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Article

Liraglutide Exerts Protective Effects by Downregulation of PPARγ, ACSL1 and SREBP-1c in Huh7 Cell Culture Models of Non-Alcoholic Steatosis and Drug-Induced Steatosis

by
Tea Omanovic Kolaric
1,2,
Tomislav Kizivat
3,4,
Vjera Mihaljevic
1,2,
Milorad Zjalic
5,
Ines Bilic-Curcic
2,6,
Lucija Kuna
1,
Robert Smolic
1,
Aleksandar Vcev
7,
George Y. Wu
8 and
Martina Smolic
1,2,*
1
Department of Pharmacology and Biochemistry, Faculty of Dental Medicine and Health Osijek, Crkvena 21, 31000 Osijek, Croatia
2
Department of Pharmacology, Faculty of Medicine Osijek, J. Huttlera 4, 31000 Osijek, Croatia
3
Department of Nuclear Medicine and Oncology, Faculty of Medicine Osijek, J. Huttlera 4, 31000 Osijek, Croatia
4
Clinical Institute of Nuclear Medicine and Radiation Protection, University Hospital Osijek, J. Huttlera 4, 31000 Osijek, Croatia
5
Department of Molecular Medicine and Biotechnology, Faculty of Medicine Rijeka, B. Branchetta 20, 51000 Rijeka, Croatia
6
Department of Endocrinology, University Hospital Osijek, J. Huttlera 4, 31000 Osijek, Croatia
7
Department of Pathophysiology and Physiology with Immunology, Faculty of Dental Medicine and Health Osijek, Crkvena 21, 31000 Osijek, Croatia
8
Department of Medicine, Division of Gastroenterology-Hepatology, University of Connecticut Health Center, 135 Dowling Way, Farmington, CT 06030, USA
*
Author to whom correspondence should be addressed.
Curr. Issues Mol. Biol. 2022, 44(8), 3465-3480; https://doi.org/10.3390/cimb44080239
Submission received: 28 June 2022 / Revised: 19 July 2022 / Accepted: 25 July 2022 / Published: 2 August 2022
(This article belongs to the Topic Clinical, Translational and Basic Research on Liver Diseases)
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Versions Notes

Abstract

:
(1) Background: With the aging of the population and polypharmacy encountered in the elderly, drug-induced steatosis (DIS) has become frequent cause of non-alcoholic steatosis (NAS). Indeed, NAS and DIS may co-exist, making the ability to distinguish between the entities ever more important. The aim of our study was to study cell culture models of NAS and DIS and determine the effects of liraglutide (LIRA) in those models. (2) Methods: Huh7 cells were treated with oleic acid (OA), or amiodarone (AMD) to establish models of NAS and DIS, respectively. Cells were treated with LIRA and cell viability was assessed by MTT, lipid accumulation by Oil-Red-O staining and triglyceride assay, and intracellular signals involved in hepatosteatosis were quantitated by RT-PCR. (3) Results: After exposure to various OA and AMD concentrations, those that achieved 80% of cells viabilities were used in further experiments to establish NAS and DIS models using 0.5 mM OA and 20 µM AMD, respectively. In both models, LIRA increased cell viability (p < 0.01). Lipid accumulation was increased in both models, with microsteatotic pattern in DIS, and macrosteatotic pattern in NAS which corresponds to greater triglyceride accumulation in latter. LIRA ameliorated these changes (p < 0.001), and downregulated expression of lipogenic ACSL1, PPARγ, and SREBP-1c pathways in the liver (p < 0.01) (4) Conclusions: LIRA ameliorates hepatocyte steatosis in Huh7 cell culture models of NAS and DIS.

