demonstrated the absolute requirement of these two KLFs to maintain normal endothelial physiology and vessel integrity in the adult animal (Sangwung et al., 2017). We have previously shown in EC cultures that KLF2 directly binds to the Cx37 promoter and induces its expression under HLSS (Pfenniger et al., 2012). Reduction of KLF2 in vitro did not affect Cx40 expression. In this study, we show that KLF4 binds to the Cx40 promoter and gradually regulates its expression in response to increasing levels of shear stress. Of note, KLF4 silencing did not affect Cx37 expression. The KLF-specific regulation of endothelial Cxs in vitro is mirrored by the responses of these Cxs to carotid casting in vivo. Indeed, Cx37 expression was low in regions of imposed LLSS as well as OSS, however, Cx40 expression was only down-regulated in the OSS region (Pfenniger et al., 2012; Denis et al., 2017). The reason and significance of the different KLF2-Cx37 vs. KLF4-Cx40 induction set-points for arterial physiology remains to be investigated. In this respect, it is noteworthy that hypermethylation of the KLF4 promoter has been observed in regions with disturbed blood flow (Jiang et al., 2014). Indeed, flow-dependent epigenomic DNA methylation patterns alter endothelial gene expression, thereby regulating vascular biology and disease (Dunn et al., 2015). Whether, the differential levels of promoter methylation may explain the gradual induction of KLF4 expression by laminar shear stress remains to be investigated as well.

Small metabolites conveyed through gap junctions but also channel-independent effector functions of the cytosolic C-terminal domain (CT) of Cxs control crucial cell processes, including cell growth, in physiology and disease (Naus and Laird, 2010; Kibschull et al., 2015; Leithe et al., 2018). Tissue ischemia activates a cascade of vasodilatory, inflammatory and remodeling processes and endothelial Cxs are increasingly recognized to orchestrate these events. Indeed, Cx37-deficient mice were shown to recover ischemic hind limb function faster and to a greater extent than wild-type animals (Fang et al., 2012). Cx37 appeared to limit recovery from ischemic hind limb injury by exerting growth suppressive effects on arteriogenic and angiogenic responses to ischemia (Fang et al., 2011). In contrast, Cx40-deficient mice exhibited profound and rapid failure of limb survival after an ischemic insult (Fang et al., 2012) due to compromised regulation of tissue perfusion, vascular remodeling and a prolonged inflammatory response (Fang et al., 2013). Targeting endothelial Cx40 in mice reduces angiogenesis in the developing retina and in a tumor setting (Alonso et al., 2016; Haefliger et al., 2017). Although Cx40 expression levels are not affected in Cx37 knock-out mice (Wong et al., 2006), Cx37 expression levels are severely reduced in Cx40-deficient mice (Chadjichristos et al., 2010; Meens et al., 2015), making it impossible to ascribe the above-described effects in Cx40-deficient animals exclusively to this endothelial Cx. Here, we used a RNA silencing rather than a knock-out approach to down-regulate Cx40 expression and this procedure did not affect the expression levels of Cx37, as demonstrated in the RNAseq data (fold-change Gja4: 1.017). Thus, our study permits to investigate the selective function of Cx40 in EC growth. The RNAseq/GSEA revealed significant up-regulation of pathways related to cell cycle control in ECs with knock-down of Cx40 exposed to arterial flow rates (Figures 3H, 4A,B and Supplementary Table 6) and involved genes encoding for replication proteins DNA polymerases and PCNA. Moreover, we showed that the proliferation rate was increased in ECs treated with siCx40 under these flow conditions (Figures 4C,D). Interestingly, proliferation rate of HeLa cells was decreased after transfection of Cx40 in this Cx-deficient cell line (Figure 4F). This illustrates not only that the inverse relation between Cx40 levels and cell proliferation may be extended to another (epithelial) cell type, but also that this relation is independent of which promoter was used for induction of Cx40 expression. In further support of this hypothesis are preliminary experiments using the silent heart zebrafish model Tg(flk1:eGFP) sih-/- showing at 48 hpf similar Cx41.8 and Cx45.6 expression levels in absence of blood flow than in littermate Tg(flk1:eGFP) sih+/- and Tg(flk1:eGFP) sih+/+ controls with beating heart (data not shown). Taken together, our data show that Cx40 is a critical regulator of the inhibition of EC proliferation. Whether the regulation of EC proliferation in healthy arteries depends on the synchronization of endothelial responses via gap junctions or channel-independent effects of Cx40 remains to be investigated.

