Clinical studies demonstrated that nonalcoholic steatohepatitis is associated with liver-related outcomes in chronic hepatitis B. Furthermore, primary biliary fibrosis and biliary atresia occurred in patients with HBV infection. Interestingly, hepatitis B virus surface protein (HBs) transgenic mice spontaneously develop hepatic steatosis. Our aim is to investigate the effect of Abcb4 knockout-induced cholestasis on liver steatosis in HBs transgenic mice. Hybrids of HBs transgenic and Abcb4−/− mice were bred on the BALB/c genetic background. Lipid synthesis, storage, and catabolism as well as proteins and genes that control lipid metabolism were analyzed using HPTLC, qPCR, western blot, electrophoretic mobility shift assay (EMSA), lipid staining, and immunohistochemistry. Hepatic neutral lipid depots were increased in HBs transgenic mice and remarkably reduced in Abcb4−/− and HBs/Abcb4−/− mice. Similarly, HPTLC-based quantification analyses of total hepatic lipid extracts revealed a significant reduction in the amount of triacylglycerols (TAG), while the amount of free fatty acids (FFA) was increased in Abcb4−/− and HBs/Abcb4−/− in comparison to wild-type and HBs mice. PLIN2, a lipid droplet-associated protein, was less expressed in Abcb4−/− and HBs/Abcb4−/−. The expression of genes-encoding proteins involved in TAG synthesis and de novo lipogenesis (Agpat1, Gpat1, Mgat1, Dgat1, Dgat2, Fasn, Hmgcs1, Acc1, Srebp1-c, and Pparγ) was suppressed, and AMPK and CREB were activated in Abcb4−/− and HBs/Abcb4−/− compared to wild-type and HBs mice. Simulating cholestatic conditions in cell culture resulted in AMPK and CREB activation while FASN and PLIN2 were reduced. A concurrent inhibition of AMPK signaling revealed normal expression level of FASN and PLIN2, suggesting that activation of AMPK–CREB signaling regulates hepatic lipid metabolism, i.e. synthesis and storage, under cholestatic condition. In conclusions, in vivo and mechanistic in vitro data suggest that cholestasis reduces hepatic lipid storage via AMPK and CREB signaling. The results of the current study could be the basis for novel therapeutic strategies as NASH is a crucial factor that can aggravate chronic liver diseases.
The injury of bile ducts is a hallmark of chronic cholestatic liver disorders of multifactorial origin leading to hepatic accumulation of bile acids (BA) and subsequent liver tissue damage [1, 2]. Bile production is a complex process involving hepatocytes, cholangiocytes, and a number of different bile acid transporters that coordinate bile formation . ATP-binding cassette subfamily B member 4 (ABCB4) is a phospholipid translocator at the canalicular membrane of the hepatocyte, which “flops” phosphatidylcholine into the bile. Phosphatidylcholines are essential for the formation of bile acid-containing micelles, a crucial process in protecting cholangiocyte membranes from being exposed to high concentrations of free cell-toxic BA . Dysfunction or deficiency of this transporter can cause liver diseases such as progressive familial intrahepatic cholestasis type 3, low phospholipid-associated cholelithiasis, intrahepatic cholestasis of pregnancy, drug-induced liver injury, and chronic cholangiopathy with biliary fibrosis and cirrhosis . Similar to human cholestatic liver diseases, Abcb4 knockout mice develop liver fibrosis, multiple derangements of lipid metabolism, including alterations in cholesterol and phospholipid metabolism [3, 4]. Chronic viral hepatitis (CVH) implies liver damage causing liver fibrosis and subsequent hepatocellular carcinoma formation . It has been shown recently in a large combined tertiary center cohort that patients with concomitant nonalcoholic steatohepatitis (NASH) and chronic hepatitis B infection had poorer clinical outcomes . Interestingly, the transgenic mice overexpressing HBV surface proteins without viral infection  that were used in the current study, developed hepatic steatosis . Apart from steatosis, further histopathological changes have been reported in the same transgenic model including inflammation, regenerative hyperplasia, endoplasmatic reticulum stress, and associated unfolded protein response [9,10,11].
Characteristics of the metabolic syndrome like obesity, hypertension, and lipometabolic disorders are associated with the presence of NASH in patients with chronic hepatitis B . Moreover, concurrent NASH drives a “second hit” to the liver in patients with chronic HBV infection  and even noninvasive score models for the prediction of NASH in patients with chronic hepatitis B and superimposed nonalcoholic fatty liver diseases (NAFLD) have been suggested . NAFLD depicts the leading cause of liver diseases in the Western world . Apart from HBV, also other risk factors like malnutrition, gut microbes, and drugs can aggravate NASH [15,16,17].
Adenosine monophosphate-activated kinase (AMPK) is believed to act as a key master switch that modulates lipid metabolism by directly phosphorylating proteins or modulating gene transcription in specific tissues such as liver, fat, and muscle [18, 19]. SREBP1c, P-ACC1, FASN, SCD1, HMGCS1, GPAT1, etc are involved either in synthesis, oxidation, or lipolysis, which are modulated directly through phosphorylation or modulation at gene transcription level by activated AMPK . In addition, activation of AMPK also activates the expression of CREB . The most abundant proteins associated with lipid droplets (LDs) belong to the perilipin (PLIN) protein family . PLIN proteins (PLIN1–PLIN5) are important regulators of cellular lipid metabolism, directly controlling how and when cells and tissues store, mobilize, and utilize lipids. Previous studies reported on the activated AMPK-mediated phosphorylation of LD associated protein PLIN2 and subsequent triggering of lipolysis , suggesting an interplay between AMPK and PLIN2 in maintaining intracellular triacylglycerols (TAG) storage.
The dysregulation of hepatic and systemic lipid metabolism in Abcb4−/− mice has been described before . Interestingly, the authors reported that liver injury was critically linked to impaired lipid homeostasis, which was ameliorated by norUDCA treatment and additionally by dietary intervention in Abcb4−/− mice under HFD. Similarly, we previously reported that hepatitis B virus surface proteins could accelerate cholestatic liver injury and tumor progression in Abcb4−/− mice reflecting a model of simultaneous liver damage with enhanced carcinogenesis . Based on these findings, the present study was designed to investigate the effect of Abcb4 knockout-induced cholestasis on lipid metabolism in HBs transgenic mice.