1. Introduction

Drug-induced liver injury (DILI) is an emerging public health problem with continuously increasing incidence and progression to more severe stages of liver disease. Pathophysiological mechanisms have still not been fully elucidated. The Roussel Uclaf Causality Assessment Method (RUCAM) and liver biopsy may help clinicians better diagnose and differentiate DILI in clinical practice [1]. The majority of countries and regions around the world have also compiled lists of empirical DILI treatment strategies and established guidelines. DILI is currently classified into three clinical patterns based on the serum alanine transaminase (ALT) and alkaline phosphatase (ALP) ratio from the first available biochemical test: hepatocellular, cholestatic, or mixed injury (liver-damaged target cells) [2]. In addition, DILI can also manifest as acute hepatic necrosis, chronic hepatitis, fatty liver, bland cholestasis, sinusoidal obstruction syndrome, and acute liver failure [3,4]. One specific form of DILI is a DIS, which occurs in up to 27% of DILI cases [5]. DIS can present in several histopathological forms, such as macro and microvesicular steatosis, and steatohepatitis which can then progress to liver fibrosis and eventually liver cirrhosis. It is not uncommon for DIS to be associated with non-alcoholic fatty liver disease (NAFLD). NAFLD is usually associated with the development of insulin resistance and occurs as a feature of another major global health problem, the metabolic syndrome. Nevertheless, a small proportion of NAFLD cases are due to drug toxicity, or to drugs that may exacerbate pre-existing fatty liver injury [6]. Some of the drugs capable of causing DIS are glucocorticoids, AMD, methotrexate, estrogens, tamoxifen, nonsteroidal anti-inflammatory drugs (NSAIDs), acetaminophen, 5-fluorouracil, metoprolol, valproic acid, tetracycline, aspirin, ibuprofen, zidovudine, glucocorticoids, perhexiline, and propranolol.
AMD is a class II antiarrhythmic drug used to treat severe ventricular arrhythmias. It can cause numerous side effects including significant hepatotoxicity [7]. Several mechanisms responsible for this effect have been proposed including stimulation of lipogenesis by affecting the expression of genes involved in lipogenesis (peroxisome proliferator-activated receptor γ-PPARγ, sterol regulatory element-binding protein 1c–SREBP-1c, PPARα), disruption of mitochondrial function followed by a decrease in β-oxidation of free fatty acids (FFAs), increased accumulation of reactive oxygen species (ROS) (affecting the expression of CPT1), and decreased glutathione (GSH) levels [7,8,9,10,11,12]. Although discontinuation of the potentially toxic drug is generally recommended, in some cases withdrawal may also have negative effects on patient health, considering the severity of the heart disease. Therefore, a better understanding of the development of DIS is necessary to identify appropriate diagnostics and therapeutics.
To date, various agents such as antioxidants vitamin E and C, and L-carnitine have been studied as potential therapeutic options [1,7]. Numerous studies have demonstrated the beneficial role of glucagon-like peptide-1 receptor agonists (GLP-1RA) in the treatment of NAFLD [13,14,15,16,17,18,19,20]. These drugs have a broad spectrum of effects on the liver, in addition to numerous effects on other organs. GLP-1 RA (semaglutide, exenatide, liraglutide) improve hepatic insulin sensitivity, decrease inflammation and fibrosis, and reduce hepatic de novo lipogenesis and fat deposition [21]. Semaglutide and exenatide, two of the agonists, have a stronger effect on lowering ALT levels, inflammation, and weight, while liraglutide (LIRA) has a stronger effect on reducing mild steatosis and hepatocyte ballooning [15,19,22]. Interestingly, the effects of LIRA on liver fibrosis are not so clear. Authors in the LEAN study listed the short duration of the treatment as a possible cause of the lack of improvement in fibrosis stage in LIRA treated group of patients [23]. Nevertheless, other effects, such as decreasing lipid over-accumulation by upregulating autophagy, adjusting lipid metabolism by SHP1/AMPK/SREBP1 signaling pathway, decreasing apoptosis, oxidative stress of liver cells, proliferation and activation of hepatic stellate cells through RAGE/NOX2, reducing lipotoxicity-induced oxidative stress possibly by modulation of NRF2, decreasing expression of main elements involved in lipogenesis (phospho-ACC), peroxisomal β-oxidation (ACOX1), and lipid flux/storage (PPARγ), make LIRA a promising GLP-1R agonist for treatment and/or prevention of NAS [13,16,17,24,25,26]. Considering the role of the PPARγ and SREBP-1c signaling pathway in NAS and DIS development, and LIRA hepatoprotective action, analysis of these and other signaling pathways related to it (such as Acyl-CoA Synthetase Long Chain Family Member 1, ACSL1, which channels fatty acids from fatty acid oxidation to lipid synthesis), could help better understand their effects on hepatocytes [13,26,27]. Yasmin et al. showed that apart from PPARγ involvement in fatty liver changes in rats, upregulation of C/EBPα (CCAAT Enhancer Binding Protein α) is also responsible for steatosis progression [28].
The Huh7 cell line was selected for developing NAS and DIS cell culture models because of its availability, easy handling, unlimited propagation potential, and stable phenotype [29]. Its limitations include a lack of substantial hepatocyte function with regard to the biotransformation capacity [29]. However, Gupta et al. showed that both Huh7 and HepG2 cell lines are suitable for the development of in vitro models of fatty liver, and that GLP-1R is present in both cell lines [30].
Further studies are needed to better understand underlying mechanisms for fatty liver development, and for the introduction of LIRA or other agents into daily practice. Therefore, the aim of the current study was to use an Huh7 cell culture model of DIS and to investigate whether LIRA could also play a protective role in the DIS model as has been shown for NAS in previous studies [30,31,32,33,34].