Growth control by Cxs, in particular Cx43, does not always correlate with the extent of gap junctional communication (Moorby and Patel, 2001; Qin et al., 2002). Moreover, ectopic expression of Cx43-CT in, for example, mouse neuroblastoma cells suppressed the growth of these cells to a similar extent as expression of full-length Cx43 (Moorby and Patel, 2001). Mechanistically, it has been shown that Cx43-CT promotes the degradation of S phase kinase-associated protein 2 (Skp2), which subsequently affects p27 degradation and cell growth (Zhang et al., 2003). In addition, direct interactions of Cx43-CT allowing for crosstalk with regulators of cell growth, including β-Catenin, CCN3, c-Src and Cyclin E, have been previously found (Leybaert et al., 2017; Leithe et al., 2018). Interestingly, Cx43 mRNA undergoes alternative translation to generate N-terminal truncated isoforms (Smyth and Shaw, 2013; Salat-Canela et al., 2014). An increasing number of pathophysiological roles are currently ascribed to this Cx43-20k isoform, including actin- and microtubule-based protein transport and epithelial–mesenchymal transition (Basheer et al., 2017; Fu et al., 2017; James et al., 2018). Knowledge on Cx40-CT interacting proteins is limited and whether alternative translation of Cx40 mRNA occurs is presently a matter of debate.

In addition to channel-independent effects, synchronization of cellular responses via gap junctions has also been demonstrated to control cancer cell growth (Chandrasekhar et al., 2013). Mechanistically, intercellular redistribution of cAMP throughout a cell population by open Cx26 gap junction channels appeared to eliminate the cell cycle-dependent oscillations in cAMP in individual cells, thereby inhibiting cell cycle progression. By acting as a pathway to “sink” cAMP, gap junctional communication may thus provide a general means to limit the mitotic rate of cell populations (Chandrasekhar et al., 2013). As cAMP has been shown to permeate Cx40 channels (Kanaporis et al., 2008), a gap junction channel-dependent effect of Cx40 on cell growth inhibition in healthy arterial endothelium may involve a similar mechanism. In line with this hypothesis, zebrafish embryos knock-out for Cx40 orthologs showed faster vascular development, an effect that was further strengthened by potential dominant negative effects of the Cx41.8tq mutant on gap junctional channels formed by other Cxs in the endothelium (Figures 5E,F). Moreover, preliminary experiments on low-density cultures seem not to recapitulate the Cx40-dependent proliferation inhibition observed in HeLa transfectants (data not shown).

Continued research efforts are performed to develop pharmacological strategies aimed at preventing excessive EC proliferation in for instance diabetic retinopathy or tumor growth. Recent studies, including ours, have demonstrated that Cx40 may represent an attractive novel target for the development of molecules that promote endothelial quiescence.

Author Contributions

J-FD, MD, FM, AH, TL, and SL performed the experiments and/or analyzed the data. BK designed the research. MW, SL, and JB participated to the design of some experiments. J-FD and BK wrote the manuscript. All co-authors corrected the manuscript.

Funding

This work was supported by grants from the Swiss National Science Foundation (310030_162579 and 310030_182573 to BK and 310030_166515 to JB) and the Swiss SystemsX.ch initiative, evaluated by the Swiss National Science Foundation (to BK).

Conflict of Interest Statement

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.

Acknowledgments

We thank Julien Vermot (University of Strasbourg, France) for sending sih embryos, and Graziano Pelli, Bernard Foglia, Tahir Idris and the Genomic platform of the University of Geneva for excellent technical help.

Supplementary Material

The Supplementary Material for this article can be found online at: https://www.frontiersin.org/articles/10.3389/fphys.2019.00080/full#supplementary-material

Footnotes

  1. ^https://www.genomatix.de
  2. ^http://www.wikipathways.org/index.php/WikiPathways
  3. ^http://www.genome.jp/kegg/

References

Aasen, T., Mesnil, M., Naus, C. C., Lampe, P. D., and Laird, D. W. (2016). Gap junctions and cancer: communicating for 50 years. Nat. Rev. Cancer 16, 775–788. doi: 10.1038/nrc.2016.105