Material and methods
BALB/c-Abcb4 mice (C.FVB (129P2)-Abcb4tm1Bor herein called Abcb4−/− mice) were bred and housed as described previously . Characterization of Abcb4−/− genotype, sample collection, and routine analysis has been described elsewhere . Generation and characteristics of transgenic lineages Tg (Alb1HBV) (C57BL/6J-Tg (Alb1HBV) 44Bri/J) have been described . These mice were crossed to BALB/cJ background (C.B6J-Tg (Alb1HBV) 44Bri herein called HBs mice) for nine generations. HBs mice were crossed with Abcb4−/− mice, resulting in the F2 generation BALB/c-Abcb4/Alb1HBV hybrid mice (C.Cg-Tg (Alb1HBV) 44Bri-Abcb4tm1Bor herein called HBs/Abcb4−/− mice). All mice were housed in a pathogen-free environment under a constant 12-h light–dark cycle at 22 °C temperature and 50% humidity. The mice were fed standard chow (Altromin, Lage, Germany) and water ad libitum.
Mice were sacrificed at the age of 12–19 weeks (n = 4–5 per age and sex). Livers were collected and underwent morphological diagnosis. Remaining samples were preserved for analyses as indicated. Serum samples were stored at −80 °C until analysis of serum TAGs and cholesterol using the Reflotron plus Analyzer (Roche, Mannheim, Germany). This study was carried out in strict accordance to the recommendations laid in the guide for the care and use of laboratory animals of the German law of animal welfare. All experiments were approved by the committee on the ethics of animal experiments of the Regierungspraesidium Giessen, Giessen, Germany (permit number: V54-19c 2015c GI20/10 Nr. A36/2011, Nr. A5/2012, and Nr. 52_2011).
Liver and cell lysates were prepared in 1× laemmli buffer and boiled at 95 °C for 10 min, and then briefly centrifuged for 5 min. After SDS-PAGE, proteins were transferred to a nitrocellulose membrane following the standard protocol . Protein detection was performed using specific antibodies against AMPK (Genetex: #GTX50863-100), Phospho-AMPKα (Thr172) (CST: #2531)), Perilipin2/PLIN2 (Proteintech: #15294-1-AP, CIDEC: #198204), Phospho-CREB (Ser133) (87G3) rabbit mAb (CST: #9198), CREB (CST: #9104), and GAPDH (Proteintech: 60004-1-Ig). The proteins were visualized using peroxidase-conjugated secondary antibodies and chemoluminescent reagent developed on Intas ECL chemostar (Göttingen, Germany). Alternatively, visualization was performed using alkaline phosphatase conjugated secondary antibodies with soluble 5-bromo-4-chloro-3-indolyl phosphate and nitroblue tetrazolium.
Immunohistochemistry (IHC) was performed using Impress Peroxidase/Alkaline Detection Reagents (Vector Laboratories) and antibodies specific for PLIN2 (Proteintech: #15294-1-AP), CIDEC (Novus: NBP1-76950), lysosomal acid lipase (LAL) (Novus: NBPI-54155SS), Lipoprotein lipase (LPL) (Proteintech: #21133-1-AP), Phospho-CREB (Ser133) (CST: #9198), DGAT1 (Proteintech: #11561-1-AP), or MGAT1 (Santa Cruz: #sc376079). Color reaction was developed with VECTOR VIP Peroxidase Substrate Kit or DAB Peroxidase Substrate Kit (Vector Laboratories, USA) or HighDef® red IHC AP chromogen (Enzo, USA).
Sample preparation and real-time PCR
RNA isolation was conducted according to the manufacturer’s protocol using the Direct-zol RNA extraction kit (Zymo research). cDNA synthesis was produced using the High capacity cDNA synthesis kit (Thermo, 4374966). Real-time qPCR was performed according to the protocol described before . Primers were ordered from Microsynth (Switzerland). qPCR data were analyzed using the ΔΔCT method . Sequences and properties of primers are listed in Table 1.
Oil red O staining
Oil red O staining was performed as described previously . Staining was assessed by bright-field microscopy.
High performance thin layer chromatography (HPTLC)
The liver tissue extracts were prepared as described  with slight modifications. Briefly, 20 mg of frozen liver tissue were weighed and subsequently homogenized with 1.0 mL n-hexane/2-propanol 3:2 (V/V) for 1 h. This suspension was centrifuged at 4 °C at 10,000 × g for 10 min. The supernatant was transferred to a vial, dried under nitrogen gas and the residue was resuspended in 100 µL of chloroform/methanol 2:1 (V/V). For application on the HPTLC plate, this stock solution was further diluted 1:4 in chloroform/methanol 1:1 (V/V). Individual lipid stock solutions (25 mg/mL) were mixed to obtain a lipid standard mixture of 300 ng/µL each in chloroform/methanol 1:1 (V/V). The sample and standard solutions were sprayed with the Automatic TLC Sampler 4 (ATS4, CAMAG, Muttenz, Switzerland) as 8-mm bands allowing up to 21 tracks to be applied on one HPTLC plate of 20 × 10 cm (distance from lower edge 8 mm, distance from left edge 14.5 mm, automatic distance between bands). For calibration, 0.3, 6, 12, and 21 µg of the standard mixture solution were sprayed on the HPTLC plate (300–2100 ng/band) along with 2.5 µL liver extract samples. After drying of the start zones for 0.5 min (hair dryer), development was performed according to  on an HPTLC plate silica gel 60 F254-MS-grade (Merck, Darmstadt, Germany; preheated to 110 °C for 15 min) with n-hexane/diethyl ether/acetic acid (8:2:0.4, V/V/V) in the Twin-Through chamber (CAMAG, with filter paper) pre-saturated for 20 min. The developing distance was 65 mm (from the lower edge of the plate). After plate drying for 2 min, detection was performed by immersion into primuline reagent (100 mg primuline in 200 mL acetone/water 4:1, V/V) at an immersion speed of 3 cm/s and an immersion time of 1 s using the TLC Chromatogram Immersion Device III (CAMAG). After plate drying for 2 min, the fluorescence measurement was performed at 366/>400 nm using the TLC scanner 4 (CAMAG, mercury lamp, measurement slit 6.0 mm × 0.2 mm, scanning speed 20 mm/s, optical filter K400). The chromatogram was documented at UV 366 nm via the TLC Visualizer (CAMAG). All instrumentation and data processing were operated with the winCATS software (CAMAG, version 22.214.171.1242).
