Characterization of regulatory transcriptional mechanisms in hepatocyte lipotoxicity

Pérez-Schindler, Joaquín; Vargas-Fernández, Elyzabeth; Karrer-Cardel, Bettina; Ritz, Danilo; Schmidt, Alexander; Handschin, Christoph

doi:10.1038/s41598-022-15731-4

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Published: 07 July 2022

Characterization of regulatory transcriptional mechanisms in hepatocyte lipotoxicity

Joaquín Pérez-Schindler¹^nAff2,
Elyzabeth Vargas-Fernández¹,
Bettina Karrer-Cardel¹,
Danilo Ritz¹,
Alexander Schmidt¹ &
…
Christoph Handschin¹

Scientific Reports volume 12, Article number: 11477 (2022) Cite this article

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Abstract

Non-alcoholic fatty liver disease is a continuum of disorders among which non-alcoholic steatohepatitis (NASH) is particularly associated with a negative prognosis. Hepatocyte lipotoxicity is one of the main pathogenic factors of liver fibrosis and NASH. However, the molecular mechanisms regulating this process are poorly understood. The main aim of this study was to dissect transcriptional mechanisms regulated by lipotoxicity in hepatocytes. We achieved this aim by combining transcriptomic, proteomic and chromatin accessibility analyses from human liver and mouse hepatocytes. This integrative approach revealed several transcription factor networks deregulated by NASH and lipotoxicity. To validate these predictions, genetic deletion of the transcription factors MAFK and TCF4 was performed, resulting in hepatocytes that were better protected against saturated fatty acid oversupply. MAFK- and TCF4-regulated gene expression profiles suggest a mitigating effect against cell stress, while promoting cell survival and growth. Moreover, in the context of lipotoxicity, some MAFK and TCF4 target genes were to the corresponding differentially regulated transcripts in human liver fibrosis. Collectively, our findings comprehensively profile the transcriptional response to lipotoxicity in hepatocytes, revealing new molecular insights and providing a valuable resource for future endeavours to tackle the molecular mechanisms of NASH.

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Introduction

Non-alcoholic fatty liver disease (NAFLD) is a spectrum of disorders that progresses from NAFL (hepatic steatosis) to non-alcoholic steatohepatitis (NASH), leading to cirrhosis and liver cancer¹. NASH is characterized by chronic liver damage, inflammation and fibrosis, a stage that significantly increases morbidity and mortality¹. Several genetic and environmental factors (e.g. a sedentary lifestyle) drive the development of NAFLD, among which the excessive supply of saturated fatty acids to the liver and, consequently, hepatocyte lipotoxicity is the main risk factor for NASH^1,2. Importantly, hepatocyte lipotoxicity is the leading cause of liver fibrosis that remains as the main predictor of liver-related death^1,2. However, therapies to target this process are scarce, as evidenced by the lack of approved medications for the treatment of NASH³.

Although the molecular underpinnings controlling hepatocyte lipotoxicity are elusive, key biological processes such as oxidative stress, endoplasmic reticulum (ER) stress and inflammation are known to play a central role^1,2. Interestingly, obesogenic diets extensively remodel the transcriptome, epigenome and chromatin accessibility landscape of mouse liver^4,5,6,7. These studies suggest that disruption of transcriptional networks and chromatin function are fundamental to pathogenic progression. Such transcriptional networks are regulated by transcription factors that, upon activation, are recruited to DNA regulatory elements located in regions of accessible chromatin⁸. Despite the great therapeutic potential, the transcriptional mechanisms regulating hepatocyte lipotoxicity remain virtually unknown. Therefore, the main aim of this study was to characterize gene regulatory networks deregulated by saturated fatty acids oversupply in hepatocytes. We achieved this aim by implementing a multi-omics approach in which human and mouse datasets were integrated to uncover conserved transcriptional responses.

Results

NASH and lipotoxicity share a common molecular signature

To discover conserved hepatocyte-specific mechanisms linked to lipotoxicity and, potentially, NASH development, we implemented a multi-omics strategy in which we integrated analyses from human liver biopsies and mouse hepatocytes. Liver tissue was obtained from healthy control (CON) subjects and NASH patients suffering from obesity and diabetes (Fig. 1A). In addition, lipotoxicity was investigated in FL83B mouse hepatocytes that were stimulated with bovine serum albumin (BSA) or BSA conjugated with the saturated fatty acid palmitate (PAL) for 24 h. As expected, PAL induced a dose-dependent increase in hepatocyte cytotoxicity (Fig. 1B). We found that while a low dose of PAL increases the accumulation of intracellular lipids, incubating cells with a higher dose had no significant effect (Fig. 1C). Consistently, a lower capacity to incorporate saturated fatty acids into triglyceride has been demonstrated to mediate the cytotoxic effect of PAL overload⁹. Therefore, all of the following experiments were carried out under high PAL concentration (0.4 mM).

We initially assessed whether human liver from NASH patients and mouse hepatocyte lipotoxicity share a common transcriptional response. Of note, human RNA-seq data exhibited a high level of variability, which resulted in a low number of differentially expressed genes (DEG) when using the adjusted p-value (q-value) as cut-off. We thus used non-adjusted p-value as a less stringent approach, which we subsequently complement with extensive cross-comparison of our data with independent mouse and human datasets (see below). Accordingly, in humans, NASH was associated with the up- and down-regulation of 422 and 615 genes, respectively (Fig. 1D and Table S1). Compared to these chronic changes in human NASH, mouse hepatocytes exhibited a stronger acute transcriptional response as evidenced by a higher number of DEG, comprising 1744 and 1396 up- and down-regulated genes, respectively (Fig. 1E and Table S1). Although there was a small overlap of DEG between human NASH and hepatocyte PAL treatment (Fig. 1F,G; purple lines), we observed a high degree of functional overlap reflected by a large number of genes belonging to the same ontology terms (Fig. 1F,G; blue lines). Consistent with the induction of lipotoxicity and NASH, up-regulated genes were related to oxidative stress, nuclear receptor function and cellular response to stress (Fig. 1H), while down-regulated genes were linked to processes such as the remodelling of the extracellular matrix, cell cycle progression and survival (Fig. 1I). To further validate our findings, we determine whether such functional overlap is conserved when comparing our data with publicly available human liver RNA-seq data (GEO accession: GSE135251) from NASH patients exhibiting cirrhosis (NASH F4; n = 14)¹⁰. Accordingly, this analysis revealed an overlap between disease-relevant ontology terms enriched in NASH F4 subjects and our mouse and human data, further supporting the link between hepatocyte lipotoxicity and NASH (Table S2).