2. Materials and Methods

2.1. Chemicals

AMD, sodium oleate, and Oil-Red-O were purchased from Sigma-Aldrich (St. Louis, MO, USA), and LIRA was purchased from Novo Nordisk (Bagsvaerd, Denmark).

2.2. Cell Culture

Huh7 cell line was a generous gift from Prof. George Y. Wu, University of Connecticut Health Center in Farmington, NM, USA. Huh7 cells are a human hepatocyte cell line established from a well-differentiated liver cancer. Cells were sub-cultivated in 10 cm dishes in Dulbecco’s modified Eagle’s medium (DMEM) supplemented with 10% fetal bovine serum (FBS/Thermo Fisher Scientific Cat. No. 16000036) and 1% penicillin/streptomycin solution (Thermo Fisher Scientific Inc., Waltham, MA, USA) at 37 °C in a humidified atmosphere of 5% CO2 v/v in air. Cells were passaged every 3–4 days until 75% confluence was reached.

2.3. NAS and DIS Cell Culture Models

To establish NAS and DIS models, cells were cultured as mentioned above and grown overnight in a 96-well plate to reach 90% confluence. Afterward, cells were maintained in DMEM without FBS, and exposed to increasing concentrations of oleic acid (0.5 mM and 1 mM) or AMD (5, 10, 20, 40, 80 µM) for 24 h up to 72 h. Experiments were performed in triplicates [9,35,36]. Two controls were used: a negative control (cells incubated only in DMEM without FBS) and a positive control (cells incubated in OA, as NAS model). The effect of drugs on cell viability was determined by an MTT colorimetric assay (Cruz chemicals, Dallas, TX, USA) on a microplate reader (iMarkTM microplate absorbance reader; Bio-Rad, Hercules, CA, USA), according to the manufacturer’s protocol and as described previously [37]. For further experiments, optimal concentrations of AMD (20 µM) and OA (0.5 mM) and a time period of 24 h, were selected because these concentrations reduced cell viability to 80% compared to the negative control, and induced steatosis for NAS and DIS models. These results were also confirmed by the Erythrosin B color exclusion test and cell counting with a Neubauer hemocytometer (data not shown).

2.4. Measurement of the Hepatoprotective Effect of LIRA in NAS and DIS Cell Culture Models

LIRA was prepared in three different final concentrations (5 nM, 10 nM, 20 nM). LIRA was then added as a co-treatment to the above-mentioned NAS and DIS models. In short, first, the cells were grown overnight in 96 well and 6- well plates to reach 90% confluence. The cell subgroups for the determination of the hepatoprotective effect of LIRA were designed as follows: Huh7 cells grown in DMEM as a negative control; Huh7 cells treated with increasing concentrations of LIRA (5, 10, and 20 nM); cells treated with OA as a positive control; Huh7 cells treated with OA and increasing concentrations of LIRA; Huh7 cells treated with AMD; Huh7 cells treated with AMD and increasing concentrations of LIRA. On the second day of the experiment, determinations of cell survival and viability were performed by MTT colorimetric assay and Erythrosin B color exclusion test as previously described. Results are shown as a percentage relative to the negative control of at least three biological replicates.

2.5. Visualization of Fat Accumulation

According to the above-described protocol, cells were incubated and treated for 24 h in 24-well plates with cover slides previously prepared following the protocol by Zjalic et al. [38] and coated with poly-D-Lysine (Sigma Aldrich, St. Louis, MO, USA). At the end of the experiment, cells were fixed with formaldehyde for 30 min at +4 °C. Afterwards, cells were washed 2x with PBS. Neutral lipids were stained using Oil-Red-O dye (ChemCruz, Huissen, The Netherlands). Fixed cells were stained with a working Oil-Red-O solution for 30 min. Oil-Red-O 0.5% stock solution was dissolved in isopropanol, and the working solution was prepared as 60% Oil-Red-O stock solution with 40% water. Fixed cells were stained with a working Oil-Red-O solution for 30 min. After rinsing two times with phosphate buffered saline (PBS), cells were mounted in the fluorescent mounting medium with 4′,6′-diamidino-2-phenylindole (DAPI) (Abcam, Cambridge, UK). The cells were visualized using a microscope (Axioskop 2 MOT Inverted microscope, Carl Zeiss, Göttingen Germany) with an Olympus D70 camera, controlled through the computer program DP Manager 1.2.1.107 and DP Controller 1.2.1.108. ImageJ-Fiji software was used to count cell nuclei and measure integrated density relative to the cell count. Results are shown as a percentage relative to the negative control of at least three biological replicates.