For qualitative visualization, HPTLC plates were derivatized using sulfuric acid-anisaldehyde reagent (201 mL sulfuric acid/acetic acid/methanol/anisaldehyde, 1:2:17:0.1, V/V/V/V). The plate was immersed into the derivatization reagent at a speed of 3.5 cm/s and a time of 1 s, followed by heating at 110 °C for 9 min. The chromatograms were subsequently documented at white light illumination.
The selected zones were online transferred with methanol (flow rate 0.1 mL/min) using the TLC-MS Interface 2 (equipped with an elution head, 4 × 2 mm, CAMAG) coupled to the Q Exactive Plus Hybrid Quadrupole-Orbitrap Mass Spectrometer (Thermo Fisher Scientific). Between the interface and the mass spectrometer, a filter frit (Upchurch Scientific A-356 and PEEK-Frit Blue UPA-703, Techlab, Erkerode, Germany) was installed to prevent the mass spectrometer from particles. As ion source was used atmospheric pressure chemical ionization. The spectrometer was operated and spectra were recorded with Xcalibur 3.0.63 software (Thermo Fisher Scientific). High-resolution mass spectra were measured as full scan at a resolution of 280,000 in the range of m/z 100–1000.
Electrophoretic mobility shift assay (EMSA)
The target oligo’s probe sequence for CREB consensus binding site was provided by Santa Cruz Biotechnology, Inc. (sc-2504). CREB consensus sequences (F) 5′-AGA GAT TGC CTG ACG TCA GAG AGC TG-3′(R) 5′-CTA GCT CTC TGA CGT CAG GCA ATC TCT-3′. PPAR consensus binding sequences: (F) 5′-CAA AAC TG GTC AAA GGT CA-3′, (R) 5′-TGA CCT TTG ACC TG TTT TG-3′. The 5′ ends of all single-stranded probes were biotin labeled. Nonbiotin-labeled probes were also used as competitor probe (Microsynth, Germany).
Nuclear proteins extraction from liver samples was performed using NE-PER™ Nuclear and Cytoplasmic Extraction Reagents (Thermo scientific, cat no. 78833). For the EMSA reaction, 2 μg of the nuclear protein was incubated with reaction reagents as per the protocol given in Light shift Chemiluminescent EMSA Kit (Thermo Scientific, cat no 20148). After a 10 min equilibration to 25 °C, biotin labeled (hot probe) and excess of nonbiotin probes (cold probe) were added and further incubated for 20–30 min at room temperature. After hybridization, the complexes were resolved by electrophoresis on 5% nondenaturing polyacrylamide gels in 0.5× TBE (Tris-borate-EDTA) buffer at 10 V/cm for 1 h. The gel was subsequently transferred to a positively charged nylon membrane using a semidry transfer cell. DNA was detected using Light shift Chemiluminescent EMSA Kit (cat no 20148, Thermo Scientific). Images were processed by Intas Imager (ECL chemostar, Intas, Germany).
Lipase activity assay
Liver samples were weighed and lysates prepared in PBS plus protease inhibitor in cold condition as per protocol (Cayman cat no. 700640).
Free fatty acid (FFA) quantification
Liver samples were weighed and lysates were prepared as per protocol for FFA quantification (Promokine, cat no. PK-CA577-K612).
TAG colorimetric assay
Liver samples were weighed and lysates prepared as recommended by the manufacturer (Cayman, cat no. 10010303). The assay was initiated with the enzymatic hydrolysis of the TAGs by lipase to produce glycerol and FFAs. The glycerol released was subsequently measured by a coupled enzymatic reaction system with a colorimetric readout at 540 nm.
HepG2 cell culture
HepG2 cell lines were obtained from CLS services Germany. HepG2 cells were grown at 37 °C in an atmosphere of 5% CO2, 95% air in cell culture dish using 10 mL of DMEM–F-12 medium with 10% fetal calf serum, 1% penicillin, 1% streptomycin, and 1% fungizone. Cells were plated at a split ratio of 1:4. The preconfluent cells were left either untreated (control cells) or pretreated with oleic acid (BSA conjugated oleic acid, Sigma cat no. O3008-5ML), at a concentration of 250 μM for 12 h. Subsequent treatment with BA (Sigma-Aldrich, cat no. 48305-50G-F) was performed in serum free DMEM–F-12 medium. Similarly, for inhibitor assays, the cells were pretreated with Dorsomorphin (AMPK inhibitor, Merck, P5499, 10 µM) for 1 h prior to treatment with the BA. The plasmid pCH9/200LMS is a replication-defective variant of plasmid pCH9/3091  and encodes the HBV surface proteins under their natural promoters. HepG2 cells with 80% confluence were transfected with and without the plasmid pCH9/200LMS for 48 h, followed by treatment with oleic acid for 12 h. After that treated with bile acid in serum free DMEM for the next 24 h.
The results are presented as means ± SEM. One-way ANOVA followed by Tukey’s multiple comparisons test was performed using GraphPad Prism version 7.00 for Windows, GraphPad Software, La Jolla, CA, USA, and controlled with SPSS26.0, IBM, Ehningen, Germany.
Abcb4 knockout reduced hepatic lipid accumulation in HBs transgenic mice
We investigated the effects of Abcb4−/−-induced cholestasis in two distinct models, Abcb4-deficient mice (Abcb4−/−) and HBs overexpressing mice as well as chimera of both, knockout and transgene, on BALB/c genetic background (HBs, HBs/Abcb4−/−). Oil red O staining revealed a remarkable reduction of neutral lipid depots in the hepatocytes of both, Abcb4−/− and HBs/Abcb4−/−, mice in comparison to wild-type and HBs transgenic mice, respectively, (Fig. 1a).