PubMed Abstract | CrossRef Full Text | Google Scholar

Alonso, F., Domingos-Pereira, S., Le Gal, L., Derre, L., Meda, P., Jichlinski, P., et al. (2016). Targeting endothelial connexin40 inhibits tumor growth by reducing angiogenesis and improving vessel perfusion. Oncotarget 7, 14015–14028. doi: 10.18632/oncotarget.7370

PubMed Abstract | CrossRef Full Text | Google Scholar

Atkins, G. B., and Jain, M. K. (2007). Role of Kruppel-like transcription factors in endothelial biology. Circ. Res. 100, 1686–1695. doi: 10.1161/01.RES.0000267856.00713.0a

PubMed Abstract | CrossRef Full Text | Google Scholar

Basheer, W. A., Xiao, S., Epifantseva, I., Fu, Y., Kleber, A. G., Hong, T., et al. (2017). GJA1-20k arranges actin to guide cx43 delivery to cardiac intercalated discs. Circ. Res. 121, 1069–1080. doi: 10.1161/CIRCRESAHA.117.311955

PubMed Abstract | CrossRef Full Text | Google Scholar

Brown, A. J., Teng, Z., Evans, P. C., Gillard, J. H., Samady, H., and Bennett, M. R. (2016). Role of biomechanical forces in the natural history of coronary atherosclerosis. Nat. Rev. Cardiol. 13, 210–220. doi: 10.1038/nrcardio.2015.203

PubMed Abstract | CrossRef Full Text | Google Scholar

Chadjichristos, C. E., Scheckenbach, K. E., van Veen, T. A., Richani Sarieddine, M. Z., de Wit, C., Yang, Z., et al. (2010). Endothelial-specific deletion of connexin40 promotes atherosclerosis by increasing CD73-dependent leukocyte adhesion. Circulation 121, 123–131. doi: 10.1161/CIRCULATIONAHA.109.867176

PubMed Abstract | CrossRef Full Text | Google Scholar

Chandrasekhar, A., Kalmykov, E. A., Polusani, S. R., Mathis, S. A., Zucker, S. N., and Nicholson, B. J. (2013). Intercellular redistribution of cAMP underlies selective suppression of cancer cell growth by connexin26. PLoS One 8:e82335. doi: 10.1371/journal.pone.0082335

PubMed Abstract | CrossRef Full Text | Google Scholar

Chen, J. N., Haffter, P., Odenthal, J., Vogelsang, E., Brand, M., van Eeden, F. J., et al. (1996). Mutations affecting the cardiovascular system and other internal organs in zebrafish. Development 123, 293–302.

PubMed Abstract | Google Scholar

Cruciani, V., and Mikalsen, S. O. (2007). Evolutionary selection pressure and family relationships among connexin genes. Biol. Chem. 388, 253–264. doi: 10.1515/BC.2007.028

PubMed Abstract | CrossRef Full Text | Google Scholar

Cuttano, R., Rudini, N., Bravi, L., Corada, M., Giampietro, C., Papa, E., et al. (2016). KLF4 is a key determinant in the development and progression of cerebral cavernous malformations. EMBO Mol. Med. 8, 6–24. doi: 10.15252/emmm.201505433

PubMed Abstract | CrossRef Full Text | Google Scholar

Davies, P. F., Civelek, M., Fang, Y., and Fleming, I. (2013). The atherosusceptible endothelium: endothelial phenotypes in complex haemodynamic shear stress regions in vivo. Cardiovasc. Res. 99, 315–327. doi: 10.1093/cvr/cvt101

PubMed Abstract | CrossRef Full Text | Google Scholar

Dekker, R. J., van Thienen, J. V., Rohlena, J., de Jager, S. C., Elderkamp, Y. W., Seppen, J., et al. (2005). Endothelial KLF2 links local arterial shear stress levels to the expression of vascular tone-regulating genes. Am. J. Pathol. 167, 609–618. doi: 10.1016/S0002-9440(10)63002-7

PubMed Abstract | CrossRef Full Text | Google Scholar

Denis, J.-F., Scheckenbach, L., Pfenniger, A., Meens, M., Krams, R., Miquerol, L., et al. (2017). Connexin40 controls endothelial activation by dampening NFkB activation. Oncotarget 8, 50972–50986. doi: 10.18632/oncotarget.16438

PubMed Abstract | CrossRef Full Text | Google Scholar

Dobin, A., Davis, C. A., Schlesinger, F., Drenkow, J., Zaleski, C., Jha, S., et al. (2013). STAR: ultrafast universal RNA-seq aligner. Bioinformatics 29, 15–21. doi: 10.1093/bioinformatics/bts635

