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Article

Increased Expression of RUNX1 in Liver Correlates with NASH Activity Score in Patients with Non-Alcoholic Steatohepatitis (NASH)

by
Savneet Kaur
1,*,
Preety Rawal
2,†,
Hamda Siddiqui
1,2,†,
Sumati Rohilla
2,
Shvetank Sharma
1,
Dinesh M Tripathi
1,
Sukriti Baweja
1,
Mohsin Hassan
1,
Sebastian Vlaic
3,
Reinhard Guthke
3,
Maria Thomas
4,
Rania Dayoub
5,
Chaggan Bihari
1,
Shiv K. Sarin
1 and
Thomas S. Weiss
5,*
1
Institute of Liver and Biliary Sciences, New Delhi-110070, India
2
Department of Biotechnology, Gautam Buddha University, Greater Noida-201308, India
3
Leibniz Institute for Natural Product Research and Infection Biology—Hans Knöll-Institute, 07745 Jena, Germany
4
Dr. Margarete Fischer-Bosch Institute of Clinical Pharmacology, Stuttgart, and University of Tuebingen, 72076 Tuebingen, Germany
5
University Children Hospital (KUNO), University Hospital of Regensburg, 93053 Regensburg, Germany
*
Authors to whom correspondence should be addressed.
†
Contributed equally.
Cells 2019, 8(10), 1277; https://doi.org/10.3390/cells8101277
Submission received: 27 September 2019 / Revised: 16 October 2019 / Accepted: 16 October 2019 / Published: 18 October 2019
(This article belongs to the Special Issue Cellular and Molecular Mechanisms Underlying the Pathogenesis of Hepatic Fibrosis)
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Versions Notes

Abstract

:
Given the important role of angiogenesis in liver pathology, the current study investigated the role of Runt-related transcription factor 1 (RUNX1), a regulator of developmental angiogenesis, in the pathogenesis of non-alcoholic steatohepatitis (NASH). Quantitative RT-PCRs and a transcription factor analysis of angiogenesis-associated differentially expressed genes in liver tissues of healthy controls, patients with steatosis and NASH, indicated a potential role of RUNX1 in NASH. The gene expression of RUNX1 was correlated with histopathological attributes of patients. The protein expression of RUNX1 in liver was studied by immunohistochemistry. To explore the underlying mechanisms, in vitro studies using RUNX1 siRNA and overexpression plasmids were performed in endothelial cells (ECs). RUNX1 expression was significantly correlated with inflammation, fibrosis and NASH activity score in NASH patients. Its expression was conspicuous in liver non-parenchymal cells. In vitro, factors from steatotic hepatocytes and/or VEGF or TGF-β significantly induced the expression of RUNX1 in ECs. RUNX1 regulated the expression of angiogenic and adhesion molecules in ECs, including CCL2, PECAM1 and VCAM1, which was shown by silencing or over-expression of RUNX1. Furthermore, RUNX1 increased the angiogenic activity of ECs. This study reports that steatosis-induced RUNX1 augmented the expression of adhesion and angiogenic molecules and properties in ECs and may be involved in enhancing inflammation and disease severity in NASH.

Graphical Abstract

1. Introduction

Non-alcoholic fatty liver disease (NAFLD) includes a wide compass of liver pathologies, ranging from simple steatosis, usually a mild, benign and non-progressive condition, to non-alcoholic steatohepatitis (NASH), which may progress to liver cirrhosis and ultimately hepatocellular carcinoma (HCC). With NAFLD affecting both children and adults alike, it is postulated to emerge as the leading cause of end-stage liver diseases in the coming years [1]. Several cellular and molecular events conspire and collaborate to transform simple steatosis to NASH to HCC. However, the underlying precise mechanisms of disease pathogenesis and NAFLD progression have just begun to be understood. Some of the newly emerging concepts include iron overload, inflammation, dysregulated fat metabolism, oxidative stress, gut microbiota and angiogenesis [2].
Angiogenesis or new blood vessel formation is a crucial aspect of inflammation and a critical step in tissue damage, healing, and vascular remodeling. Changes in liver vascular architecture have been linked to the progression of fibrosis, cirrhosis and HCC in chronic liver diseases (CLD) [3,4]. Almost all experimental and clinical conditions of CLD, including NASH, have been associated with an over-expression of pro-angiogenic cytokines and related receptors. Although various studies have reported an upregulation of angiogenic factors, particularly VEGF in NASH, the underlying mechanisms that regulate angiogenesis, inflammation and fibrogenesis in NASH pathology remain obscure [5,6,7].
In the current study, we explored the role of Runt-related transcription factor 1 (RUNX1) in the pathogenesis of NASH. RUNX1, also known as acute myeloid leukemia 1 (AML1), is a powerful and pivotal regulator of hematopoiesis and angiogenesis [8,9]. A defect in RUNX1 is associated with impairment in angiogenesis accompanied by the absence of hematopoietic stem cells [10]. Given the significance of RUNX1 in angiogenesis and its rarely identified role in NASH, we investigated the expression and function of RUNX1 in NASH pathology by addressing its emergence in endothelial cells (ECs).

2. Materials and Methods

2.1. Study Subjects and Collection of Samples

Human liver tissues were histologically examined for patients without NAFLD (n = 33), patients with simple liver steatosis (n = 46) and patients with NASH (n = 43) as described earlier [11,12] (for tissue characteristics see Supplementary Table S1). A subset of these samples was used for a mRNA microarray analysis: patients without NAFLD (n = 7), patients with simple liver steatosis (n = 7), and with non-alcoholic steatohepatitis (NASH) (n = 7). The experimental procedures were performed according to the guidelines of the charitable state-controlled foundation HTCR (Human Tissue and Cell Research, Regensburg, Germany), with written informed consent from patients. The study in Germany and the consent form were approved by the local ethical committee of the University of Regensburg (ethics statement 12-101-0048, University of Regensburg, Germany). Additionally, immunohistochemistry (IHC) studies were conducted on liver biopsies collected from NASH patients’ samples (n = 16) and control liver tissues (n =10) collected in ILBS, New Delhi (for patient characteristics see Supplementary Table S2). The study performed in India was duly approved by the Human ethics committee of ILBS, New Delhi (ethics approval F25/5/64/ILBS/AC2014/1484). All experiments involving human tissues and cells were carried out in accordance to The Code of Ethics of the World Medical Association (Declaration of Helsinki).

2.2. Differential Gene Expression Studies and qRT-PCRs

About 17 differentially expressed genes (DEGs) obtained from a microarray experiment and associated with gene ontology (GO) term angiogenesis were selected for further Taqman quantitative real time-PCR (qRT-PCR) validation studies (Supplementary Table S3A) using a larger cohort of NAFLD liver tissue samples (Supplementary Table S1). For in vitro assays, SYBR Green PCR master mix (Applied Biosystems, Foster City, CA, USA) based qRT-PCR studies were done (Supplementary Table S3B).