We next assessed the liver and hepatocyte proteome to complement the transcriptome analysis and improve the comparison between NASH and lipotoxicity. Similar to the human RNA-seq results described above, the human proteomics data analysis was based on non-adjusted p-value as cut-off. We found that proteome remodelling was also milder in liver from NASH patients (up-regulated: 92 and down-regulated: 191) compared to the effects of PAL stimulation in mouse hepatocytes (up-regulated: 830 and down-regulated: 552) (Fig. 2A,F; Table S3). Similar to the transcriptome analysis, NASH and PAL proteomes showed a high level of functional overlap (Fig. 2C,D; blue lines). A number of biological processes sensitive to both NASH and lipotoxicity were identified among up-regulated proteins, including oxidative stress and cellular response to stress, thus resembling the effects observed at the RNA level (Fig. 2E). Moreover, our data demonstrate that down-regulated proteins were characterized by dysregulation of shared biological processes involved in protein folding, ER function, RNA processing and apoptosis (Fig. 2F). Such functional overlap at the RNA and protein level suggest that lipotoxicity in mouse hepatocytes and in human NASH livers share a common molecular response.

NASH and lipotoxicity remodel the chromatin accessibility landscape

We next performed chromatin accessibility analysis by assay for transposase-accessible chromatin by sequencing (ATAC-seq) to elucidate transcriptional mechanisms mediating hepatocyte lipotoxicity and NASH. The total number of ATAC-seq peaks (representing regions of accessible chromatin) was similar between liver from CON and NASH (Fig. 3A). In contrast, mouse hepatocytes treated with PAL had a lower number of peaks compared to the BSA control condition (Fig. 3B). Both human and mouse ATAC-seq data showed that the vast majority of peaks were located in introns and DNA regulatory elements such as promoters and enhancers, at distal intergenic regions (Fig. 3A,B). Interestingly, our data revealed that the proportion of genomic regions (e.g. introns and promoters) harbouring accessible chromatin is to a large extent unaltered by NASH or lipotoxicity (Fig. 3A,B). Globally, chromatin accessibility was slightly increased and strongly decreased in liver from NASH patients and in hepatocyte lipotoxicity, respectively (Fig. 3C,D). Notably, in human livers, around 20% of the peaks were exclusively found in CON or NASH samples (Fig. 3E,G). These data demonstrate that although the total number of ATAC-seq peaks is similar between groups, there are specific regions on the chromatin in which accessibility is lost (CON-specific peaks) or gained (NASH-specific peaks) during NASH development. In the context of mouse hepatocyte lipotoxicity, we observed a higher proportion of BSA-specific (35%) than PAL-specific (13%) peaks (Fig. 3F,H), which is consistent with the global decrease in chromatin accessibility induced by PAL.

To determine the link between changes in chromatin accessibility and gene expression, we identified the closest down- and up-regulated genes associated with chromatin regions with decreased and increased accessibility, respectively. This analysis showed that repressed genes linked to CON-specific peaks were related to the regulation of cellular integrity, growth and vascularization, whereas up-regulated genes linked to NASH-specific peaks were mainly related to metabolic pathways (Fig. 3I). Hepatocytes stimulated with PAL also exhibited a subset of down-regulated genes linked to BSA-specific peaks that we found to be primarily associated with the regulation of cell cycle and survival (Fig. 3J). Moreover, genes up-regulated by PAL and linked to PAL-specific peaks were involved in the positive regulation of the unfolded protein response (UPR) and the development of fibrosis (Fig. 3J), thus supporting the role of hepatocyte lipotoxicity in NASH development. Our data therefore further support the strong transcriptional component in both hepatocyte lipotoxicity and NASH.

Lipotoxicity regulates a specific subset of transcription factors

Our findings strongly suggest that transcription factors play a central regulatory role in hepatocyte lipotoxicity, a process that holds great therapeutic potential for the treatment of NASH³. We initially sought to identify such transcription factors via motif enrichment analysis of chromatin areas showing a loss (CON/BSA-specific) or gain (NASH/PAL-specific) in accessibility at distal intergenic regions (e.g. enhancers) and promoters. CON- and NASH-specific peaks had similar numbers of enriched transcription factor motifs at distal intergenic regions, but NASH was characterized by a strong enrichment of CTCF and CTCFL motifs (Fig. 4A and Table S4). In the context of hepatocyte lipotoxicity, we found that PAL treatment substantially decreased the number and enrichment of transcription factor motifs (CON-specific: 239 vs. PAL-specific: 55) at distal intergenic regions (Fig. 4B and Table S4). Analysis of promoters revealed similar results, where CON and NASH exhibited comparable number of enriched transcription factor motifs (Fig. 4C and Table S4), whereas PAL exerted a strong blunting effect (Fig. 4D and Table S4). Of note, the negative effect of PAL on transcription factor motifs enrichment is likely associated with a mild change in chromatin accessibility (e.g. PAL-specific ATAC-seq peaks). We next defined the subset of transcription factor motifs shared between human liver and mouse hepatocytes at distal intergenic regions (CON/BSA: 103 and NASH/PAL: 25) and promoters (CON/BSA: 82 and NASH/PAL: 29). Interestingly, while most NASH/PAL transcription factor motifs were shared with CON/BSA, we found that 76% and 67% of transcription factor motifs were less enriched in distal intergenic regions and promoters, respectively, in the context of NASH and lipotoxicity (Fig. 4E,F). In order to infer multi-protein transcriptional complexes dysregulated by NASH and lipotoxicity, we performed protein–protein interaction (PPI) network analysis. This approach revealed AP-1 transcription factor members as the only common significant PPI network in both distal intergenic regions and promoters (Fig. 4G,H). In contrast, we found that CON/BSA-specific transcription factors formed distinct PPI networks (Figs. 4G,H, S1A and S1B; distal intergenic: 5 and promoters: 4). Indeed, a number of transcription factors with known function in the regulation of liver function and NAFLD development were members of PPI networks at distal intergenic regions and promoters, including HNF4A, SMADs, ATF3, RXRA and ARNTL (Figs. 4G,H, S1A and S1B)^11,12,13,14.