PubMed Abstract | CrossRef Full Text | Google Scholar

Dunn, J., Thabet, S., and Jo, H. (2015). Flow-Dependent epigenetic DNA methylation in endothelial gene expression and atherosclerosis. Arterioscler. Thromb. Vasc. Biol. 35, 1562–1569. doi: 10.1161/ATVBAHA.115.305042

PubMed Abstract | CrossRef Full Text | Google Scholar

Eastman, S. D., Chen, T. H., Falk, M. M., Mendelson, T. C., and Iovine, M. K. (2006). Phylogenetic analysis of three complete gap junction gene families reveals lineage-specific duplications and highly supported gene classes. Genomics 87, 265–274. doi: 10.1016/j.ygeno.2005.10.005

PubMed Abstract | CrossRef Full Text | Google Scholar

Elfgang, C., Eckert, R., Lichtenberg-Frate, H., Butterweck, A., Traub, O., Klein, R. A., et al. (1995). Specific permeability and selective formation of gap junction channels in connexin-transfected HeLa cells. J. Cell. Biol. 129, 805–817. doi: 10.1083/jcb.129.3.805

PubMed Abstract | CrossRef Full Text | Google Scholar

Fang, J. S., Angelov, S. N., Simon, A. M., and Burt, J. M. (2011). Cx37 deletion enhances vascular growth and facilitates ischemic limb recovery. Am. J. Physiol. Heart Circ. Physiol. 301, H1872–H1881. doi: 10.1152/ajpheart.00683.2011

PubMed Abstract | CrossRef Full Text | Google Scholar

Fang, J. S., Angelov, S. N., Simon, A. M., and Burt, J. M. (2012). Cx40 is required for, and cx37 limits, postischemic hindlimb perfusion, survival and recovery. J. Vasc. Res. 49, 2–12. doi: 10.1159/000329616

PubMed Abstract | CrossRef Full Text | Google Scholar

Fang, J. S., Angelov, S. N., Simon, A. M., and Burt, J. M. (2013). Compromised regulation of tissue perfusion and arteriogenesis limit, in an AT1R-independent fashion, recovery of ischemic tissue in Cx40(-/-) mice. Am. J. Physiol. Heart Circ. Physiol. 304, H816–H827. doi: 10.1152/ajpheart.00719.2012

PubMed Abstract | CrossRef Full Text | Google Scholar

Fu, Y., Zhang, S. S., Xiao, S., Basheer, W. A., Baum, R., Epifantseva, I., et al. (2017). Cx43 Isoform GJA1-20k promotes microtubule dependent mitochondrial transport. Front. Physiol. 8:905. doi: 10.3389/fphys.2017.00905

PubMed Abstract | CrossRef Full Text | Google Scholar

Gabriels, J. E., and Paul, D. L. (1998). Connexin43 is highly localized to sites of disturbed flow in rat aortic endothelium but connexin37 and connexin40 are more uniformly distributed. Circ. Res. 83, 636–643. doi: 10.1161/01.RES.83.6.636

PubMed Abstract | CrossRef Full Text | Google Scholar

Haefliger, J. A., Allagnat, F., Hamard, L., Le Gal, L., Meda, P., Nardelli-Haefliger, D., et al. (2017). Targeting Cx40 (Connexin40) expression or function reduces angiogenesis in the developing mouse retina. Arterioscler. Thromb. Vasc. Biol. 37, 2136–2146. doi: 10.1161/ATVBAHA.117.310072

PubMed Abstract | CrossRef Full Text | Google Scholar

Huang, T. Y., Chu, T. F., Chen, H. I., and Jen, C. J. (2000). Heterogeneity of [Ca(2+)](i) signaling in intact rat aortic endothelium. FASEB J. 14, 797–804. doi: 10.1096/fasebj.14.5.797

CrossRef Full Text | Google Scholar

James, C. C., Zeitz, M. J., Calhoun, P. J., Lamouille, S., and Smyth, J. W. (2018). Altered translation initiation of Gja1 limits gap junction formation during epithelial-mesenchymal transition. Mol. Biol. Cell. 29, 797–808. doi: 10.1091/mbc.E17-06-0406