2.6. Measurement of Triglyceride Levels

After treatment according to the above-described protocol, the accumulation of triglycerides in 12 subgroups of cells was measured by triglyceride GPO—PAP method (glycerol 3 phosphate oxidase—4-Amino-antipyrine, Greiner Diagnostic, Bahlingen, Germany). Triglyceride standards were used in order to quantify absolute concentration of triglycerides. Results were expressed as absolute values in mg/dl.

2.7. Total RNA Isolation and Reverse Transcription Polymerase Chain Reaction (RT-PCR) Analysis

To evaluate the expression of various genes (ACSL1, C/EBPα, PPARγ, SREBP-1c), total RNA from cells was isolated on the third day of experiment using TRI Reagent (T9424, Sigma Aldrich, St. Louis, MS, USA) according to the manufacturer’s protocol. cDNA strand was synthesized using a commercially available kit (High-Capacity cDNA Reverse Transcription Kit, Applied Biosystems, Thermo Fisher Scientific Inc., Waltham, MA, USA) according to the manufacturer’s instructions. A commercially available kit (Taq PCR Core Kit, Qiagen, Hilden, Germany) was used to amplify the obtained cDNA using a DNA Engine® Thermal Cycler (Bio-Rad, Hercules, CA, USA, SAD). PCR conditions are listed in Table 1. The synthesized cDNA was amplified using specific primer sequences as shown in Table 2. As an internal control to determine the possible presence of different cDNA concentrations β-actin was used. PCR results were visualized on a 1.6% agarose gel stained with Diamond™ Nucleic Acid Dye (Promega, Madison, WI, USA) according to the manufacturer’s instructions, visualized by Gel Imaging System (ChemiDocTM Imaging System, Bio-Rad, Hercules, CA, USA). The images were semi-quantified by an Image Lab 6.0.1 build 34 Bio-Rad Laboratories (normalized to the housekeeping gene β-actin mRNA levels) [39]. Results are shown as a percentage relative to the negative control of at least three biological replicates.

2.8. Statistical Analyses

To determine statistical significance, data were analyzed with One-way and Two-way ANOVA. Normality of data distribution was tested with Shapiro–Wilk test. Homoscedasticity of groups was tested with Bartlett’s F test. In both tests, the calculated p value was higher than 0.05 indicating normality of data distribution and homoscedasticity between groups, a prerequisite for ANOVA.
The main limitation of our study is the simplicity of NAS and DIS models established in Huh7 cell line. An advantage of these in vitro models is the opportunity to assess direct effect of LIRA on hepatocytes.

3. Results

3.1. Establishment of the Cell Culture Model of DIS and NAS, and Assessment of the Effect of Amiodarone and Oleic Acid on Cell Viability

The toxicity of AMD and OA in Huh7 cells was assessed by MTT assay after treatment with five different AMD concentrations (5, 10, 20, 40, and 80 µM), and two different concentrations of OA (0.5 and 1 mM) at various time points: 24 h, 48 h, 72 h. Each experiment was repeated at least three times to ensure consistency of the results. After 24 h exposure to 0.5 mM OA, cells had 80% viability, the same as exposure to 20 µM AMD at the same time point. Cell viability significantly decreased to 30% in cells treated with 40 µM AMD at 24 h. The viabilities of AMD-treated cells were significantly different compared to negative DMEM control as shown in Figure 1. Exposure of cells for longer time periods (48 h, 72 h) led to a significant drop in cell viability even with lower concentrations of AMD as shown in Figure 1 (p < 0.001). From the MTT results, the concentrations of 0.5 mM OA, and 20 µM AMD and a duration of exposure of 24 h were selected as the Huh7 models of NAS and DIS, respectively, in all subsequent experiments.

3.2. Assessment of the Protective Effect of LIRA (LIRA) on Cell Viability in DIS and NAS Cell Culture Models

Three different concentrations of LIRA (LIRA) (5, 10, and 20 nM) were used to assess its hepatoprotective effect in NAS and DIS cell culture models as shown in Figure 2. Cell viability was determined, and compared to the negative control, and to cells treated with OA and AMD. In the NAS model (cells treated with OA), 5 nM LIRA significantly increased cell viability (p < 0.01). On the other hand, higher LIRA concentrations had the opposite effect. All three concentrations of LIRA had a beneficial effect on cell viability in the DIS model, but without statistical significance.