To refine the identification of relevant transcription factor candidates in an unbiased manner, we performed transcription factor motif enrichment analysis with each of the independent datasets generated from human liver and mouse hepatocytes (Table S4). The overlap between these datasets uncovered 227 motifs representing 170 transcription factors commonly enriched both in human liver and mouse hepatocytes (Fig. 5A). We next used our transcriptomic data to perform Integrated System for Motif Activity Response Analysis (ISMARA), which specifically infers transcription factor activity at proximal promoter regions located 500 base pairs upstream and downstream of transcription start sites¹⁵. This approach identified 36 and 172 motifs representing 63 and 249 transcription factors predicted to have altered activity in NASH and lipotoxicity, respectively (Table S5). By integrating these analyses, we found 35 transcription factors deregulated by NASH and lipotoxicity, among which a subset of 13 also exhibited motif enrichment within regions of accessible chromatin (Fig. 5A). Clustering analysis based on ISMARA-predicted activity showed a small fraction of transcription factors in which NASH and PAL induced the same effect (Fig. 5B). Assessment of changes in the RNA levels of these transcription factors implies that, generally, the predicted activity does not directly relate to gene expression patterns (Fig. 5B). Transcription factors sharing the same response might reflect redundant regulators due to similarities in their corresponding binding motifs on the DNA. We thus performed clustering analysis based on the consensus sequence of such motifs. Although we were able to define 5 distinct clusters, they did not match clustering patterns based on inferred transcription factor activity (Fig. S2A). This suggests that most of these transcription factors regulate unique transcriptional networks related to hepatocyte lipotoxicity. We additional performed Cis-Regulatory Element Motif Activities analysis (CREMA; https://crema.unibas.ch/crumara/), which infers genome-wide transcription factor activity based on chromatin accessibility data (ATAC-seq). Supporting the analyses described above, CREMA revealed several transcription factors showing the same response to NASH and lipotoxicity, such as CEBPZ, ATF3 and NFIB (Table S5). These data suggest that shared effects of NASH and lipotoxicity on transcription factors activity are extended to regulatory elements beyond proximal promoters. Of note, the results generated here represent a valuable resource to perform additional analyses integrating transcriptomic data and focusing on distal regulatory elements, such as the Integrated analysis of Motif Activity and Gene Expression changes of transcription factors (IMAGE)¹⁶.

Subsequently, we selected a subset of transcription factor candidates that exhibit equal changes in activity both in NASH and lipotoxicity. We then either overexpressed (OE) repressed transcription factors (EGR2, KLF4, NFYA, NFYB, SP3 and TFEB) or knocked out (KO) those that were activated (MAFK and TCF4) in mouse hepatocytes (Fig. S2B). This strategy allowed us to determine whether OE or KO of candidate transcription factors would confer protection against PAL-induced lipotoxicity. Only NFYA OE induced a minor decrease in the cytotoxic response to PAL (Fig. 5C). We found that genetic deletion of either MAFK or TCF4 was sufficient to lower the cytotoxic response to PAL in mouse hepatocytes (Fig. 5C). When TFEB was OE, we observed a slight decreased content of intracellular lipids (Fig. 5D), whereas OE or KO of the other transcription factors had no effect on intracellular lipid storage (Fig. 5D). Of note, to determine the reproducibility of our findings in the small sample size (n = 4) of human NASH, we carried out an additional ISMARA analysis with a different RNA-seq dataset (GEO accession: GSE126848) from a large cohort of human liver samples, comprising a mild (NAFL, n = 15) and advance (NASH, n = 16) stage of NAFLD¹⁷. Supporting our original results, this new transcription factor activity analysis showed that the predicted activity of MAFK and TCF4 was significantly increased in human liver from both NAFL and NASH patients (Fig. 5E). Interestingly, CREMA analysis of our ATAC-seq data revealed that only NASH is predicted to activate MAFK and TCF4 (Table S5). This suggest that the effects of PAL on MAFK and TCF4 are primarily driven by their function at proximal promoters. Since the liver exhibits a high degree of cellular heterogeneity, we then performed ISMARA analysis using RNA-seq data from hepatocytes isolated from a diet-induced NASH mouse model (GEO accession: GSE162876)¹⁸. Consistently, this analysis also predicts that NASH induces the activation of both MAFK and TCF4 specifically in hepatocytes (Fig. 5F). Importantly, these independent validations of our findings further demonstrates that MAFK and TCF4 are lipotoxicity-sensitive transcription factors in hepatocytes, exhibiting a conserved response in liver from NAFLD patients.