2.3. Immunohistochemistry Analysis

Samples of human liver tissues were fixed and stained as per standard protocols. IHC scoring was done on a scale of 1–4 by counting RUNX1 positive cells per field. Details of the protocols and antibodies used are given in the supplementary material and Supplementary Table S4.

2.4. Culture of Endothelial Cells with Conditioned Medium from Hepatoma Cells Treated with Palmitic Acid

Huh7 cells or mouse primary hepatocytes were treated with 200 µM palmitic acid-BSA (PA) for 48 h according to previously published methods [13]. BSA treated cells served as controls. To investigate the effect of steatotic liver cells on gene expression, human umbilical vein endothelial cells (HUVECs) or LSECs (mouse) were incubated with conditioned medium (CM) from BSA/PA treated Huh7 cells or primary hepatocytes, respectively, for 24 h and then assayed for gene expression. For validation of VEGF in the induction of RUNX1 gene expression, studies were also conducted by adding VEGF blocking antibody in HUVECs along with CM from BSA/PA treated Huh7 cells.

2.5. Induction of RUNX1 Expression in HUVECs

To study induction of RUNX1 expression in HUVECs, HUVECs were treated with or without 10 ng/mL VEGF (Himedia Laboratories, Mumbai, India) or TGF-β for 24 h. After 24 h, cells were trypsinized for analysis of RUNX1 gene expression in unstimulated and stimulated cells.

2.6. RUNX1 Inhibition and Overexpression in HUVECs

To elucidate the role of RUNX1 in inflammation and angiogenesis, steatotic or activated HUVECs were transfected with 50 nmol/mL × 106 cells of either negative control (NC) siRNA (Catalogue no# AM4635) or pre-designed RUNX1-specific siRNA (siRNA ID: s229352) (Thermofisher Scientific, Waltham, MA, USA) using lipofectamine 2000 (Invitrogen, Carlsbad, CA, USA) according to the manufacturer’s instructions. Forty-eight hours after transfection, cells were analyzed by qRT-PCR to confirm the knockdown of RUNX1. For overexpression studies, HUVECs were transfected with 2μg/L × 106 cells of control plasmid (pControl, empty vector) or RUNX1 plasmid (pcDNA3.1+ /C-(K)-DYK vector with RUNX1b, Gene Script # OHu26354), referred to as pRUNX1, in the absence or presence of 10 ng/mL VEGF. For transfection, lipofectamine 2000 (Invitrogen, Carlsbad, CA, USA) was used according to the manufacturer’s instructions. pcDNA3-EGFP plasmid vector (kind gift from Dr. Vijay) was used as the control of transfection efficiency and expression in all the transfection experiments. Forty-eight hours after plasmid transfection, cells were analyzed by qRT-PCR. HUVECs with loss of RUNX1 or gain of RUNX1 expression were assayed for gene expression of adhesion molecules, angiogenic markers by qRT-PCR, flow cytometry and angiogenic functions by matrigel assays. CCL2 levels were assayed by ELISA in HUVECs under different conditions.

2.7. Flow Cytometry Analysis

The labeled antibodies used for flow cytometry are given in Supplementary Table S4. After antibody incubation in PBS for 45 min at 4 °C, the cells were fixed with paraformaldehyde in PBS. Multicolor flow cytometry was performed using FACS Verse (BD Biosciences, San Jose, CA, USA) and minimum of 1 million events using live cells were acquired. Analysis of flow cytometry data was performed using Flow-Jo v10 software (BD Biosciences, San Jose, CA, USA). Unstained cells without any antibody were used as negative controls.

2.8. Statistical Analysis

PCR data obtained from patient samples were evaluated for normality distribution by a Shapiro–Wilk test. Statistical differences between the two groups were analyzed by a two-tailed Mann–Whitney U Test or a Student's unpaired t-test (in vitro and flow cytometry experiments) and statistical differences between several groups (data from human samples) by a Kruskal–Wallis Test (SPSS Statistics program, IBM, Leibniz Rechenzentrum, München, Germany). A value of p < 0.05 was regarded as significant. The Pearson correlation (r) was calculated using the IBM SPSS Statistics program. Each experiment was performed in at least triplicates and data were expressed as means ± SD (standard deviation).
More details and description of additional methods are summarized in Supplementary Files.

3. Results

3.1. Expression of Transcription Factor RUNX1 is Increased in NAFLD Controlling Differentially Expressed Genes (Degs) Associated with Angiogenesis

In a preliminary microarray study, we compared mRNA expression in either groups of control (N or normal liver), steatosis (S) and NASH (SH) and identified differentially expressed genes (DEGs) followed by a gene enrichment analysis to identify GO-categories. A subset of 17 DEGs associated with GO-terms angiogenesis and in part with hypoxia and lipid metabolism was selected (Supplementary Table S5), and together with known angiogenic genes (VEGFA, FLT1/VEGFR1, KDR/VEGFR2, CXCR4, PPARγ) [3] further analyzed in a validation study using qRT-PCR. By comparison of the relative mRNA expression of the three groups, N, S and SH, we could confirm a significant differential expression of several genes, but not all in a larger cohort of liver tissue samples (Table 1 and Supplementary Table S6). Among the confirmed DEGs, we found transcription factor RUNX1, quite recently described to regulate stellate cell activation in NASH [14], and known targets of RUNX1 comprised of CCL2, NOS3 (eNOS), PI3KCA and PRKCE. Intriguingly, among the genes, which were not significantly different among the controls and patient groups, were typical angiogenic genes VEGFA, VEGFR1 and VEGFR2 (Supplementary Table S6).

3.2. RUNX1 Expression Correlates with the Severity of NAFLD

The transcription of RUNX1 gene is regulated by differential splicing and promoter utilization, which results in three major isoforms: RUNX1a, RUNX1b and RUNX1c [15]. In all the NAFLD samples analyzed in this study, we found RUNX1b as the predominant isoform (data not shown) and therefore, total RUNX1 expression levels correspond to RUNX1b. To analyze the relevance of RUNX1 mRNA expression with regard to disease progress in our patients, its correlation analysis was performed with the histopathological NASH activity score (NAS), the grade of steatosis, as well as inflammation, and the fibrosis score. RUNX1 mRNA expression demonstrated a significant positive correlation with NAS, steatosis and inflammation degree (Figure 1A–D). In addition to RUNX1, other validated DEGs (Table 1) showing significant correlations with histopathological disease progress are shown in Supplementary Figure S1A–D. RUNX1 target genes, CCL2 and PIK3CA significantly correlated to NAS, steatosis, inflammation grade and fibrosis score, NOS3 to NAS and inflammation grade and PRKCE to NAS and steatosis grade.
To study RUNX1 protein expression, we performed an IHC analysis of RUNX1 in NASH liver biopsies. NASH patients showed varying degrees of RUNX1 protein expression in the liver (Figure 2A). RUNX1 nuclear positivity was almost absent in parenchymal cells and well evident in liver NPCs, presumably among others in ECs and hepatic stellate cells. Negative antibody controls (with RUNX1 antibody and without secondary antibody) are shown in Supplementary Figure S2. Furthermore, RUNX1 expression was significantly positively correlated with fibrosis score (r = 0.80, p < 0.001), NAS (r = 0.77, p < 0.001) and inflammatory grade (r = 0.79, p < 0.01) in NASH liver tissues (Figure 2B–D) and therefore correlates with NASH disease severity. In addition, RUNX1 protein expression (IHC scores) in the liver tissues of NASH patients were significantly positively correlated with its liver mRNA expression (r = 0.81, p < 0.001, Figure 2E).