An HPTLC method with fluorescence detection after derivatization with the primuline reagent (HPTLC-FLD) allowed the separation and detection of five different lipid species (cholesterol, FFAs with oleic acid as reference, TAG, methyl oleate, and cholesteryl oleate) in liver extract samples. The lipid fractions were assigned using a lipid standard mixture (Fig. 1b). These preliminary assignments were confirmed by high-resolution mass spectrometry (Supplementary Fig. 1a–d). The HPTLC-FLD chromatogram and its quantitative analysis revealed a decrease in hepatic TAGs in Abcb4−/− mice as compared to wild type (Fig. 1c). HBs mice presented with higher hepatic TAG levels than Abcb4−/− mice, which were reduced in HBs/Abcb4−/− (Fig. 1c). The hepatic levels of FFA, on the other hand, were significantly increased in Abcb4-deficient mice and HBs/Abcb4−/− in comparison to wild-type and HBs mice, respectively (Fig. 1d). The amount of hepatic cholesterol and cholesteryl oleate was not altered among groups (Fig. 1e, f). Alternative HPTLC assessments of TAGs and FFAs strengthened this outcome and displayed comparable results (Supplementary Fig. 1a, b).
Serum levels of TAGs and cholesterol were reduced in all groups in comparison to WT but not altered in HBs/Abcb4−/− mice compared to HBs and Abcb4−/− mice, respectively, (Fig. 1g, h). Taken together, TAGs were reduced in liver but not in the serum of HBs/Abcb4−/− compared to HBs mice.
Abcb4 knockout altered hepatic lipid metabolism in HBs/Abcb4−/− mice
The reduction of TAGs in hepatocytes of HBs/Abcb4−/− mice in comparison to HBs mice prompted us to investigate the genes involved in de novo lipogenesis, lipid uptake, and transport.
Although Srebp-1c appeared increased in HBs and reduced in HBs/Abcb4−/− by trend, statistical significance was not reached and the expression of Srebp-1c was not altered in Abcb4−/−, HBs, and HBs/Abcb4−/− mice in comparison to wild type (Fig. 2a).
Fatty acid synthase (Fasn) gene expression was reduced in Abcb4−/− and HBs/Abcb4−/− compared to wild type (Fig. 2b). Acc1 and Scd1 were reduced in Abcb4−/− and HBs/Abcb4−/− compared to HBs mice (Fig. 2c, d). Hmgcs1was reduced in HBs/Abcb4−/− compared to HBs mice (Fig. 2e). The transcription factor Pparγ was downregulated in Abcb4−/− and HBs/Abcb4−/− mice compared to HBs (Fig. 2f).
Furthermore, Cd36 (fatty acid translocase) was induced in HBs compared to WT and reduced in Abcb4−/− and HBs/Abcb4−/− mice compared to HBs (Fig. 2g). ApoE was reduced in HBs/Abcb4−/− mice compared to HBs (Fig. 2h). Although Mttp appeared increased in HBs and reduced in HBs/Abcb4−/− by trend, statistical significance was not reached and Mttp (Microsomal TAG transfer protein) was not altered (Fig. 2i). Phosphatidylcholine transfer protein (Pctp), responsible for transfer of phosphatidylcholine, was reduced in Abcb4−/− and HBs/Abcb4−/− compared to HBs (Fig. 2j).
Taken together, our results indicate that Abcb4 knockout suppressed the expression of genes involved in de novo lipogenesis as well as transcription factors and genes involved in lipid transport in HBs/Abcb4−/− mice.
Abcb4 knockout reduced hepatic lipid droplet-associated protein PLIN2, TAG synthesis, and TAG storage in HBs mice
Among PLIN proteins, PLIN2 is the constitutive and ubiquitously expressed protein that has been used as a marker for LDs, correlating with the amount of LDs and TAG storage . We therefore investigated the effect of an Abcb4 knockout on the PLIN2 expression as an additional marker for intracellular lipid storage. Real-time PCR, western blot, and IHC revealed a reduced expression of PLIN2 in HBs/Abcb4−/− compared to HBs transgenic mice (Fig. 3a–c). Western blotting analyses suggested a similar reduction of hepatic PLIN2 in female mice (Supplementary Fig. 2a, b). Plin2 is stained red. The protein expression of PLIN3 and PLIN5, however, was not regulated (data not shown). CIDEC, another LD-associated protein, showed a remarkable reduction in protein expression in Abcb4−/− and HBs/Abcb4−/− mice compared to wild-type and HBs transgenic mice (Fig. 3b). In conclusion, the reduction of PLIN2 might be considered as an indicator of reduced TAG storage in consequence of the Abcb4 knockout.
Thus, we further investigated genes mainly involved in TAG synthesis pathways. Transcription of Mgat1was highly upregulated by HBs (Fig. 4a). Diacylglycerol acyltransferase 1 (DGAT1) and DGAT2 both catalyze the final committed step of TAG synthesis. At transcriptional level, Dgat2 was downregulated in HBs and HBs/Abcb4−/− as compared to WT, while Dgat1 showed no significant regulation (Fig. 4b, c). Similarly, acyl-CoA: glycerol-3-phosphate acyltransferase (GPAT) and acyl-CoA: 1-acyl-glycerol-3-phosphate acyltransferase (AGPAT) are involved in the de novo synthesis of TAGs in the glycerol-3-phosphate pathway. Our results displayed a downregulation of Gpat1 in HBs/Abcb4−/− mice in comparison to WT but only in tendency in comparison to HBs (P = 0.081). Agpat1 was reduced at transcriptional level in both, Abcb4−/− and HBs/Abcb4−/− mice, compared to wild-type and HBs mice (Fig. 4d, e). Taken together our findings suggest that the reduction of TAG synthesis is associated with the reduction of LDs and LD-associated proteins in Abcb4-deficient HBs mice. DGAT1 protein expression, however, showed a remarkable reduction in HBs/Abcb4−/− in comparison to Abcb4−/− and HBs mice (Fig. 4f). The protein expression of MGAT1, which synthesizes DAGs by catalyzing the acylation of monoacylglycerols (MAGs), showed a slight reduction in HBs/Abcb4−/− compared to HBs (Fig. 4g).
Abcb4 knockout enhanced lipolysis in HBs/Abcb4−/− mice
Increased TAG lipolysis with increased FFA accumulation associated with PPARα activation in Abcb4−/− mice was reported earlier . In order to investigate whether the increase in FFA—as observed in HBs/Abcb4−/− mice (Fig. 1d)—was caused by increased TAG lipolysis, we performed a total lipase activity assay using total liver lysates. We found increased lipase activity in Abcb4−/− mice but no differences between HBs and HBs/Abcb4−/− mice (Fig. 5a).