MAFK and TCF4 regulate distinct transcriptional networks linked to hepatocyte lipotoxicity

Next, we performed a proof of principle study to assess whether our data represent a useful resource to dissect mechanistic insights linked to the development of hepatocyte lipotoxicity and NASH. We achieved this by performing transcriptome analysis of CON and KO cells in the absence (BSA) or presence of PAL. TCF4 KO had a mild effect under basal condition, inducing the up- and down-regulation of 106 and 27 genes, respectively (Fig. S3A and Table S6). The total number of DEG induced by PAL was slightly higher in TCF4-KO cells, with about 26% of DEG being regulated in a TCF4-sensitive manner (Figs. 6A, S3B, S3C and Table S6). Moreover, direct comparison of cells stimulated with PAL revealed 80 and 97 gene showing a higher and lower expression in TCF4-KO cells, respectively (Fig. S3D and Table S6), representing commonly regulated genes also sensitive to TCF4 deletion. We performed gene ontology analysis with all DEG sensitive to PAL in CON and TCF4-KO cells to identify biological processes regulated in a TCF4-dependent manner. Interestingly, we observed that genetic deletion of TCF4 prevented induction of genes linked to cell death, stress and protein translation in response to PAL, while preventing the repression of genes promoting cell growth and survival (Fig. 6B).

We next carried out an analogous characterisation of MAFK-KO hepatocytes in the context of lipotoxicity. KO of MAFK under basal conditions resulted in the up- and down-regulation of 37 and 30 genes, respectively (Fig. S3E and Table S7). Transcriptome remodelling of PAL-stimulated cells was slightly higher in CON and, similarly to TCF4-KO cells, about 20% of DEG were regulated in a MAFK-sensitive manner (Figs. 6C, S3F, S3G and Table S7). We additionally found 21 and 17 up- and down-regulated genes, respectively, in MAFK-KO cells when compared to CON, both following PAL stimulation (Fig. S3H and Table S7). Similarly, the enrichment of terms associated to cell stress, toxicity and blunted growth was prevented in MAFK-KO cells (Fig. 6D). Therefore, our data suggest that KO of both TCF4 and MAFK induces distinct gene expression signatures linked to the protective effect against lipotoxicity.

Considering the link between hepatocyte lipotoxicity and liver fibrosis in NASH prognosis, we subsequently defined the association between TCF4- and MAFK-sensitive genes and human NASH at different stages of fibrosis. We leveraged RNA-seq data (GEO accession: GSE135251) from a large human study comprising liver samples from NASH patients with moderate fibrosis (F2), severe fibrosis (F3) and cirrhosis (F4) (Fig. 7A)¹⁰. We found 90 and 16 up- and down-regulated genes, respectively, shared in humans NASH F4 and mouse hepatocyte lipotoxicity (Fig. 7B). Among these genes, the up- and down-regulation of 17 and 3 was controlled by TCF4, respectively (Fig. 7B). Interestingly, the expression of TCF4-sensitive genes appears to be directly related to liver fibrosis, where a higher degree of fibrosis is associated with a stronger effect in human liver (Fig. 7C). While CON hepatocytes stimulated with PAL recapitulated the expression patterns of a subset of genes observed in liver from NASH F4 patients, genetic deletion of TCF4 was able to counteract such a response (Fig. 7C). Similarly, when compared to human NASH F4, we identified 13 and 2 up- and down-regulated genes, respectively, regulated in a MAFK-depended manner (Fig. 7D). MAFK-sensitive gene regulation was also linked to fibrosis in human liver, with genetic deletion of this transcription factor attenuating the effects of lipotoxicity (Fig. 7E). These preliminary loss-of-function studies in mouse hepatocytes demonstrate that our results can be efficiently used for future data-integrated approaches to further dissect the molecular underpinnings of hepatocyte lipotoxicity and NASH.

Discussion

The development of hepatocyte lipotoxicity plays a crucial role in the development liver fibrosis associated to NASH, for which to date there are no approved medications³. The overload of intracellular lipids in hepatocytes due to an oversupply of saturated fatty acids and/or enhanced de novo lipogenesis (e.g. high fructose consumption) induces the acute activation of pathway promoting cellular injury and death such as the UPR, oxidative stress and pro-inflammatory signals¹. However, the molecular underpinnings by which this process is regulated at the transcriptional level in hepatocyte has been poorly characterized, which to some extent has limited the identification of therapeutic targets for NASH. The current study provides a comprehensive profiling of the effects of lipotoxicity on the hepatocyte transcriptome, proteome and chromatin accessibility landscape, revealing several transcriptional networks with potential regulatory function conserved between mouse and human.

Beyond elucidating transcriptional mechanism in hepatocyte lipotoxicity, our findings can be leveraged to identify molecular insights with potential relevance in human disease. However, a key limitation of this study is the small number of human samples, for which we integrated our data with those from two and one independent human and mouse studies, respectively, comprising samples from liver biopsies from NAFL and NASH patients or mice. Thereby, a very stringent stratification of transcriptional programs and regulators was achieved. While this stringency might result in false negative calling of candidates due to the focus on hepatocytes and acute effects of PAL, this combined approach will reveal transcription factors featuring a regulation and function with potential relevance for the human liver biology and disease. Importantly, the integration of transcriptome and chromatin accessibility analyses allowed us to discover lipotoxicity-sensitive transcription factor networks and their downstream biological processes in hepatocytes.

Liver metabolism and function is regulated by a variety of transcriptional factors, some of which have been implicated in the development of NAFLD^11,19. The pathogenic relevance of transcription factors is supported by several studies demonstrating that NAFLD is associated with altered chromatin function and, thus, gene expression^4,5,6,7. By performing a small pilot study, we identified TCF4 and MAFK as lipotoxicity-sensitive transcription factors in hepatocytes. To our knowledge, none of these transcription factors have been implicated in the development of hepatocyte lipotoxicity. However, a recent preprint article reports that liver from NASH-prone patients exhibit an enrichment of several transcription factor motifs located at enhancers that are shared with our data, including MAFK, TCF3 (with similar motif to TCF4), JUND, ATF3 and BACH2 among others²⁰. Of particular interest, we found that, in the context of lipotoxicity, TCF4 and MAFK regulated the expression of a subset of genes regulating cell stress, survival and homeostasis. For instance, TCF4-KO cells did not show an increase and decrease of genes linked to enhanced protein synthesis and cell growth, respectively. An abnormal increase in protein synthesis can overload the ER and thereby activate the UPR that consequently impairs cell growth and viability^21,22. MAFK-sensitive genes did reveal a similar effects, characterized by the prevention of up- and down-regulation of genes involved in oxidative stress and cell growth, respectively. Therefore, our global unbiased analyses revealed a wide collection of MAFK- and TCF4-sensitive gene providing novel mechanistic insight into hepatocyte lipotoxicity.