PubMed Abstract | CrossRef Full Text | Google Scholar

Jiang, Y. Z., Jimenez, J. M., Ou, K., McCormick, M. E., Zhang, L. D., and Davies, P. F. (2014). Hemodynamic disturbed flow induces differential DNA methylation of endothelial Kruppel-Like Factor 4 promoter in vitro and in vivo. Circ. Res. 115, 32–43. doi: 10.1161/CIRCRESAHA.115.303883

PubMed Abstract | CrossRef Full Text | Google Scholar

Jin, S. W., Beis, D., Mitchell, T., Chen, J. N., and Stainier, D. Y. (2005). Cellular and molecular analyses of vascular tube and lumen formation in zebrafish. Development 132, 5199–5209. doi: 10.1242/dev.02087

PubMed Abstract | CrossRef Full Text | Google Scholar

Kanaporis, G., Mese, G., Valiuniene, L., White, T. W., Brink, P. R., and Valiunas, V. (2008). Gap junction channels exhibit connexin-specific permeability to cyclic nucleotides. J. Gen. Physiol. 131, 293–305. doi: 10.1085/jgp.200709934

PubMed Abstract | CrossRef Full Text | Google Scholar

Kibschull, M., Gellhaus, A., Carette, D., Segretain, D., Pointis, G., and Gilleron, J. (2015). Physiological roles of connexins and pannexins in reproductive organs. Cell. Mol. Life Sci. 72, 2879–2898. doi: 10.1007/s00018-015-1965-4

PubMed Abstract | CrossRef Full Text | Google Scholar

Kwak, B. R., Back, M., Bochaton-Piallat, M. L., Caligiuri, G., Daemen, M. J., Davies, P. F., et al. (2014). Biomechanical factors in atherosclerosis: mechanisms and clinical implications. Eur. Heart J. 35, 3013–3020. doi: 10.1093/eurheartj/ehu353

PubMed Abstract | CrossRef Full Text | Google Scholar

Kwak, B. R., Pepper, M. S., Gros, D. B., and Meda, P. (2001). Inhibition of endothelial wound repair by dominant negative connexin inhibitors. Mol. Biol. Cell. 12, 831–845. doi: 10.1091/mbc.12.4.831

PubMed Abstract | CrossRef Full Text | Google Scholar

Lawson, N. D., and Weinstein, B. M. (2002). Arteries and veins: making a difference with zebrafish. Nat. Rev. Genet 3, 674–682. doi: 10.1038/nrg888

PubMed Abstract | CrossRef Full Text | Google Scholar

Leithe, E., Mesnil, M., and Aasen, T. (2018). The connexin 43 C-terminus: a tail of many tales. Biochim. Biophys. Acta 1860, 48–64. doi: 10.1016/j.bbamem.2017.05.008

PubMed Abstract | CrossRef Full Text | Google Scholar

Leybaert, L., Lampe, P. D., Dhein, S., Kwak, B. R., Ferdinandy, P., Beyer, E. C., et al. (2017). Connexins in cardiovascular and neurovascular health and disease: pharmacological implications. Pharmacol. Rev. 69, 396–478. doi: 10.1124/pr.115.012062

PubMed Abstract | CrossRef Full Text | Google Scholar

Meens, M. J., Alonso, F., Le Gal, L., Kwak, B. R., and Haefliger, J. A. (2015). Endothelial connexin37 and connexin40 participate in basal but not agonist-induced no release. Cell. Commun. Signal. 13:34. doi: 10.1186/s12964-015-0110-1

PubMed Abstract | CrossRef Full Text | Google Scholar

Misu, A., Yamanaka, H., Aramaki, T., Kondo, S., Skerrett, I. M., Iovine, M. K., et al. (2016). Two different functions of connexin43 confer two different bone phenotypes in zebrafish. J. Biol. Chem. 291, 12601–12611. doi: 10.1074/jbc.M116.720110

PubMed Abstract | CrossRef Full Text | Google Scholar

Molica, F., Figueroa, X. F., Kwak, B. R., Isakson, B. E., and Gibbins, J. M. (2018). Connexins and pannexins in vascular function and disease. Int. J. Mol. Sci. 19:E1663. doi: 10.3390/ijms19061663

PubMed Abstract | CrossRef Full Text | Google Scholar

Moorby, C., and Patel, M. (2001). Dual functions for connexins: Cx43 regulates growth independently of gap junction formation. Exp. Cell Res. 271, 238–248. doi: 10.1006/excr.2001.5357