Since FFAs can activate PPARα, which subsequently regulates the peroxisomal beta oxidation pathway of fatty acids , we investigated the PPARα activation in our experimental setup. The transcriptional analysis demonstrated equal expression of Pparα in HBs and HBs/Abcb4−/− (Fig. 5b). Interestingly Pparα expression was reduced in HBs/Abcb4−/− in comparison to Abcb4−/− (Fig. 5b). EMSA indicated an increased nuclear binding activity of PPARα in Abcb4−/− mice but not in HBs/Abcb4−/−-mice (Fig. 5c). PPARα activation subsequently regulates its downstream targets such as LPL and adipose TAG lipase (ATGL) . Lpl expression was significantly increased in Abcb4−/− and HBs/Abcb4−/− compared to WT (Fig. 5d). In addition, the LPL protein expression was remarkably increased in HBs/Abcb4−/− compared to HBs mice (Fig. 5e). PPARα activity is, therefore, in line with LPL expression in Abcb4−/−-mice but not in HBs/Abcb4−/−-mice. Apart from LPL, other lipases such as ATGL or LAL, which are also regulated by PPARα , yielded no significant differences in expression (data not shown). Taken together, our results demonstrated an increased hepatic LPL expression in HBs/Abcb4−/− mice.
Abcb4 knockout activated AMPK and CREB signaling in HBs/Abcb4−/− mice
AMPK is an energy sensor that can induce a cellular cascade for maintaining energy homeostasis . AMPK was activated in Abcb4−/− and HBs/Abcb4−/− compared to WT and HBs (Fig. 6a). CREB and related proteins are downstream targets for AMPK and therefore likely involved in mediating effects of AMPK . Thus, we also investigated the hepatic activation of CREB in Abcb4−/− mice. Immunoblotting demonstrated the increased activation of CREB in Abcb4−/− and HBs/Abcb4−/− compared to wild-type and HBs transgenic mice (Fig. 6a). Similarly, immunohistochemical studies with specific P-CREB antibodies confirmed the above findings (Fig. 6b). Western blot analysis and immunostaining also demonstrated the increased activation of CREB in Abcb4−/−, HBs, and HBs/Abcb4−/− compared to wild type in female mice (Supplementary Fig. 3a, b). In addition, EMSA results showed increased nuclear binding of CREB in HBs/Abcb4−/− compared to Abcb4−/−, wild-type, and HBs transgenic mice (Fig. 6c). Hence, our data suggest that Abcb4−/− induced cholestatic liver injury might affect hepatic lipid metabolism by the activation of AMPK and CREB signaling in HBs transgenic mice.
Bile acid treatment induced AMPK–CREB activation in HepG2 cells
To further prove the mechanistic principle of cholestasis induced disturbances in lipid metabolism in HBs mice, HepG2 cells were used to mimic the situation in vitro. Oleic acid pretreatment of HepG2 cells increased intracellular LDs. The subsequent treatment with BA increased the phosphorylation of AMPK and CREB in HepG2 cells (Fig. 7a). The protein expression of FASN and PLIN2 was reduced in the BA treated group, which was concomitant with the activation of AMPK signaling by bile acid treatment (Fig. 7a). In addition, the LDs associated protein, PLIN2, was reduced remarkably in the treated group compared to vehicle (Fig. 7a). Furthermore, we simulated the in vivo situation by the treatment of HBs overexpressing HepG2 cells with BA. Central aspects like CREB activation and PLIN2 reduction were also demonstrated in this setting (Fig. S4).
To confirm that the effect of bile acid on decreased TAG synthesis and storage was dependent on AMPK–CREB signaling, HepG2 cells preloaded with oleic acid were treated with the specific AMPK inhibitor dorsomorphin in the presence and absence of BA. The activation of AMPK and also CREB by BA was blocked by dorsomorphin (Fig. 7b). Importantly, the downstream targets of AMPK, FASN, and PLIN2, were induced after treatment with the inhibitor (Fig. 7b), suggesting that AMPK activation by BA regulates genes that are involved in lipid synthesis. Our data suggest that bile acid suppresses TAG synthesis and storage in HepG2 cells via activation of the AMPK and CREB signaling pathways.
Cholestasis in NAFLD patients is associated with more pronounced liver injury, inflammation, and disturbances in glucose and lipid metabolism contributing to the progressive course of NAFLD . Clinical studies reported that primary biliary fibrosis and biliary atresia occurred in patients with HBV infection [38, 39]. Similarly, biliary diseases might even be attributed to or caused by HBV infection . We have reported earlier that HBs can enhance cholestatic liver injury, fibrosis, and tumorigenesis in Abcb4 knockout mice . Therefore, there is an urgent need for medical correction of cholestasis at the earliest form of fatty liver diseases. With regard to chronic HBV infection, concurrent NAFLD represents a “second hit” that can aggravate the disease  and the metabolic syndrome is associated with severe fibrosis in CVH . In the current study, we investigated the effect of an Abcb4 knockout on hepatic lipid metabolism in HBs transgenic mice to understand the relevant biological processes with regard to disease development and progression. Our present study demonstrates reduced hepatic lipogenesis, reduced TAG synthesis, and enhanced lipid catabolism in HBs/Abcb4−/− mice. The activation of AMPK–CREB pathway is suggested to be a major player regulating the changes in hepatic lipid metabolism thereby contributing significantly to the pathogenesis of cholestatic liver injury in HBs mice.
Remarkably, our study revealed a reduction of hepatic TAGs in HBs/Abcb4−/− mice (Fig. 1a–c). Serum TAGs and cholesterol were reduced in HBs/Abcb4−/− mice compared to wild types (Fig. 1g, h). Cholestatic liver disease with toxic accumulation of bile components might disturb many aspects of lipid absorption and metabolism . Furthermore, BA are involved in regulating their own synthesis and enterohepatic circulation, but also TAGs, cholesterol, glucose, and energy homeostasis . Interestingly, we observed increased hepatic FFA levels in Abcb4−/− and HBs/Abcb4−/− mice (Fig. 1d). The induction of hepatic fatty acyl-CoAs and the reduction of TAG esterification and storage has already been described in Abcb4−/− mice . Accordingly, our data also demonstrated a similar effect of Abcb4−/− on enhanced hepatic TAG levels in HBs transgenic mice (Fig. 1a–d).