An important strategy of our study was to determine candidate transcription factors and downstream target genes exhibiting a conserved response to NASH/lipotoxicity between human liver and mouse hepatocytes. Candidates showing such level of conservation are expected to play a central role in the regulation of hepatocyte function, with a possible link to disease development. In line with this idea, we found several genes with a known regulatory role in liver fibrosis (Sema7a, Cdh11)^23,24,25 and NAFLD development (Adam28, Lgals3, Cxcl10)^26,27,28,29 among MAFK- and TCF4-sensitive genes that are also regulated in human NASH. Notably, while the TCF4-sensitive gene Cxcl10 has been proposed as a NASH biomarker²⁹, the Lgals3 (also known as Galectin 3) inhibitor Belapectin is a promising medication for NASH currently under investigation and development for phase 3 clinical trials^3,30. Collectively, this proof of principle study demonstrate that the datasets generated in this study are a valuable resource to dissect molecular mechanisms by which saturated fatty acids oversupply induces hepatocyte cytotoxicity, while uncovering genes with potential clinical relevance. In particular, we predict that integration of our data with work leveraging cell type-specific analyses such as single cell RNA-seq and ATAC-seq will be of particular relevance. However, future studies will be required to further investigate the relevance and therapeutic potential of the transcriptional networks identified in this study, for instance using mouse or human primary hepatocytes and preclinical mouse models of NASH.

In conclusion, our findings have uncovered a new layer of complexity in hepatocyte lipotoxicity, where transcriptional networks sensitive to saturated fatty acids promote cell death. By performing thorough comparisons to human datasets and experimental validation, we identified a number of transcriptional networks and biological processes associated with the development of hepatocyte lipotoxicity. Furthermore, our data provide a rich resource to generate new hypotheses for future studies aiming at tackling liver lipotoxicity, the central pathogenic factor of NASH and liver-related death.

Methods

Human samples

Fresh frozen and pulverized human liver samples were purchased from Sekisui XenoTech. Samples were obtained from normal (lot #: H1281, H1296, H1310 and H1336) and non-alcoholic steatohepatitis (lot #: H0847, H0958, H1027 and H1060) donors, with appropriate consent and ethical approval obtained by Sekisui XenoTech. Detailed information about donors and biopsies characterization can be found at https://www.xenotech.com/in-vitro-test-systems/tissue-samples/tissue-preparations/ under “see donor list for availability of hepatocytes” and the associated data sheets.

Cell culture and palmitate treatment

FL83B mouse hepatocytes (ATCC^®, #CRL-2390™) were grown in F-12K medium (Thermo Fisher Scientific, #21127030) supplemented with 10% fetal bovine serum (growth medium). Cells were maintained at 37 °C, 95% O₂ and 5% CO₂.

A stock solution of 25 mM sodium palmitate (PAL) (Sigma-Aldrich, #P9767) was prepared in serum-free F-12K media containing 1% fatty acid free bovine serum albumin (BSA) (Sigma-Aldrich, #A8806), which was incubated at 70 °C for 30 min shaking at 1000 rpm before use. Next, cells were incubated in 0, 200 and 400 µM PAL diluted in growth medium for 24 h. One percent BSA diluted in growth medium was used as control.

Cytotoxicity assay

Cytotoxicity was measured with CellTox™ Green Cytotoxicity Assay (Promega, #G8742), according to the manufacturer’s instructions.

Intracellular lipid staining

Cells were incubated with a staining solution containing 1 μg/ml of Hoechst 33342 (Thermo Fisher Scientific, #H3570) and 500 ng/ml of Nile Red (Sigma-Aldrich, #N3013) in phosphate buffered saline (PBS) for 20 min covered from light at 37 °C and 5% CO₂. Next, staining solution was removed and cells were washed twice with PBS. Fresh PBS was added before measuring Nile Red (excitation/emission = 488/550 nm) and Hoechst 33342 (excitation/emission = 350/461 nm) fluorescence with a microplate reader. Nile Red signal (lipids) was normalized to Hoechst 33342 signal (DNA) to account for differences in cell number.

Transient transfections

Transfection of FL83B cells was performed using Opti-MEM™ (Thermo Fisher Scientific, #31985070) and polyethylenimine (Polysciences, # 23966). Plasmids and polyethylenimine were diluted in Opti-MEM™, following which they were mixed in a 1:3 ratio of μg DNA:μg polyethylenimine and incubated for 20 min at room temperature before adding to the cells. Cells were transfected 24 h after seeding with 0.1 or 1 μg per well of a 96 and 12 well plate, respectively, of pcDNA 3.1, pAd-Klf4 (Addgene, # 19770, gift from Konrad Hochedlinger), pFLAG/HA/mSp3 (VectorBuilder, #VB200204-1104aty), pFLAG/HA/mTfeb (VectorBuilder, #VB200204-1105cfn), pFLAG/HA/mEgr2 (VectorBuilder, #VB200204-1106upe), pFLAG/HA/mNfya (VectorBuilder, #VB200204-1107xne) or pFLAG/HA/mNfyb (VectorBuilder, #VB200204-1108efg) for a total of 48 h. Palmitate treatment was started 24 h after transfection.