PubMed Abstract | CrossRef Full Text | Google Scholar

Mootha, V. K., Lindgren, C. M., Eriksson, K. F., Subramanian, A., Sihag, S., Lehar, J., et al. (2003). PGC-1alpha-responsive genes involved in oxidative phosphorylation are coordinately downregulated in human diabetes. Nat. Genet 34, 267–273. doi: 10.1038/ng1180

PubMed Abstract | CrossRef Full Text | Google Scholar

Morbiducci, U., Kok, A. M., Kwak, B. R., Stone, P. H., Steinman, D. A., and Wentzel, J. J. (2016). Atherosclerosis at arterial bifurcations: evidence for the role of haemodynamics and geometry. Thromb. Haemost. 115, 484–492. doi: 10.1160/TH15-07-0597

PubMed Abstract | CrossRef Full Text | Google Scholar

Naus, C. C., and Laird, D. W. (2010). Implications and challenges of connexin connections to cancer. Nat. Rev. Cancer 10, 435–441. doi: 10.1038/ nrc2841

PubMed Abstract | CrossRef Full Text | Google Scholar

Pfenniger, A., Wong, C., Sutter, E., Cuhlmann, S., Dunoyer-Geindre, S., Mach, F., et al. (2012). Shear stress modulates the expression of the atheroprotective protein Cx37 in endothelial cells. J. Mol. Cell. Cardiol. 53, 299–309. doi: 10.1016/j.yjmcc.2012.05.011

PubMed Abstract | CrossRef Full Text | Google Scholar

Pogoda, K., Kameritsch, P., Mannell, H., and Pohl, U. (2018). Connexins in the control of vasomotor function. Acta Physiol. 225:e13108. doi: 10.1111/apha.13108

PubMed Abstract | CrossRef Full Text | Google Scholar

Qin, H., Shao, Q., Curtis, H., Galipeau, J., Belliveau, D. J., Wang, T., et al. (2002). Retroviral delivery of connexin genes to human breast tumor cells inhibits in vivo tumor growth by a mechanism that is independent of significant gap junctional intercellular communication. J. Biol. Chem. 277, 29132–29138. doi: 10.1074/jbc.M200797200

PubMed Abstract | CrossRef Full Text | Google Scholar

Quinlan, A. R., and Hall, I. M. (2010). BEDTools: a flexible suite of utilities for comparing genomic features. Bioinformatics 26, 841–842. doi: 10.1093/bioinformatics/btq033

PubMed Abstract | CrossRef Full Text | Google Scholar

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, 139–140. doi: 10.1093/bioinformatics/btp616

PubMed Abstract | CrossRef Full Text | Google Scholar

Salat-Canela, C., Sese, M., Peula, C., Ramon y Cajal, S., and Aasen, T. (2014). Internal translation of the connexin 43 transcript. Cell. Commun. Signal. 12:31. doi: 10.1186/1478-811X-12-31

PubMed Abstract | CrossRef Full Text | Google Scholar

Sangwung, P., Zhou, G., Nayak, L., Chan, E. R., Kumar, S., Kang, D. W., et al. (2017). KLF2 and KLF4 control endothelial identity and vascular integrity. JCI Insight 2:e91700. doi: 10.1172/jci.insight.91700

PubMed Abstract | CrossRef Full Text | Google Scholar

SenBanerjee, S., Lin, Z., Atkins, G. B., Greif, D. M., Rao, R. M., Kumar, A., et al. (2004). KLF2 Is a novel transcriptional regulator of endothelial proinflammatory activation. J. Exp. Med. 199, 1305–1315. doi: 10.1084/jem.20031132

PubMed Abstract | CrossRef Full Text | Google Scholar

Simmons, R. D., Kumar, S., and Jo, H. (2016). The role of endothelial mechanosensitive genes in atherosclerosis and omics approaches. Arch. Biochem. Biophys. 591, 111–131. doi: 10.1016/j.abb.2015.11.005

PubMed Abstract | CrossRef Full Text | Google Scholar

Smyth, J. W., and Shaw, R. M. (2013). Autoregulation of connexin43 gap junction formation by internally translated isoforms. Cell. Rep. 5, 611–618. doi: 10.1016/j.celrep.2013.10.009

PubMed Abstract | CrossRef Full Text | Google Scholar

Subramanian, A., Tamayo, P., Mootha, V. K., Mukherjee, S., Ebert, B. L., Gillette, M. A., et al. (2005). Gene set enrichment analysis: a knowledge-based approach for interpreting genome-wide expression profiles. Proc. Natl. Acad. Sci. U.S.A. 102, 15545–15550. doi: 10.1073/pnas.0506580102

PubMed Abstract | CrossRef Full Text | Google Scholar

Tabas, I., Garcia-Cardena, G., and Owens, G. K. (2015). Recent insights into the cellular biology of atherosclerosis. J. Cell. Biol. 209, 13–22. doi: 10.1083/jcb.201412052

PubMed Abstract | CrossRef Full Text | Google Scholar

Team, R. D. C. (2008). R: A Language and Environment for Statistical Computing. Vienna: R Foundation for Statistical Computing.