FFAs have been shown to activate PPARα . The functional nuclear binding of PPARα was increased in our Abcb4−/− mice but nearly no differences were found between HBs and HBs/Abcb4−/− (Fig. 5c). PPARα itself can regulate all sequential steps of TAG catabolism including the regulation of lipases, including LPL . The current data do not provide an explanation for the discrepancy between PPARα and LPL regulation. Nevertheless, PPARα target genes, including lipases, were found to be regulated in HBs/Abcb4−/− mice (Fig. 5d, e). As the liver specific knockout of LPL has no impact on hepatic TG levels , it is questionable if the increased expression of LPL, both on transcriptional and translational level in HBs/Abcb4−/− mice in comparison to HBs and WT, might be causal for the reduction of TAGs.
In normal physiological states, FFA serve as a preferential substrate for TAG esterification and storage. Herein, higher levels of FFA, in parallel with low levels of TAGs in Abcb4−/− and HBs/Abcb4−/− indicate either a suppression of the enzyme machinery involved in TAG synthesis or an enhancement of lipolytic activity. The genes and proteins regulating the enzymes involved in TAG synthesis might also contribute to the reduced TAG levels in HBs/Abcb4−/− mice (Fig. 4a–g). TAG biosynthesis from glycerol-3-phosphate is catalyzed by a number of protein isoforms of the glycerol phosphate acyltransferase (GPAT), acylglycerolphosphate acyltransferase (AGPAT), and lipin (phosphatidate phosphatase) families, that appear to catalyze similar biochemical reactions . Notably, AGPAT1 and GPAT1 were significantly reduced in HBs/Abcb4−/− mice (Fig. 4d, e). The protein expression of DGAT1 and the transcriptional level of DGAT2 appeared remarkably decreased in HBs/Abcb4−/− (Fig. 4c, f). The reduced expression of AGPAT1, GPAT1, MGAT1, and DGAT2 suggests that FFAs could not be utilized for TAG synthesis in Abcb4−/− and HBs/Abcb4−/− mice.
Several studies indicated the beneficial effects of lipid storage and loss of TAG storage capacity being critically linked to lipotoxicity, which has been shown to exacerbate liver injury . Therefore, increased FFA levels in parallel with suppression of TAG synthesis and storage along with enhanced lipolysis pathways in HBs/Abcb4−/− mice might also contribute to the acceleration of liver injury .
The activation of AMPK inhibits hepatic fatty acid synthesis and promotes fatty acid oxidation via phosphorylation and inactivation of ACC1  and the phosphorylation of specific transcription factors such as SREBP1c by AMPK results in a reduced expression of lipogenic and gluconeogenic enzymes . Our data clearly show an increased activation of AMPK in Abcb4−/− and HBs/Abcb4−/− mice (Fig. 6a). Alongside the increased activation of AMPK, we demonstrate a decrease in genes responsible for lipogenesis, i.e. Srebp1c, Fasn, Acc1 Scd1, Hmgcs1, and Pparγ in HBs/Abcb4−/− mice (Fig. 2a–f). Also genes which are involved in the uptake and secretion of lipids such as Cd36, ApoE, and Pctp were downregulated in HBs/Abcb4−/− mice. Although Hmgcs1 expression decreased in HBs/Abcb4−/− mice compared to HBs (Fig. 2e), the hepatic cholesterol level remained constant (Fig. 1e). Nevertheless, serum cholesterol was significantly decreased in HBs/Abcb4−/− mice compared to wild-type mice (Fig. 1h). Cholesterol absorption is dependent on micellar solubilization together with BA and fatty acids . Thus, cholesterol uptake might be affected in HBs/Abcb4−/− mice (Fig. 1h) as elevated plasma bile acid levels are a characteristic hallmark in Abcb4−/− mice  as well as in HBs/Abcb4−/− mice .
Previous studies reported that the AMPK-mediated phosphorylation of the LD-associated protein PLIN2 is essential for subsequent selective degradation and triggering of lipolysis , suggesting an interplay between AMPK and PLIN2 in regulating intracellular TAG storage. PLIN2, being the major LD-associated protein, protects and stabilizes LDs, provides a “shielding effect” and modulates lipase’s accessibility to TAGs . Furthermore, the reduction of PLIN2 expression by antisense oligonucleotide treatment led to decreased hepatic lipid accumulation . However, the association of Abcb4 mediated reduction of TAGs and PLIN2 has not been reported so far. Here our study showed a reduction of PLIN2 both in vivo and in vitro (Figs. 3a–c and 7a, b) suggesting a role of cholestasis mediated regulation on PLIN2 expression.
Previous reports suggested that CREB could be induced by AMPK . These observations, along with scanning of peptide sequences for AMPK recognition motifs, led to the hypothesis that CREB may influence lipid homeostasis together with AMPK . Notably, CREB was activated in HBs/Abcb4−/− in comparison to Abcb4−/− and HBs mice (Fig. 6a, b). In addition to its role in promoting fatty acid breakdown, CREB also appears to block the expression of lipogenic pathways . Intriguingly, our study also shows a decreased expression of PPARγ in HBs/Abcb4−/− mice (Fig. 2f). Mice deficient in CREB activity have a fatty liver phenotype and display an elevated expression of the nuclear hormone receptor PPAR-γ, a key regulator of lipogenic genes . Similarly, our cell culture models of cholestasis demonstrated increased activation of AMPK and CREB along with downregulation of FASN and PLIN2 in HepG2 cells, emphasizing the possible role of bile acid in lipid metabolism during cholestatic liver injury (Fig. 7a, b). Finally, AMPK inhibition reversed this effect, which underlines a mechanistic association.
In summary, the hepatic lipid metabolism in HBs mice was altered by concomitant cholestasis induced via Abcb4 transporter knockout. AMPK and CREB signaling could mediate this process. The results of the current study may trigger the development of novel therapeutic strategies as NASH is a crucial factor able to aggravate chronic liver disease in HBV infected patients . In conclusion, a pharmacological modulation of AMPK and CREB signaling might be a promising therapeutic concept for the treatment of fatty liver diseases.