3.3. Palmitic Acid Treated Huh7 Cells Release VEGF and TGF-β-Inducing RUNX1 Gene Expression in ECs

To investigate if steatosis induces RUNX1 expression, studies were further carried out in in vitro models of NAFLD. PA treatment of Huh7 cells led to significant increases of lipid droplets in these cells visualized by BODIPY staining (Supplementary Figure S3A). Analysis of mRNA expression of BSA treated control cells (BSA-Huh7) and Huh7 cells treated with PA (PA-Huh7) revealed a low but significant increase in the expression of CCL2, CXCL8, PPARγ and PRKCE (Figure 3A), of which the latter was also significantly enhanced in steatotic compared to normal human liver samples (Table 1). Of note, RUNX1 expression was not altered by PA treatment in Huh7 cells. Therefore, in addition to the expression of some angiogenic genes in steatotic hepatocytes, other hepatic cells may contribute to a greater extent to angiogenic gene expression in NASH tissue.
Moreover, HUVECs maintained for 24 h in culture medium (CM) from Huh7 cells treated with PA or BSA demonstrated a substantial upregulation of RUNX1 and its target gene CCL2, as well as the angiogenic gene expression of CXCR4, VCAM1, VEGFR1 and PRKCE after treatment with CM from PA-Huh7 cells (Figure 3B). To verify the impact of CM from PA-Huh7 cells on RUNX1 expression, HUVECs were solely incubated with 200 µM PA, showing a moderate increase of RUNX1 mRNA expression compared to the control cells, but considerably less than in PA-Huh7 CM treated HUVECs (Supplementary Figure S3B). However, only the PA treatment of HUVECs resulted in enhanced cell death and hence, this setup was not used in further assays (data not shown). Furthermore, we confirmed our results in mouse LSECs incubated with CM from primary mouse hepatocytes treated with PA for 24 h, showing a more than two-fold increase in the expression of RUNX1 mRNA compared to control cells (Supplementary Figure S3C).
Then, we analyzed the CMs of PA treated hepatoma cells for angiogenic factors, potentially regulating RUNX1 expression, such as VEGF, PDGF-BB and TGF-β, well known for their proangiogenic and fibrogenic role [16]. Out of the three factors analyzed, both VEGF and TGF-β were significantly enhanced in the PA-treated CM of hepatoma cells in comparison to BSA-treated conditioned media after 24 h of incubation (Figure 3D). However, levels of PDGF-BB were barely detected (Figure 3C). Next, we studied the effect of both VEGF and TGF-β on the gene expression of RUNX1 in HUVECs. At similar concentrations (10 ng/mL), both VEGF and TGF-β substantially upregulated the gene expression of RUNX1 in the HUVECs as compared to the respective non-induced control cells (Figure 3D). Treatment with VEGF antibody reduced the expression of RUNX1 mRNA by about 60% in HUVECs incubated with CM from PA-Huh7 cells in comparison to that seen in untreated cells under the same conditions (Supplementary Figure S3D). VEGF was used as one of the positive controls and a stimulator of RUNX1 expression in further studies. In conclusion, RUNX1 expression is not induced in hepatoma cells by PA treatment, but in ECs, mainly through VEGF and TGF-β, released from hepatoma cells after PA treatment.

3.4. RUNX1 Enhances Expression of Angiogenic Markers and Adhesion Molecules in HUVECs

To study the effects of RUNX1 expression on endothelial cell phenotype, we performed both RUNX1 knock-down and overexpression studies in HUVECs. For the RUNX1 knock-down, we attenuated RUNX1 gene expression in HUVECs treated with CM from PA-Huh7 through RUNX1 siRNA, which led to a more than 50% reduction in RUNX1 mRNA expression in HUVECs compared with NC siRNA (Figure 4A, Supplementary Figure S4A) (RUNX1 siRNA1 is further described as RUNX1 siRNA). In comparison to controls, RUNX1 knockdown conditions led to a significant decrease in the expression of VEGFR1 and RUNX1 target genes, including PRKCE and PI3KCA in HUVECs cultured with CM from PA-Huh7 (Figure 4A). Hypothesizing the role of RUNX1 in endothelial cell mediated inflammation and leukocyte infiltration, we also evaluated the expression of adhesion molecules and chemotactic factor CCL2 (target gene of RUNX1) in HUVECs. When HUVECs were treated with RUNX1 siRNA, expression of VCAM1, PECAM1 and CCL2 was significantly downregulated as compared to that observed in the controls (Figure 4A). On the other hand, transfection with expression vector for RUNX1 (pRUNX1) led to a more than four-fold increase in the expression of RUNX1 gene in the HUVECs compared to control vector transfected cells (Supplementary Figure S4B). Furthermore, in HUVECs transfected with pRUNX1, mRNA expression of PECAM1, VCAM1 and CCL2 was markedly higher as compared to that in the controls (Figure 4B) and this was not enhanced by additional VEGF treatment, except for ICAM1 expression. Although we did not study the underlying mechanisms that lead to increased expression of these molecules by VEGF and RUNX1, an additive effect observed after treatment with both VEGF + pRUNX1 suggests that VEGF may be acting through both RUNX1-dependent and -independent mechanisms in inducing the expression of these molecules in endothelial cells. In addition, these results were confirmed by protein expression analysis using flow cytometry for PECAM1 and VCAM1 (Figure 4C, Supplementary Figure S5) as well as ELISA assay for CCL2 (Figure 4D). Thus, RUNX1 can regulate the expression of adhesion molecules and chemotactic factors, such as CCL2, in ECs.

3.5. RUNX1 Increases Angiogenic Activity of HUVECs

Next, we analyzed if the angiogenic ability of HUVECs was also governed by RUNX1. HUVECs treated with VEGF and/or transfected with pRUNX1 had a substantially augmented angiogenic ability compared to HUVECs transfected with control plasmid, in terms of increased branch points and tube length (Figure 5A–C). The matrigel tube formation ability of HUVECs was also enhanced when cultured in CM from PA-Huh7 cells as compared to that when treated with CM from BSA-Huh7 cells (Supplementary Figure S6A). Both the number of branch points and tube length were increased in the HUVECs after treatment with CM from PA-Huh7 cells and this enhancement was significantly abrogated by additional treatment with RUNX1 siRNA (Supplementary Figure S6A–C). Our data demonstrate that RUNX1, induced by VEGF released from PA treated hepatoma cells, is one of the key responsible factors enhancing angiogenic activity in ECs.