Generation of knockout cells

Gene knockout (KO) was achieved by using the CRISPR-Cas9 system. To KO the mouse Tcf4 gene, FL83B cells were transfected as described above with the following plasmids: p-hCas9-mTcf4-gRNA#32572-mTcf4-gRNA#30405 (VectorBuilder, #VB200206-1079fgw) and p-hCas9-Scramble-gRNA1-Scramble-gRNA2 (VectorBuilder, #VB200206-1080bvj) as non-targeting control. Deletion of the mouse Mafk gene was performed using the Edit-R gene editing system (Horizon Discovery). First, stable Cas9 expression was induced by transducing FL83B cells with lentiCas9-Blast (Addgene, #52962-LV, gift from Feng Zhang) lentivirus at a multiplicity of infection (MOI) of 0.5 in growth medium containing 10 µg/ml of polybrene (Sigma-Aldrich, #107689). Next, cells were selected with 6 μg/ml of blasticidin (Thermo Fisher Scientific, #A1113903) and a monoclonal cell line was obtained via limiting dilution. Cas9 expressing FL83B cells were subsequently transduced with Mafk (#VSGM10144-246720110) or non-targeting control (#VSGC10215) lentiviral sgRNA at an MOI of 0.5 in growth medium containing 10 µg/ml of polybrene. Seventy two hours after Tcf4 or Mafk targeting, cells were selected with 1 μg/ml of puromycin (Thermo Fisher Scientific, #A1113803) to generate a polyclonal population of KO cells for downstream experiments.

RNA purification and quantitative PCR (qPCR)

Liver tissue and cells were lysed in 1 ml of TRI Reagent (Sigma #T9424) and incubated for 5 min at room temperature. Aqueous phase was obtained with chloroform following the manufacturer’s instructions, following which RNA was purified and reverse transcribed using Direct-zol™ RNA MiniPrep (Zymo Research, #R2050) and iScript™ cDNA Synthesis Kit (Bio-Rad, #1708891), respectively. Relative changes in mRNA content was quantified by qPCR on a StepOnePlus system (Applied Biosystems) using Fast SYBR™ Green Master Mix (Thermo Fisher Scientific, #4385612). The ΔΔCT method was used for analysis, with TATA binding protein (Tbp) as endogenous control.

RNA sequencing (RNA-seq)

Libraries from human liver tissue and wild type FL83B cells were prepared with TruSeq Stranded Total RNA Library Prep Gold (Illumina, #20020599), single-read sequencing was performed using the NextSeq 500 (Illumina). Libraries from knockout FL83B cells and their corresponding non-targeting controls were prepared with TruSeq Stranded mRNA Library Kit (Illumina, #20020595), pair-end sequencing was performed using the NovaSeq 6000 (Illumina). All data was analysed on the Galaxy platform (https://usegalaxy.eu/). Reads were trimmed with Trim Galore! (Galaxy version 0.4.3.1) and quality was assessed using FastQC (Galaxy version 0.72 + galaxy1). Reads were aligned to the hg38 or mm10 version of the human and mouse genome, respectively, using STAR (Galaxy version 2.7.7a) (Table S8). Strand specificity and read counting was performed with Infer Experiment (Galaxy version 2.6.4.1) and featureCounts (Galaxy version 2.0.1), respectively. Next, we used DESeq2 (Galaxy version 2.11.40.6 + galaxy1) for differential expression analysis (fold change ≥ 1.5, p-value < 0.05 for human liver tissue and q-value < 0.05 for FL83B cells) and the resulting data was annotated with Annotate DESeq2/DEXSeq output tables (Galaxy version 1.1.0). Overlap between different datasets was determined with Venny (version 2.1, https://bioinfogp.cnb.csic.es/tools/venny/) and volcano plots generated with Volcano Plot (Galaxy Version 0.0.3). Generation of circular plots and Gene Ontology (GO) analysis was performed with Metascape (https://metascape.org/gp/index.html#/main/step1)³¹. Transcription factors activity analysis was achieved with ISMARA (https://ismara.unibas.ch/mara/), where z-value ≥ 1.5 was consider as significant. We used DESeq2 normalized counts to generate heat maps and for hierarchical clustering using Morpheus (https://clue.io/morpheus).

Mass spectrometry analysis of whole cell proteome

Fifteen milligrams of powdered human liver tissue were lysed in 200 μl of lysis buffer [8 M Urea, 50 mM Tris–HCl pH7.5, 150 mM NaCl and 1 × Halt™ Protease Inhibitor Cocktail (Thermo Fisher Scientific, #87786)], vortexed at max speed for 15 s and incubated for 30 min at 4 °C with shaking at 14,000 rpm. Next, samples were sonicated (amplitude 100%, Cycle 0.5) four times for 30 s in a vial tweeter sonicator with 2 min pause on ice between cycles. Samples were then centrifuged for 13,000g for 10 min at 4 °C, supernatant was transferred to a new tube and the pellet was homogenized in 50 μl of lysis buffer. Following an additional centrifugation at 13,000g for 10 min at 4 °C, supernatant was combined with the previous supernatant. Samples were centrifuged a final time at 13,000g for 10 min at 4 °C and supernatant was used for mass spectrometry. On the other hand, mouse hepatocytes were seeded in 6 well plates and harvested in 80 μl of lysis buffer per well (1% sodium deoxycholate (SDC), 0.1 M TRIS, 10 mM TCEP, pH = 8.5), following lysis with 10 cycles of sonication (Bioruptor, Diagnode). All samples were reduced for 10 min at 95 °C and alkylated at 15 mM chloroacetamide for 30 min at 37 °C. Proteins were digested by incubation with sequencing-grade modified trypsin (1/50 w/w; Promega, V5113) for 12 h at 37 °C. Tryptic digests were acidified (pH < 3) using TFA and cleaned up using iST cartridges (PreOmics, P.O.00027) according to the manufacturer’s instructions. Samples were dried under vacuum and stored at − 20 °C.