Trauner M, Fickert P, Stauber RE. Inflammation-induced cholestasis. J Gastroenterol Hepatol. 1999;14:946–59.
Reichert MC, Lammert F. ABCB4 gene aberrations in human liver disease: an evolving spectrum. Semin Liver Dis. 2018;38:299–307.
Moustafa T, Fickert P, Magnes C, Guelly C, Thueringer A, Frank S, et al. Alterations in lipid metabolism mediate inflammation, fibrosis, and proliferation in a mouse model of chronic cholestatic liver injury. Gastroenterology. 2012;142:140–51.
Ikenaga N, Liu SB, Sverdlov DY, Yoshida S, Nasser I, Ke Q, et al. A new Mdr2(−/−) mouse model of sclerosing cholangitis with rapid fibrosis progression, early-onset portal hypertension, and liver cancer. Am J Pathol. 2015;185:325–34.
Mendes LC, Stucchi RS, Vigani AG. Diagnosis and staging of fibrosis in patients with chronic hepatitis C: comparison and critical overview of current strategies. Hepat Med. 2018;10:13–22.
Choi HSJ, Brouwer WP, Zanjir WMR, Man RA, de, Feld JJ, Hansen BE, et al. Nonalcoholic steatohepatitis is associated with liver-related outcomes and all-cause mortality in chronic hepatitis B. Hepatology. 2020;71:539–48.
Chisari FV, Filippi P, Buras J, McLachlan A, Popper H, Pinkert CA, et al. Structural and pathological effects of synthesis of hepatitis B virus large envelope polypeptide in transgenic mice. Proc Natl Acad Sci USA. 1987;84:6909–13.
Chung Y-L, Wu M-L. The role of promyelocytic leukemia protein in steatosis-associated hepatic tumors related to chronic hepatitis B virus infection. Transl Oncol. 2018;11:743–54.
Chisari FV, Klopchin K, Moriyama T, Pasquinelli C, Dunsford HA, Sell S, et al. Molecular pathogenesis of hepatocellular carcinoma in hepatitis B virus transgenic mice. Cell. 1989;59:1145–56.
Churin Y, Roderfeld M, Stiefel J, Würger T, Schröder D, Matono T, et al. Pathological impact of hepatitis B virus surface proteins on the liver is associated with the host genetic background. PLoS ONE. 2014;9:e90608.
Montalbano R, Honrath B, Wissniowski TT, Elxnat M, Roth S, Ocker M, et al. Exogenous hepatitis B virus envelope proteins induce endoplasmic reticulum stress: involvement of cannabinoid axis in liver cancer cells. Oncotarget. 2016;7:20312–23.
Bondini S, Kallman J, Wheeler A, Prakash S, Gramlich T, Jondle DM, et al. Impact of non-alcoholic fatty liver disease on chronic hepatitis B. Liver Int. 2007;27:607–11.
Liang J, Liu F, Wang F, Han T, Jing L, Ma Z, et al. A noninvasive score model for prediction of NASH in patients with chronic hepatitis B and nonalcoholic fatty liver disease. Biomed Res Int. 2017;2017:8793278.
Roeb E, Geier A. Nonalcoholic steatohepatitis (NASH)—current treatment recommendations and future developments. Z Gastroenterol. 2019;57:508–17.
Alwahsh SM, Gebhardt R. Dietary fructose as a risk factor for non-alcoholic fatty liver disease (NAFLD). Arch Toxicol. 2017;91:1545–63.
Brandt A, Hernández-Arriaga A, Kehm R, Sánchez V, Jin CJ, Nier A, et al. Metformin attenuates the onset of non-alcoholic fatty liver disease and affects intestinal microbiota and barrier in small intestine. Sci Rep. 2019;9:6668.
Mahli A, Saugspier M, Koch A, Sommer J, Dietrich P, Lee S, et al. ERK activation and autophagy impairment are central mediators of irinotecan-induced steatohepatitis. Gut. 2018;67:746–56.
Towler MC, Hardie DG. AMP-activated protein kinase in metabolic control and insulin signaling. Circ Res. 2007;100:328–41.
Wang Q, Liu S, Zhai A, Zhang B, Tian G. AMPK-mediated regulation of lipid metabolism by phosphorylation. Biol Pharm Bull. 2018;41:985–93.
Herzig S, Hedrick S, Morantte I, Koo S-H, Galimi F, Montminy M. CREB controls hepatic lipid metabolism through nuclear hormone receptor PPAR-gamma. Nature. 2003;426:190–3.
Kimmel AR, Brasaemle DL, McAndrews-Hill M, Sztalryd C, Londos C. Adoption of PERILIPIN as a unifying nomenclature for the mammalian PAT-family of intracellular lipid storage droplet proteins. J Lipid Res. 2010;51:468–71.
Kaushik S, Cuervo AM. AMPK-dependent phosphorylation of lipid droplet protein PLIN2 triggers its degradation by CMA. Autophagy. 2016;12:432–8.
Zahner D, Glimm H, Matono T, Churin Y, Herebian D, Mayatepek E, et al. Hepatitis B virus surface proteins accelerate cholestatic injury and tumor progression in Abcb4-knockout mice. Oncotarget. 2017;8:52560–70.
Roderfeld M, Rath T, Lammert F, Dierkes C, Graf J, Roeb E. Innovative immunohistochemistry identifies MMP-9 expressing macrophages at the invasive front of murine HCC. World J Hepatol. 2010;2:175–9.
Roderfeld M, Rath T, Voswinckel R, Dierkes C, Dietrich H, Zahner D, et al. Bone marrow transplantation demonstrates medullar origin of CD34+ fibrocytes and ameliorates hepatic fibrosis in Abcb4-/- mice. Hepatology. 2010;51:267–76.
Roderfeld M, Padem S, Lichtenberger J, Quack T, Weiskirchen R, Longerich T, et al. Schistosoma mansoni egg-secreted antigens activate hepatocellular carcinoma-associated transcription factors c-Jun and STAT3 in hamster and human hepatocytes. Hepatology. 2018. https://doi.org/10.1002/hep.30192.