4. Discussion

In the current study, we report increased expression of RUNX1 in liver NPCs, presumably among others in ECs of NASH livers. We describe a novel angiogenic and inflammatory role of RUNX1 in NASH pathogenesis. Signals such as VEGF from PA-treated hepatocytes induce/increase the expression of RUNX1 in ECs, resulting in an enhanced expression of angiogenic and adhesion molecules in these cells, potentially augmenting increased leucocyte migration and adhesion.
Oxidative stress and inflammation-driven pathological angiogenesis is an important mechanism in the progression of NAFLD from steatosis to NASH to cirrhosis and subsequently HCC [17]. Studies have documented both increased and decreased hepatic expression of the angiogenic genes, such as VEGFA and their cognate receptors in patients with NAFLD when compared to control tissues [5,18]. In our study subjects, we did not observe a significant difference in the gene expression of known angiogenic factors such as VEGFA, VEGFR1 and VEGFR2. However, we found a group of angiogenesis associated genes to be differentially expressed in NASH. Among the transcription factors known to control these DEGs, we became particularly interested in RUNX1, which was significantly positively correlated with the histopathological features of NASH. PPARγ was another transcription factor, which was a part of our validated DEGs and showed a good correlation with NAS, steatosis and inflammation degree of the patients and the role of PPARγ in NAFLD is also well established [19].
RUNX1 is a salient factor that is known to control diversification between hematopoietic and endothelial cell lineages [20,21]. Gain and loss of function in RUNX1 has been correlated with cancer progression and metastasis, most notably in acute myeloid leukemia [22]. The role of RUNX1 in enhancing TLR4-mediated inflammation has been demonstrated previously [23]. In our study, there was an increased expression of RUNX1 in liver endothelial cells of NASH patients that significantly correlated with severity of disease, hypothesizing a pathogenic role of endothelial-specific expression of RUNX1 in NASH. Our findings are in concordance with those of Lam et al. who have also identified RUNX1 as a gene upregulated in CD31-positive vascular ECs obtained from human proliferative diabetic retinopathy fibrovascular membranes [24]. Although RUNX1 was not present in parenchymal liver cells, hepatocytes and cholangiocytes, we did find faint RUNX1 mRNA expression in Huh7 cells, which is in concordance with the observation of a low RUNX1 nuclear expression in other hepatoma cells such as human Hep3B and mouse AML12 [25]. Furthermore, RUNX1 was shown to regulate TIMP1 (Tissue Inhibitor of Metalloproteinase 1) expression in hepatic stellate cells (HSCs) and to play a role in activating HSCs in a mouse NASH model [14,26]. This may be because in earlier studies, they solely analyzed RUNX1 in the HSCs and in our study, we focused on endothelial-specific expression of RUNX1 and its potential role in NAFLD pathogenesis. However, it is highly possible that an increased RUNX1 expression in HSCs or other NPCs such as Kupffer cells also contributes to NASH pathogenesis via distinct mechanisms.
Performing in vitro cultures, we observed an increased expression of RUNX1 in HUVECs which were treated with CM from PA treated hepatoma cells, indicating that non-saturated fatty acids and/or high fat conditions, which are associated with oxidative stress and generation of reactive oxygen species (ROS), may be inducing RUNX1 expression in HUVECs. Interestingly, a study has reported an increase in mRNA expression of RUNX1 in liver tissue of a NAFLD guinea pig model, suggesting a regulatory role of RUNX1 for organic cation transporter N1 (OCTN1) [27]. OCTN1 specifically transports ergothioneine, a natural radical scavenger and therefore, augments its anti-oxidative and anti-inflammatory properties. Previous studies in model organisms have shown that high glucose levels act as a trigger for RUNX1 expression via ROS–mediated upregulation of hypoxia-inducible factor 1 [24]. Therefore, RUNX1 expression seems to be triggered by cellular oxidative stress, dietary factors and with regard to hepatic steatosis, this is mediated by VEGF and TGF-β, which were shown to be released from hepatoma cells after PA treatment. The activation of RUNX1 by TGF-β and other transcription factors such as SMAD1 has also been well reported in previous studies [28,29].
Overexpression of RUNX1 in ECs resulted in substantial increase in the expression of adhesion molecules VCAM1 and PECAM1 and also that of CCL2, independent of additional treatment with VEGF. Based on this finding, we propose a novel role of RUNX1 in the potential recruitment of inflammatory cells in NASH, because VEGF is known to aggravate endothelial cell chemokine production in vitro and in vivo and functions in the recruitment of monocytes and T cells [16]. Hence, both VEGF and RUNX1 may act together as crucial angiogenic and pro-inflammatory inducers in NASH. We confirmed the angiogenic properties of RUNX1 in ECs and show that RUNX1 may be an important downstream effector of VEGF in mediating endothelial angiogenesis. However, angiogenic factors other than VEGF may also be involved in RUNX1 regulation and need further characterization.
RUNX1 attenuation also led to a decrease in the expression of known RUNX1 target genes, including CCL2, PI3KCA, PRKCE and eNOS. Furthermore, a decrease in angiogenic activity of ECs while RUNX1 mRNA expression is silenced validated its role as an angiogenic modulator. The contribution of RUNX1 towards angiogenesis in steatosis may also be deduced by the fact that many of its target genes, including eNOS and PI3KCA, are known to be involved in various aspects of angiogenesis, including EC proliferation, sprouting and vascular stabilization during hepatic steatosis and inflammation in high fat diet mice [30,31]. PRKCE is already known to play a critical role in mediating fat-induced hepatic insulin resistance through the buildup of diacylglycerol in NAFLD [32,33,34]. CCL2 is mainly secreted by infiltrating inflammatory monocytes and HSCs in an injured liver and is known to provide pro-angiogenic signals during chronic liver injury [35]. In our study, CCL2 significantly correlated with the severity of human NASH and CCL2 release from ECs was significantly altered by RUNX1 expression, adding novel insight into how RUNX1/CCL2 mediates infiltration of inflammatory cells and angiogenesis in NASH. In addition, the expression of VEGFR1 was found to be attenuated in HUVECs after RUNX1 mRNA silencing, implicating that VEGFR1 may be a vital factor downstream of RUNX1-mediated angiogenesis and disease progression in NAFLD [36]. However, whether VEGFR1 is a direct target of RUNX1 remains to be determined.

5. Conclusions

To summarize, this study implicates the role of RUNX1 in aberrant liver angiogenesis and inflammation in NASH, by modulating the expression of adhesion molecules and angiogenic properties of ECs. The study not only identifies RUNX1 as a novel prospective therapeutic target and a biomarker in NASH but also opens opportunities for exploration of the mechanisms of angiogenesis and inflammation in NASH. In vivo RUNX1 depletion studies that would provide insight into the precise contribution of RUNX1 towards inflammation and fibrosis in NASH are highly requisite.