Sample aliquots comprising 25 μg of peptides were labelled with isobaric tandem mass tags (TMT 10-plex, Thermo Fisher Scientific, #90110) as described previously³². Shortly, peptides were re-suspended in 20 μl labelling buffer (2 M urea, 0.2 M HEPES, pH 8.3) and 5 μl of each TMT reagent were added to the individual peptide samples followed by a 1 h incubation at 25 °C, shaking at 500 rpm. To quench the labelling reaction, 1.5 μl aqueous 1.5 M hydroxylamine solution was added and samples were incubated for another 10 min at 25 °C shaking at 500 rpm followed by pooling of all samples. The pH of the sample pool was increased to 11.9 by adding 1 M phosphate buffer (pH 12) and incubated for 20 min at 25 °C shaking at 500 rpm to remove TMT labels linked to peptide hydroxyl groups. Subsequently, the reaction was stopped by adding 2 M hydrochloric acid until a pH < 2 was reached. Finally, peptide samples were further acidified using 5% TFA, desalted using Sep-Pak Vac 1cc (50 mg) C18 cartridges (Waters, #WAT054960) according to the manufacturer’s instructions and dried under vacuum.

TMT-labelled peptides were fractionated by high-pH reversed phase separation using a XBridge Peptide BEH C18 column (3.5 µm, 130 Å, 1 mm × 150 mm; Waters, #186003562) on an Agilent 1260 Infinity HPLC system. Peptides were loaded on column in buffer A (20 mM ammonium formate in water, pH 10) and eluted using a two-step linear gradient from 2 to 10% in 5 min and then to 50% buffer B (20 mM ammonium formate in 90% acetonitrile, pH 10) over 55 min at a flow rate of 42 µl/min. Elution of peptides was monitored with a UV detector (215 nm, 254 nm) and a total of 36 fractions were collected, pooled into 12 fractions using a post-concatenation strategy as previously described³³ and dried under vacuum.

Dried peptides were re-suspended in 0.1% aqueous formic acid and subjected to LC–MS/MS analysis using a Q Exactive HF Mass Spectrometer fitted with an EASY-nLC 1000 (Thermo Fisher Scientific) and a custom-made column heater set to 60 °C. Peptides were resolved using a RP-HPLC column (75 μm × 30 cm) packed in-house with C18 resin (ReproSil-Pur C18–AQ, 1.9 μm resin; Dr. Maisch, r119.aq.) at a flow rate of 0.2 μl min⁻¹. The following gradient was used for separation of murine peptides: from 5% B to 15% B over 10 min to 30% B over 60 min to 45% B over 20 min to 95% B over 2 min followed by 18 min at 95% B, whereas the following gradient was used for separation of human peptides: from 5% B to 15% B over 14 min to 30% B over 80 min to 45% B over 26 min to 95% B over 2 min followed by 18 min at 95% B. Buffer A was 0.1% formic acid in water and buffer B was 80% acetonitrile, 0.1% formic acid in water.

The mass spectrometer was operated in DDA mode with a total cycle time of approximately 1 s. Each MS1 scan was followed by high-collision-dissociation (HCD) of the 10 most abundant precursor ions with dynamic exclusion set to 30 s. For MS1, 3e6 ions were accumulated in the Orbitrap over a maximum time of 100 ms and scanned at a resolution of 120,000 FWHM (at 200 m/z). MS2 scans were acquired at a target setting of 1e5 ions, maximum accumulation time of 100 ms and a resolution of 30,000 FWHM (at 200 m/z). Singly charged ions and ions with unassigned charge state were excluded from triggering MS2 events. The normalized collision energy was set to 35%, the mass isolation window was set to 1.1 m/z and one microscan was acquired for each spectrum.

The acquired raw-files were converted to the mascot generic file (mgf) format using the msconvert tool [part of ProteoWizard, version 3.0.4624 (2013-6-3)] and searched using MASCOT either against a murine database (consisting of 49434 forward and reverse protein sequences downloaded from Uniprot on 20141124) or a human database (consisting of 40832 forward and reverse protein sequences downloaded from Uniprot on 20181213) and 390 commonly observed contaminants. The precursor ion tolerance was set to 10 ppm and fragment ion tolerance was set to 0.02 Da. The search criteria were set as follows: full tryptic specificity was required (cleavage after lysine or arginine residues unless followed by proline), 3 missed cleavages were allowed, carbamidomethylation (C) and TMT6plex (K and peptide N-terminus) were set as fixed modification and oxidation (M) as a variable modification. Next, the database search results were imported into the Scaffold Q+ software (version 4.3.2, Proteome Software Inc.) and the protein false discovery rate was set to 1% based on the number of decoy hits. Proteins that contained similar peptides and could not be differentiated based on MS/MS analysis alone were grouped to satisfy the principles of parsimony. Proteins sharing significant peptide evidence were grouped into clusters. Acquired reporter ion intensities in the experiments were employed for automated quantification and statistical analysis using a modified version of our in-house developed SafeQuant R script v2.3³². This analysis included adjustment of reporter ion intensities, global data normalization by equalizing the total reporter ion intensity across all channels, summation of reporter ion intensities per protein and channel, calculation of protein abundance ratios and testing for differential abundance using empirical Bayes moderated t-statistics. The calculated p-values were corrected for multiple testing using the Benjamini–Hochberg method, with significance defined as fold change ≥ 1.3, p-value < 0.05 for human liver tissue and q-value < 0.05 for FL83B cells. Volcano plots were generated on the Galaxy platform (https://usegalaxy.eu/) with Volcano Plot (Galaxy Version 0.0.3). Generation of circular plots and Gene Ontology (GO) analysis was performed with Metascape (https://metascape.org/gp/index.html#/main/step1)³¹. Overlap between different datasets was determined with Venny (version 2.1, https://bioinfogp.cnb.csic.es/tools/venny/).