Google Scholar

Vorderwulbecke, B. J., Maroski, J., Fiedorowicz, K., Da Silva-Azevedo, L., Marki, A., Pries, A. R., et al. (2012). Regulation of endothelial connexin40 expression by shear stress. Am. J. Physiol. Heart Circ. Physiol. 302, H143–H152. doi: 10.1152/ajpheart.00634.2011

PubMed Abstract | CrossRef Full Text | Google Scholar

Warboys, C. M., de Luca, A., Amini, N., Luong, L., Duckles, H., Hsiao, S., et al. (2014). Disturbed flow promotes endothelial senescence via a p53-dependent pathway. Arterioscler. Thromb. Vasc. Biol. 34, 985–995. doi: 10.1161/ATVBAHA.114.303415

PubMed Abstract | CrossRef Full Text | Google Scholar

Watanabe, M. (2017). Gap junction in the teleost fish lineage: duplicated connexins may contribute to skin pattern formation and body shape determination. Front. Cell. Dev. Biol. 5:13. doi: 10.3389/fcell.2017.00013

PubMed Abstract | CrossRef Full Text | Google Scholar

Watanabe, M., Iwashita, M., Ishii, M., Kurachi, Y., Kawakami, A., Kondo, S., et al. (2006). Spot pattern of leopard Danio is caused by mutation in the zebrafish connexin41.8 gene. EMBO Rep. 7, 893–897. doi: 10.1038/sj.embor.7400757

PubMed Abstract | CrossRef Full Text | Google Scholar

Watanabe, M., Sawada, R., Aramaki, T., Skerrett, I. M., and Kondo, S. (2016). The physiological characterization of connexin41.8 and connexin39.4, which are involved in the striped pattern formation of zebrafish. J. Biol. Chem. 291, 1053–1063. doi: 10.1074/jbc.M115.673129

PubMed Abstract | CrossRef Full Text | Google Scholar

Westerfield, M. (2000). The Zebrafish Book. A Guide for the Laboratory Use of Zebrafish. Eugene, OR: University of Oregon Press.

Google Scholar

Wong, C. W., Christen, T., Roth, I., Chadjichristos, C. E., Derouette, J. P., Foglia, B. F., et al. (2006). Connexin37 protects against atherosclerosis by regulating monocyte adhesion. Nat. Med. 12, 950–954. doi: 10.1038/nm1441

PubMed Abstract | CrossRef Full Text | Google Scholar

Zhang, Y. W., Kaneda, M., and Morita, I. (2003). The gap junction-independent tumor-suppressing effect of connexin 43. J. Biol. Chem. 278, 44852–44856. doi: 10.1074/jbc.M305072200

PubMed Abstract | CrossRef Full Text | Google Scholar

Keywords: endothelium, shear stress, KLF4, Cx40, cell proliferation

Citation: Denis J-F, Diagbouga MR, Molica F, Hautefort A, Linnerz T, Watanabe M, Lemeille S, Bertrand JY and Kwak BR (2019) KLF4-Induced Connexin40 Expression Contributes to Arterial Endothelial Quiescence. Front. Physiol. 10:80. doi: 10.3389/fphys.2019.00080

Received: 11 September 2018; Accepted: 24 January 2019;
Published: 12 February 2019.

Edited by:

Jincai Luo, Peking University, China

Reviewed by:

Dong Liu, Nantong University, China
Jingjing Zhang, Affiliated Hospital of Guangdong Medical University, China
John Y. J. Shyy, University of California, San Diego, United States

Copyright © 2019 Denis, Diagbouga, Molica, Hautefort, Linnerz, Watanabe, Lemeille, Bertrand and Kwak. 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: Brenda R. Kwak, Brenda.KwakChanson@unige.ch

These authors have contributed equally to this work