Supplementary Materials

The following are available online at https://www.mdpi.com/2073-4409/8/10/1277/s1, Supplementary methods, Figure S1: Correlation of validated DEGs with histopathological parameters, Figure S2: Representative immunohistochemical images, Figure S3: RUNX1 mRNA expression in endothelial cells maintained in conditioned medium (CM) from palmitic acid (PA) treated hepatoma (Huh7) cells or primary hepatocytes, Figure S4: Expression of RUNX1 in endothelial cells, Figure S5: RUNX1 alters expression of adhesion molecules in endothelial cells, Figure S6: RUNX1 enhances angiogenic activitiy of endothelial cells, Table S1: Age, BMI, steatosis, inflammation, and fibrosis scores of the cohort studied for gene expression analysis, Table S2: Age, BMI, steatosis, inflammation, and fibrosis scores of the cohort studied for Immunohistochemical analysis, Table S3A: List of genes and assay numbers (Thermo Fisher) used for Fluidigm qRT-PCR, Table S3B: List of genes and primers used for qRT-PCR (SYBR Green-Based), Table S4: Antibodies used for Immunohistochemistry (IHC) and Flow Cytometry (FC) analysis, Table S5: DEGs obtained from mRNA micro-array analysis and associated with GO term angiogenesis are presented with their log2 fold change (FC) and p-values for comparison steatosis (S; n = 7) to normal liver (N; n = 7), NASH (SH; n = 7) to normal liver and NASH to steatosis, Table S6: Analysis of mRNA expression of genes associated with angiogenesis in tissue samples of patients with liver steatosis (S), NASH (SH) and normal liver (N) by qRT-PCR. Shown are genes, which are not significantly differentially expressed between the groups.

Author Contributions

S.K., T.S.W. and S.K.S. designed the study, M.T. performed qRT-PCR analysis of human liver samples, S.V., R.G. and R.D. analyzed mircoarray and qRT-PCR data of human liver samples, performed DEG identification, gene enrichment analysis and GO-term association, S.K., P.R. and S.R. were involved in the cell culture and in vitro studies, M.H. and H.S. performed IHCs, H.S. and S.R. performed RT-PCRs, S.B. was involved in flow cytometry experiments and analysis, C.B. and D.M.T. were involved in IHC analysis, S.S. performed bio-informatic and transcription factor analysis, S.K. and T.S.W. performed data analysis, S.K. wrote the manuscript, T.S.W. advised manuscript preparation, S.K., T.S.W. and S.K.S. did final editing of the manuscript. S.K. and T.S.W. got the funding for the study. All the authors read and approved the manuscript.

Funding

The study was part of the Indo-German Project Collaboration funded by Indian council for Medical Research (ICMR) (Grant No. 50/9/2013/BMS). Furthermore, this work was supported by the German Federal Ministry of Education and Research (BMBF), “Virtual Liver Network”, grant FKZ 0315753 (TSW) and FKZ 0315736 (RG), and “ALIV” grant FKZ 01DQ14013 (TSW).

Conflicts of Interest

The authors declare no conflict of interest.