Assay for transposase-accessible chromatin by sequencing (ATAC-seq)

Nuclei from human liver (15 mg) were isolated using with the Nuclei EZ Prep kit (Sigma-Aldrich, #NUC101) and a glass dounce homogenizer (25 strokes with lose pastel and 25 strokes with tight pastel in ice-cold Nuclei EZ Lysis Buffer). Nuclei were filter through a 40 μm cell strainer and counted before ATAC-seq. On the other hand, Fl83B mouse hepatocytes were seeded in 60 mm plates 24 h before BSA or PAL treatment. Nuclei from human liver and mouse hepatocytes were then used for ATAC-seq and library preparation as previously described³⁴. Pair-end sequencing of the libraries was performed using the Illumina NextSeq 500. All data was analysed on the Galaxy platform (https://usegalaxy.eu/). Reads were trimmed with Cutadapt (Galaxy version: 1.16.5) and quality was assessed using FastQC (Galaxy version 0.72 + galaxy1). Reads were aligned to the hg38 or mm10 version of the human and mouse genome, respectively, using Bowtie2 (Galaxy version 2.3.4.3 + galaxy0) (Table S8). Low quality reads (phred < 30) were filtered out with Filter (Galaxy Version 2.4.1) and duplicated reads were removed with MarkDuplicates (Galaxy version 2.18.2.2). As an additional quality control, we used CollectInsertSizeMetrics (Galaxy Version 2.18.2.1) and plotFingerprint (Galaxy Version 3.5.1.0.0) (Fig. S4). Next, we used Genrich (Galaxy version 0.5 + galaxy2) for peak calling (q-value < 0.05) by pooling individual BAM files (replicates) of the same experimental group, while ChIPseeker (Galaxy version, #1.18.0 + galaxy1) was used to annotate peaks. The overlap between different ATAC-seq datasets was performed with bedtools Intersect intervals (Galaxy version 2.29.0). Heat map and density plots of ATAC-seq peaks were created with plotHeatmap (Galaxy version 3.0.2.0) and plotProfile (Galaxy version 3.1.2.0.0), respectively. Data was visualized on the Integrated Genome Browser-9.1.4³⁵ to generate representative genome browser figures, for which BAM files were merged with Merge BAM Files (Galaxy version 1.2.0) and then normalized using bamCoverage (Galaxy version 3.0.2.0). CentriMo (version 5.1.0, https://meme-suite.org/meme/doc/centrimo.html) was used to perform motif enrichment analysis (E-value threshold < 0.05)³⁶. Generation of circular plots and protein–protein interaction network analysis was performed with Metascape (https://metascape.org/gp/index.html#/main/step1)³¹. GO analysis was performed with DAVID 6.8 (https://david.ncifcrf.gov/). Transcription factor activity analysis was performed with Cis-Regulatory Element Motif Activities (CREMA; https://crema.unibas.ch/crumara/). Finally, clustering of transcription factor motifs based in their consensus sequence was performed using STAMP (http://www.benoslab.pitt.edu/stamp/)³⁷.

Ethics statement

Human liver tissue was collected with appropriate informed consent and ethical approval obtained by Sekisui XenoTech. Cell culture experiments, downstream processing of cell and human samples, and other experimental protocols and methods were performed according to the current institutional guidelines and regulations of the Biozentrum, University of Basel. Work with biosafety level 1 and 2 specimen was approved by the Swiss Federal Office of Public Health and performed according to institutional and federal guidelines.

Statistics

All qPCR, cytotoxicity and intracellular lipid assays were performed at least three independent times each in triplicate. Number of replicates per experiment is indicated in the figure legend when appropriate. Values are expressed as mean ± SD. Statistical significance was determined with unpaired two-tailed t tests, with significance considered with a p < 0.05. RNA-seq, ATAC-seq and mass spectrometry experiments were performed once with three to four biological replicates as indicated in figure legends. Statistical analysis of these experiments is described above in their corresponding sections.

Data availability

RNA-seq and ATAC-seq data are available at the Gene Expression Omnibus (GEO) under accession number GSE173736. Whole proteome analysis is available at the Proteomics Identification Database (PRIDE) under accession number PXD026717. All other materials generated in this study are available from the corresponding authors upon request.

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Acknowledgements

We thank Christian Beisel (Genomics Facility Basel, ETH Zürich) and Philippe Demougin (Life Sciences Training Facility, Biozentrum, University of Basel) for technical help. We thank Eva Dazert for advice about processing of human liver samples (Biozentrum, University of Basel). This work was supported by grants from the Novartis Foundation for Medical-Biological Research and the Research Fund of the University of Basel to J.P.S. Grants from the Swiss National Science Foundation (SNSF, grant 310030_184832), the European Research Council (ERC) Consolidator grant 616830-MUSCLE_NET, Swiss Cancer Research grant KFS-3733-08-2015, the Swiss Society for Research on Muscle Diseases (SSEM), SystemsX.ch, the Novartis Stiftung für Medizinisch-Biologische Forschung and the University of Basel supported C.H.

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Joaquín Pérez-Schindler
Present address: Broad Institute of MIT and Harvard, Cambridge, MA, 02142, USA

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Biozentrum, University of Basel, 4056, Basel, Switzerland
Joaquín Pérez-Schindler, Elyzabeth Vargas-Fernández, Bettina Karrer-Cardel, Danilo Ritz, Alexander Schmidt & Christoph Handschin

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Joaquín Pérez-Schindler
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Elyzabeth Vargas-Fernández
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Bettina Karrer-Cardel
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Contributions

J.P.S. and C.H. conceived, designed and supervised the study. J.P.S., E.V.F., B.K.C., D.R. and A.S. performed experiments. J.P.S., D.R., A.S. and C.H. performed data analysis and interpretation. J.P.S. and C.H. wrote the manuscript. All authors reviewed the manuscript.

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Pérez-Schindler, J., Vargas-Fernández, E., Karrer-Cardel, B. et al. Characterization of regulatory transcriptional mechanisms in hepatocyte lipotoxicity. Sci Rep 12, 11477 (2022). https://doi.org/10.1038/s41598-022-15731-4

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Received: 24 November 2021
Accepted: 28 June 2022
Published: 07 July 2022
DOI: https://doi.org/10.1038/s41598-022-15731-4

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