Livak KJ, Schmittgen TD. Analysis of relative gene expression data using real-time quantitative PCR and the 2(-delta delta C(T)) method. Methods. 2001;25:402–8.
Anderson AA, Altafaj X, Zheng Z, Wang Z-M, Delbono O, Ronjat M, et al. The junctional SR protein JP-45 affects the functional expression of the voltage-dependent Ca2+ channel Cav1.1. J Cell Sci. 2006;119:2145–55.
Laggai S, Simon Y, Ranssweiler T, Kiemer AK, Kessler SM. Rapid chromatographic method to decipher distinct alterations in lipid classes in NAFLD/NASH. World J Hepatol. 2013;5:558–67.
Krüger S, Bürmann L, Morlock GE. Comparison and characterization of soybean and sunflower lecithins used for chocolate production by high-performance thin-layer chromatography with fluorescence detection and electrospray mass spectrometry. J Agric Food Chem. 2015;63:2893–901.
Nassal M. The arginine-rich domain of the hepatitis B virus core protein is required for pregenome encapsidation and productive viral positive-strand DNA synthesis but not for virus assembly. J Virol. 1992;66:4107–16.
Tsai T-H, Chen E, Li L, Saha P, Lee H-J, Huang L-S, et al. The constitutive lipid droplet protein PLIN2 regulates autophagy in liver. Autophagy. 2017;13:1130–44.
Reddy JK, Hashimoto T. Peroxisomal beta-oxidation and peroxisome proliferator-activated receptor alpha: an adaptive metabolic system. Annu Rev Nutr. 2001;21:193–230.
Deng T, Shan S, Li P-P, Shen Z-F, Lu X-P, Cheng J, et al. Peroxisome proliferator-activated receptor-gamma transcriptionally up-regulates hormone-sensitive lipase via the involvement of specificity protein-1. Endocrinology. 2006;147:875–84.
Heidrich F, Schotola H, Popov AF, Sohns C, Schuenemann J, Friedrich M, et al. AMPK-activated protein kinase and its role in energy metabolism of the heart. Curr Cardiol Rev. 2010;6:337–42.
Thomson DM, Herway ST, Fillmore N, Kim H, Brown JD, Barrow JR, et al. AMP-activated protein kinase phosphorylates transcription factors of the CREB family. J Appl Physiol. 2008;104:429–38.
Shipovskaya AA, Dudanova OP. Intrahepatic cholestasis in nonalcoholic fatty liver disease. Ter Arkh. 2018;90:69–74.
Rigopoulou EI, Zachou K, Gatselis NK, Papadamou G, Koukoulis GK, Dalekos GN. Primary biliary cirrhosis in HBV and HCV patients: clinical characteristics and outcome. World J Hepatol. 2013;5:577–83.
Javaid A, Poongkunran M, Allard FD, Kyaw W, Maung HH, Lau D. Subtle presentation of active primary biliary cirrhosis in chronic hepatitis B: a case report. Gastroenterol Rep. 2017;5:157–60.
Tsochatzis E, Papatheodoridis GV, Manesis EK, Kafiri G, Tiniakos DG, Archimandritis AJ. Metabolic syndrome is associated with severe fibrosis in chronic viral hepatitis and non-alcoholic steatohepatitis. Aliment Pharmacol Ther. 2008;27:80–9.
Aguiar Vallim TQ, de, Tarling EJ, Edwards PA. Pleiotropic roles of bile acids in metabolism. Cell Metab. 2013;17:657–69.
Montagner A, Polizzi A, Fouché E, Ducheix S, Lippi Y, Lasserre F, et al. Liver PPARα is crucial for whole-body fatty acid homeostasis and is protective against NAFLD. Gut. 2016;65:1202–14.
Rakhshandehroo M, Sanderson LM, Matilainen M, Stienstra R, Carlberg C, Groot PJde, et al. Comprehensive analysis of PPARalpha-dependent regulation of hepatic lipid metabolism by expression profiling. PPAR Res. 2007;2007:26839.
Liu G, Xu J-N, Liu D, Ding Q, Liu M-N, Chen R, et al. Regulation of plasma lipid homeostasis by hepatic lipoprotein lipase in adult mice. J Lipid Res. 2016;57:1155–61.
Takeuchi K, Reue K. Biochemistry, physiology, and genetics of GPAT, AGPAT, and lipin enzymes in triglyceride synthesis. Am J Physiol Endocrinol Metab. 2009;296:1195–209.
Yamaguchi K, Yang L, McCall S, Huang J, Yu XX, Pandey SK, et al. Inhibiting triglyceride synthesis improves hepatic steatosis but exacerbates liver damage and fibrosis in obese mice with nonalcoholic steatohepatitis. Hepatology. 2007;45:1366–74.
Hardie DG. AMP-activated protein kinase as a drug target. Annu Rev Pharmacol Toxicol. 2007;47:185–210.
Cai S-Y, Mennone A, Soroka CJ, Boyer JL. Altered expression and function of canalicular transporters during early development of cholestatic liver injury in Abcb4-deficient mice. Am J Physiol Gastrointest Liver Physiol. 2014;306:670–6.
Imai Y, Boyle S, Varela GM, Caron E, Yin X, Dhir R, et al. Effects of perilipin 2 antisense oligonucleotide treatment on hepatic lipid metabolism and gene expression. Physiol Genomics. 2012;44:1125–31.
Garcia D, Shaw RJ. AMPK: mechanisms of cellular energy sensing and restoration of metabolic balance. Mol Cell. 2017;66:789–800.
We thank Heike Muller and Annette Tschuschner for excellent technical assistance. This work was supported by grants from DAAD (#91606935 to KI), von-Behring-Roentgen Foundation (#58-0005 to ER and #60-0002 to MR), and University Medical Center Giessen and Marburg (UKGM) (#21_2013 GI to ER and #7_2014 GI to MR). Open Access Funding provided by Projekt DEAL.
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Irungbam, K., Roderfeld, M., Glimm, H. et al. Cholestasis impairs hepatic lipid storage via AMPK and CREB signaling in hepatitis B virus surface protein transgenic mice. Lab Invest 100, 1411–1424 (2020). https://doi.org/10.1038/s41374-020-0457-9
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