References

  1. Younossi, Z.; Anstee, Q.M.; Marietti, M.; Hardy, T.; Henry, L.; Eslam, M.; George, J.; Bugianesi, E. Global burden of NAFLD and NASH: Trends, predictions, risk factors and prevention. Nat. Rev. Gastroenterol. Hepatol. 2018, 15, 11–20. [Google Scholar] [CrossRef] [PubMed]
  2. Cohen, J.C.; Horton, J.D.; Hobbs, H.H. Human fatty liver disease: old questions and new insights. Science 2011, 332, 1519–1523. [Google Scholar] [CrossRef] [PubMed]
  3. Fernández, M.; Semela, D.; Bruix, J.; Colle, I.; Pinzani, M.; Bosch, J. Angiogenesis in liver disease. J. Hepatol. 2009, 50, 604–620. [Google Scholar] [CrossRef] [PubMed]
  4. Kaur, S.; Anita, K. Angiogenesis in liver regeneration and fibrosis: “a double-edged sword”. Hepatol. Int. 2013, 7, 959–968. [Google Scholar] [CrossRef]
  5. Coulon, S.; Francque, S.; Colle, I.; Verrijken, A.; Blomme, B.; Heindryckx, F.; De Munter, S.; Prawitt, J.; Caron, S.; Staels, B.; et al. Evaluation of inflammatory and angiogenic factors in patients with non-alcoholic fatty liver disease. Cytokine 2012, 59, 442–449. [Google Scholar] [CrossRef]
  6. Coulon, S.; Legry, V.; Heindryckx, F.; Van Steenkiste, C.; Casteleyn, C.; Olievier, K.; Libbrecht, L.; Carmeliet, P.; Jonckx, B.; Stassen, J.-M.; et al. Role of vascular endothelial growth factor in the pathophysiology of nonalcoholic steatohepatitis in two rodent models. Hepatology 2013, 57, 1793–1805. [Google Scholar] [CrossRef]
  7. Ciupińska-Kajor, M.; Hartleb, M.; Kajor, M.; Kukla, M.; Wyleżoł, M.; Lange, D.; Liszka, L. Hepatic angiogenesis and fibrosis are common features in morbidly obese patients. Hepatol. Int. 2013, 7, 233–240. [Google Scholar] [CrossRef]
  8. North, T.E.; De Bruijn, M.F.T.R.; Stacy, T.; Talebian, L.; Lind, E.; Robin, C.; Binder, M.; Dzierzak, E.; A Speck, N. Runx1 expression marks long-term repopulating hematopoietic stem cells in the midgestation mouse embryo. Immunity 2002, 16, 661–672. [Google Scholar] [CrossRef]
  9. Iwatsuki, K.; Tanaka, K.; Kaneko, T.; Kazama, R.; Okamoto, S.; Nakayama, Y.; Ito, Y.; Satake, M.; Takahashi, S.; et al. Runx1 promotes angiogenesis by downregulation of insulin-like growth factor-binding protein-3. Oncogene 2005, 24, 1129–1137. [Google Scholar] [CrossRef]
  10. Takakura, N.; Watanabe, T.; Suenobu, S.; Yamada, Y.; Noda, T.; Ito, Y.; Satake, M.; Suda, T. A Role for Hematopoietic Stem Cells in Promoting Angiogenesis. Cell 2000, 102, 199–209. [Google Scholar] [CrossRef] [Green Version]
  11. Weiss, T.S.; Lupke, M.; Ibrahim, S.; Buechler, C.; Lorenz, J.; Ruemmele, P.; Hofmann, U.; Melter, M.; Dayoub, R. Attenuated lipotoxicity and apoptosis is linked to exogenous and endogenous augmenter of liver regeneration by different pathways. PLOS ONE 2017, 12, e0184282. [Google Scholar] [CrossRef] [PubMed]
  12. Kleiner, D.E.; Brunt, E.M.; Natta, V.M.; Behling, C.; Contos, M.J.; Cummings, O.W.; Ferrell, L.D.; Liu, Y.C.; Torbenson, M.S.; Unalp-Arida, A.; et al. Nonalcoholic Steatohepatitis Clinical Research Network. Design and validation of a histological scoring system for nonalcoholic fatty liver disease. Hepatology 2005, 41, 1313–1321. [Google Scholar] [CrossRef] [PubMed]
  13. Rana, P.; Yi, L.; Will, Y. Palmitate Increases the Susceptibility of Cells to Drug-Induced Toxicity: An In Vitro Method to Identify Drugs With Potential Contraindications in Patients With Metabolic Disease. Toxicol. Sci. 2012, 129, 346–362. [Google Scholar] [Green Version]
  14. Marcher, A.-B.; Bendixen, S.M.; Terkelsen, M.K.; Hohmann, S.S.; Hansen, M.H.; Larsen, B.D.; Mandrup, S.; Dimke, H.; Detlefsen, S.; Ravnskjaer, K. Transcriptional regulation of Hepatic Stellate Cell activation in NASH. Sci. Rep. 2019, 9, 2324. [Google Scholar] [CrossRef]
  15. Miyoshi, H.; Ohira, M.; Shimizu, K.; Mitani, K.; Hirai, H.; Imai, T.; Yokoyama, K.; Soceda, E.; Ohkl, M. Alternative splicing and genomic structure of theAML1gene involved in acute myeloid leukemia. Nucleic Acids Res. 1995, 23, 2762–2769. [Google Scholar] [CrossRef]
  16. Bocca, C.; Novo, E.; Miglietta, A.; Parola, M. Angiogenesis and Fibrogenesis in Chronic Liver Diseases. Cell Mol. Gastroenterol. Hepatol. 2015, 1, 477–488. [Google Scholar] [CrossRef] [Green Version]
  17. Kitade, M.; Yoshiji, H.; Kojima, H.; Ikenaka, Y.; Noguchi, R.; Kaji, K.; Yoshii, J.; Yanase, K.; Namisaki, T.; Yamazaki, M.; et al. Neovascularization and oxidative stress in the progression of non-alcoholic steatohepatitis. Mol. Med. Rep. 2008, 1, 543–548. [Google Scholar] [CrossRef]
  18. Wang, R.; Wang, X.; Zhuang, L. Gene expression profiling reveals key genes and pathways related to the development of non-alcoholic fatty liver disease. Ann. Hepatol. 2016, 15, 190–199. [Google Scholar]
  19. Tailleux, A.; Wouters, K.; Staels, B. Roles of PPARs in NAFLD: Potential therapeutic targets. Biochim. Et Biophys. Acta (BBA) Mol. Cell Boil. Lipids 2012, 1821, 809–818. [Google Scholar] [CrossRef]
  20. Dzierzak, E.; Speck, N.A. Of lineage and legacy: The development of mammalian hematopoietic stem cells. Nat. Immunol. 2008, 9, 129–136. [Google Scholar] [CrossRef]
  21. Lam, K.; Zhang, D.E. RUNX1 and RUNX1-ETO: Roles in hematopoiesis and leukemogenesis. Front. Biosci (Landmark Ed.) 2012, 17, 1120–1139. [Google Scholar] [CrossRef] [PubMed]
  22. Blyth, K.; Cameron, E.R.; Neil, J.C. The runx genes: Gain or loss of function in cancer. Nat. Rev. Cancer 2005, 5, 376–387. [Google Scholar] [CrossRef] [PubMed]
  23. Luo, M.-C.; Zhou, S.-Y.; Feng, D.-Y.; Xiao, J.; Li, W.-Y.; Xu, C.-D.; Wang, H.-Y.; Zhou, T. Runt-related Transcription Factor 1 (RUNX1) Binds to p50 in Macrophages and Enhances TLR4-triggered Inflammation and Septic Shock. J. Boil. Chem. 2016, 291, 22011–22020. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  24. Lam, J.D.; Oh, D.J.; Wong, L.L.; Amarnani, D.; Park-Windhol, C.; Sanchez, A.V.; Cardona-Velez, J.; McGuone, D.; Stemmer-Rachamimov, A.O.; Eliott, D.; et al. Identification of RUNX1 as a Mediator of Aberrant Retinal Angiogenesis. Diabetes 2017, 66, 1950–1956. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  25. Wildey, G.M.; Howe, P.H. Runx1 is a co-activator with FOXO3 to mediate transforming growth factor beta (TGF β)-induced Bim transcription in hepatic cells. J. Biol. Chem. 2009, 284, 20227–20239. [Google Scholar] [CrossRef] [PubMed]
  26. Bertrand-Philippe, M.; Ruddell, R.G.; Arthur, M.J.P.; Thomas, J.; Mungalsingh, N.; Mann, D.A. Regulation of Tissue Inhibitor of Metalloproteinase 1 Gene Transcription by RUNX1 and RUNX2. J. Boil. Chem. 2004, 279, 24530–24539. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  27. Cheah, I.K.; Tang, R.; Ye, P.; Yew, T.S.; Lim, K.H.; Halliwell, B. Liver ergothioneine accumulation in a guinea pig model of non-alcoholic fatty liver disease. A possible mechanism of defence? Free Radic. Res. 2016, 50, 14–25. [Google Scholar] [CrossRef]
  28. Pimanda, J.E.; Donaldson, I.J.; de Bruijn, M.F.; Kinston, S.; Knezevic, K.; Huckle, L.; Piltz, S.; Landry, J.R.; Green, A.R.; Tannahill, D.; et al. The SCL transcriptional network and BMP signaling pathway interact to regulate RUNX1 activity. Proc. Natl. Acad. Sci. USA 2007, 104, 840–845. [Google Scholar] [CrossRef] [Green Version]
  29. Zhou, T.; Luo, M.; Cai, W.; Zhou, S.; Feng, D.; Xu, C.; Wang, H. Runt-Related Transcription Factor 1 (RUNX1) Promotes TGF-β-Induced Renal Tubular Epithelial-to-Mesenchymal Transition (EMT) and Renal Fibrosis through the PI3K Subunit p110δ. EBioMedicine 2018, 31, 217–225. [Google Scholar] [CrossRef]
  30. Karar, J.; Maity, A. PI3K/AKT/mTOR Pathway in Angiogenesis. Front. Mol. Neurosci. 2011, 4, 51. [Google Scholar] [CrossRef] [Green Version]
  31. Zhang, W.; Liu, Y.; Wu, M.; Zhu, X.; Wang, T.; He, K.; Li, P.; Wu, X. PI3K inhibition protects mice from NAFLD by down-regulating CMKLR1 and NLRP3 in Kupffer cells. J. Physiol. Biochem. 2017, 73, 583–594. [Google Scholar] [CrossRef] [PubMed]
  32. Jornayvaz, F.R.; Shulman, G.I. Diacylglycerol activation of protein kinase Cε and hepatic insulin resistance. Cell Metab. 2012, 15, 574–584. [Google Scholar] [CrossRef] [PubMed]
  33. Kumashiro, N.; Erion, D.M.; Zhang, D.; Kahn, M.; Beddow, S.A.; Chu, X.; Still, C.D.; Gerhard, G.S.; Han, X.; Dziura, J.; et al. Cellular mechanism of insulin resistance in nonalcoholic fatty liver disease. Proc. Natl. Acad. Sci. USA 2011, 108, 16381–16385. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  34. Ter Horst, K.W.; Gilijamse, P.W.; Versteeg, R.I.; Ackermans, M.T.; Nederveen, A.J.; La Fleur, S.E.; Romijn, J.A.; Nieuwdorp, M.; Zhang, D.; Samuel, V.T.; et al. Hepatic Diacylglycerol-Associated Protein Kinase Cε Translocation Links Hepatic Steatosis to Hepatic Insulin Resistance in Humans. Cell Rep. 2017, 19, 1997–2004. [Google Scholar] [CrossRef] [PubMed]
  35. Ehling, J.; Bartneck, M.; Wei, X.; Gremse, F.; Fech, V.; Möckel, D.; Baeck, C.; Hittatiya, K.; Eulberg, D.; Luedde, T.; et al. CCL2-dependent infiltrating macrophages promote angiogenesis in progressive liver fibrosis. Gut 2014, 63, 1960–1971. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  36. Takahashi, M. ERK/MAPK-dependent PI3K/Akt phosphorylation through VEGFR-1 after VEGF stimulation in activated hepatic stellate cells. Hepatol. Res. 2003, 26, 232–236. [Google Scholar] [CrossRef]
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Figure 1. Correlation between RUNX1 mRNA expression and histopathological parameters. Expression of RUNX1 mRNA was analyzed by qRT-PCR in liver tissue samples from patients with NASH (n = 43), hepatic steatosis (n = 46) and normal liver tissue (n = 33) and correlated to histopathologic proven (A) NASH activity score (B) steatosis grade (C) inflammation grade and (D) fibrosis grade. HPRT mRNA expression was determined for normalization, statistical differences between several grades were analyzed by Kruskal-Wallis Test (p < 0.05 was considered significant) and ‘r’ denotes the Pearson’s correlation coefficient.
Figure 1. Correlation between RUNX1 mRNA expression and histopathological parameters. Expression of RUNX1 mRNA was analyzed by qRT-PCR in liver tissue samples from patients with NASH (n = 43), hepatic steatosis (n = 46) and normal liver tissue (n = 33) and correlated to histopathologic proven (A) NASH activity score (B) steatosis grade (C) inflammation grade and (D) fibrosis grade. HPRT mRNA expression was determined for normalization, statistical differences between several grades were analyzed by Kruskal-Wallis Test (p < 0.05 was considered significant) and ‘r’ denotes the Pearson’s correlation coefficient.
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Figure 2. Immunohistochemical (IHC) analysis of RUNX1 expression in NASH patients. (A) RUNX1 immunostained images (20× objective) with an increasing number of brown nuclear immuno-positive cells (score 1–4). RUNX1 positivity was mostly observed in the non-parenchymal cells. Hematoxylin stained nuclei were distinguishable from RUNX1-positive brown nuclei. (B) Correlation between RUNX1 IHC and NASH activity score (n = 16), (C) RUNX1 IHC score and fibrosis grade (n = 16), and (D) RUNX1 IHC score and inflammatory grade (n = 16) in NASH patients. (E) Correlation between RUNX1 mRNA and its IHC score in liver tissues of patients (n = 16). The Pearson correlation (r) and statistical significance (p) were calculated.
Figure 2. Immunohistochemical (IHC) analysis of RUNX1 expression in NASH patients. (A) RUNX1 immunostained images (20× objective) with an increasing number of brown nuclear immuno-positive cells (score 1–4). RUNX1 positivity was mostly observed in the non-parenchymal cells. Hematoxylin stained nuclei were distinguishable from RUNX1-positive brown nuclei. (B) Correlation between RUNX1 IHC and NASH activity score (n = 16), (C) RUNX1 IHC score and fibrosis grade (n = 16), and (D) RUNX1 IHC score and inflammatory grade (n = 16) in NASH patients. (E) Correlation between RUNX1 mRNA and its IHC score in liver tissues of patients (n = 16). The Pearson correlation (r) and statistical significance (p) were calculated.
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Figure 3. RUNX1 and angiogenic gene expression in endothelial cells maintained in conditioned medium (CM) from palmitic acid (PA) treated hepatoma (Huh7) cells. (A) Huh7 cells treated with 0.2 mM PA for 48 h were analyzed for mRNA expression of RUNX1 and genes identified as angiogenesis associated DEGs in human NASH samples. The dotted line represents the control showing gene expression in Huh7 cells treated with BSA (n = 4). (B) HUVECs incubated with CM from PA-Huh7 cells were analyzed for mRNA expression of RUNX1, its target and angiogenic genes. The dotted line represents control, showing gene expression in HUVECs treated with CM from BSA-Huh7 cells (n = 4). 18S RNA expression was used for normalization. (C) Huh7 cells were treated with BSA or PA or CM alone and analyzed for the release of VEGF, PDGF-BB and TGF-β (pg/mL) (n = 3). (D) Relative RUNX1 mRNA expression in HUVECs treated with VEGF and TGF-β (10 ng/mL each) for 24 h. Un-induced cells without any manipulation were used as respective controls (Dotted line) (n = 3). 18S RNA expression was used for normalization. Data represent mean ± SD. * p < 0.05; ** p < 0.001.
Figure 3. RUNX1 and angiogenic gene expression in endothelial cells maintained in conditioned medium (CM) from palmitic acid (PA) treated hepatoma (Huh7) cells. (A) Huh7 cells treated with 0.2 mM PA for 48 h were analyzed for mRNA expression of RUNX1 and genes identified as angiogenesis associated DEGs in human NASH samples. The dotted line represents the control showing gene expression in Huh7 cells treated with BSA (n = 4). (B) HUVECs incubated with CM from PA-Huh7 cells were analyzed for mRNA expression of RUNX1, its target and angiogenic genes. The dotted line represents control, showing gene expression in HUVECs treated with CM from BSA-Huh7 cells (n = 4). 18S RNA expression was used for normalization. (C) Huh7 cells were treated with BSA or PA or CM alone and analyzed for the release of VEGF, PDGF-BB and TGF-β (pg/mL) (n = 3). (D) Relative RUNX1 mRNA expression in HUVECs treated with VEGF and TGF-β (10 ng/mL each) for 24 h. Un-induced cells without any manipulation were used as respective controls (Dotted line) (n = 3). 18S RNA expression was used for normalization. Data represent mean ± SD. * p < 0.05; ** p < 0.001.
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Figure 4. RUNX1 alters expression of angiogenic and adhesion molecules in endothelial cells (A) HUVECs, treated with RUNX1 siRNA or NC siRNA and incubated with CM from PA-Huh7 cells, were analyzed for mRNA expression (fold change) of angiogenic, adhesion molecule and RUNX1 target genes (n = 3). (B) HUVECs transfected with RUNX1 expression plasmid (pRUNX1), control plasmid (pControl, i.e., empty vector) and/or incubated with VEGF (10 ng/mL) were analyzed for mRNA expression of adhesion molecule and chemotactic genes. HUVECs without any treatment were used as respective controls (Dotted line) (n = 3). 18S RNA expression was used for normalization. (C) Quantitative analysis of flow cytometry from (C) is shown (n = 3). (D) CCL2 levels (pg/mL) in culture media of HUVECs transfected with RUNX1 expression plasmid (pRUNX1), control plasmid (pControl, empty vector) and/or incubated with VEGF (10 ng/mL) (n = 4). Data represent mean ± SD. * p < 0.05 and ** p < 0.001.
Figure 4. RUNX1 alters expression of angiogenic and adhesion molecules in endothelial cells (A) HUVECs, treated with RUNX1 siRNA or NC siRNA and incubated with CM from PA-Huh7 cells, were analyzed for mRNA expression (fold change) of angiogenic, adhesion molecule and RUNX1 target genes (n = 3). (B) HUVECs transfected with RUNX1 expression plasmid (pRUNX1), control plasmid (pControl, i.e., empty vector) and/or incubated with VEGF (10 ng/mL) were analyzed for mRNA expression of adhesion molecule and chemotactic genes. HUVECs without any treatment were used as respective controls (Dotted line) (n = 3). 18S RNA expression was used for normalization. (C) Quantitative analysis of flow cytometry from (C) is shown (n = 3). (D) CCL2 levels (pg/mL) in culture media of HUVECs transfected with RUNX1 expression plasmid (pRUNX1), control plasmid (pControl, empty vector) and/or incubated with VEGF (10 ng/mL) (n = 4). Data represent mean ± SD. * p < 0.05 and ** p < 0.001.
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Figure 5. RUNX1 enhances the angiogenic activitiy of endothelial cells. (A) Representative tube formation images of HUVECs on matrigel (4× objective) transfected with RUNX1 expression plasmid (pRUNX1), control plasmid (pControl, empty vector) and/or incubated with VEGF (10 ng/mL). (B) Average number of branch points per field and (C) tube length per field formed by HUVECs on matrigel under conditions described in (A) (n = 3). Data represent mean ± SD. * p < 0.05.
Figure 5. RUNX1 enhances the angiogenic activitiy of endothelial cells. (A) Representative tube formation images of HUVECs on matrigel (4× objective) transfected with RUNX1 expression plasmid (pRUNX1), control plasmid (pControl, empty vector) and/or incubated with VEGF (10 ng/mL). (B) Average number of branch points per field and (C) tube length per field formed by HUVECs on matrigel under conditions described in (A) (n = 3). Data represent mean ± SD. * p < 0.05.
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Table
Table 1. Analysis of mRNA expression of genes associated with angiogenesis in resected hepatic tissue samples of patients with normal liver (N), steatosis (S) and non-alcoholic steatohepatitis (NASH). Data are shown as means ± SD and statistical differences were analyzed by pairwise comparison using a Kruskal–Wallis Test.
Table 1. Analysis of mRNA expression of genes associated with angiogenesis in resected hepatic tissue samples of patients with normal liver (N), steatosis (S) and non-alcoholic steatohepatitis (NASH). Data are shown as means ± SD and statistical differences were analyzed by pairwise comparison using a Kruskal–Wallis Test.
Relative mRNA Expressionp-Value
GeneN (n = 33)S (n = 46)NASH (n = 43)N/SN/SHS/SH
CCL21.82 ± 1.472.30 ± 1.633.74 ± 2.130.5340.0000.002
CXCL8 (IL8)4.33 ± 4.57.16 ± 8.9916.97 ± 17.180.4040.0000.002
CXCR41.57 ± 1.182.63 ± 1.702.87 ± 1.840.0080.0021.000
EREG2.87 ± 2.265.34 ± 4.867.48 ± 6.190.1970.0010.285
FASN3.27 ± 2.076.35 ± 5.755.67 ± 5.270.0480.0771.000
HOMX1 (HO1)0.71 ± 0.360.67 ± 0.390.95 ± 0.661.0000.1260.024
NOS3 (eNOS)0.72 ± 0.320.82 ± 0.521.12 ± 0.741.0000.0110.040
PIK3CA0.61 ± 0.210.98 ± 1.220.81 ± 0.250.0130.0011.000
PPARγ0.61 ± 0.240.73 ± 0.340.97 ± 0.470.5520.0010.034
PRKCE0.71 ± 0.340.96 ± 0.421.00 ± 0.600.0040.0141.000
PROK22.55 ± 2.173.66 ± 4.136.49 ± 7.961.0000.0580.182
RUNX11.75 ± 1.211.90 ± 1.563.38 ± 2.551.0000.0000.002

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Kaur, S.; Rawal, P.; Siddiqui, H.; Rohilla, S.; Sharma, S.; Tripathi, D.M.; Baweja, S.; Hassan, M.; Vlaic, S.; Guthke, R.; et al. Increased Expression of RUNX1 in Liver Correlates with NASH Activity Score in Patients with Non-Alcoholic Steatohepatitis (NASH). Cells 2019, 8, 1277. https://doi.org/10.3390/cells8101277

AMA Style

Kaur S, Rawal P, Siddiqui H, Rohilla S, Sharma S, Tripathi DM, Baweja S, Hassan M, Vlaic S, Guthke R, et al. Increased Expression of RUNX1 in Liver Correlates with NASH Activity Score in Patients with Non-Alcoholic Steatohepatitis (NASH). Cells. 2019; 8(10):1277. https://doi.org/10.3390/cells8101277

Chicago/Turabian Style

Kaur, Savneet, Preety Rawal, Hamda Siddiqui, Sumati Rohilla, Shvetank Sharma, Dinesh M Tripathi, Sukriti Baweja, Mohsin Hassan, Sebastian Vlaic, Reinhard Guthke, and et al. 2019. "Increased Expression of RUNX1 in Liver Correlates with NASH Activity Score in Patients with Non-Alcoholic Steatohepatitis (NASH)" Cells 8, no. 10: 1277. https://doi.org/10.3390/cells8101277

APA Style

Kaur, S., Rawal, P., Siddiqui, H., Rohilla, S., Sharma, S., Tripathi, D. M., Baweja, S., Hassan, M., Vlaic, S., Guthke, R., Thomas, M., Dayoub, R., Bihari, C., Sarin, S. K., & Weiss, T. S. (2019). Increased Expression of RUNX1 in Liver Correlates with NASH Activity Score in Patients with Non-Alcoholic Steatohepatitis (NASH). Cells, 8(10), 1277. https://doi.org/10.3390/cells8101277

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