3.3. Quantification and Visualization of Lipid Accumulation in DIS and NAS Cell Culture Models, Incubated with Varying Concentrations of LIRA

Incubation of Huh7 cells with OA and AMD induced a statistically significant increase in lipid accumulation as shown in Figure 3 (p < 0.05, p < 0.01). AMD induced microsteatosis with nuclei positioned in the center of the cells, while lipid droplets in OA were larger indicating macrosteatosis occurrence. Cotreatment with LIRA reduced the lipid accumulation in both NAS and DIS models, but only the DIS model results were statistically significant (p < 0.01, p < 0.05).

3.4. Assessment of the Effect of LIRA on Triglyceride Accumulation in NAS and DIS Cell Culture Models

AMD and OA increased significantly triglyceride content in Huh7 cells (p < 0.001). LIRA reduced the triglyceride accumulation in NAS model significantly, while in the DIS model, it resulted in no significant change in triglyceride accumulation, as shown in Figure 4.

3.5. Assessment of the Effect of LIRA on Gene Expression in NAS and DIS Cell Culture Models

To determine the effect of LIRA in NAS and DIS models on the mRNA levels of ACSL1, C/EBPα, PPARγ, and SREBP-1c RT-PCT was performed. The mRNA levels in the gels were representative results of at least three biological replicates, and the values reported as percentages relative to the negative control. Gene expression was quantified by Image Lab 6.0.1 build 34 Bio-Rad Laboratories, and normalized to the housekeeping gene β-actin mRNA levels. Because the densities of blot images are frequently non-uniform, visual impressions are not as accurate as the data from the image analyzer. Both OA and AMD upregulated ACSL1 gene expression (p < 0.05), while LIRA in cotreatment decreased ACSL1 levels, but only the OA NAS model results were statistically significant (*** p < 0.001), as shown in Figure 5A. C/EBPα was downregulated with lowest LIRA treatment in NAS model, while in the DIS model higher LIRA concentrations achieved downregulation, all without statistical significance, as shown in Figure 5B. The effect of LIRA on PPARγ gene expression is shown in Figure 5C. OA increased the mRNA levels of PPARγ, while 5 nM and 20 nM LIRA reversed this effect (p < 0.05). In the AMD DIS model, PPARγ gene expression was upregulated and 10 nM LIRA reversed this effect, but without statistical significance. In both models, a slight increase in SREBP-1c expression was observed, whereas 5 nM LIRA significantly downregulated its expression in NAS model (p < 0.05), and 10 nM LIRA in DIS model (p < 0.01), as shown in Figure 5D.

4. Discussion

So far, various in vitro models for NAS have been established, mostly with palmitic acid, and/or OA added to different cell cultures. In our study, we used OA and a Huh7 cell line. Although Ricchi et al. demonstrated that OA had no effect on cell viability, our research showed a significant decrease in cell viability (20%) after treatment of Huh7 cells with 0.5 mM OA for 24 h and 48 h [35]. This effect was no longer present after 72 h of treatment. A possible explanation could be that cells had time to recover, and OA was added only at the beginning of this experiment.
After an extensive literature search, AMD was selected as a key compound for the induction of DIS. It has been shown to have a hepatosteatotic effect and is frequently used in clinical practice. Unlike some other drugs that induce hepatosteatosis, amiodarone has not been shown to have an extrahepatic effect that could significantly contribute to its hepatosteatotic activity. Therefore, AMD exerts hepatosteatotic effect by direct effect on hepatic cells, making it suitable for cell culture study [42]. After treating cells with various AMD concentrations at different time periods, a concentration of 20 µM and an incubation time of 24 h were selected because of the significant effects on cell viability, without causing apoptosis to a greater extent (that occurs with higher amiodarone concentrations, and longer incubation times). The same treatment conditions have already been used in previous studies (9). Comparing the NAS and DIS models, the effects on cell viability were similar, but OA induced triglyceride accumulation to a greater extent compared to AMD, while AMD had a greater effect on lipid accumulation/cell in general, as shown with Oil-Red-O staining. Zhou et al. showed a significant, three-fold, increase in the lipid droplet number per cell in HepG2 cells treated with AMD for 24 h [42,43]. In the current study, an even greater-, tenfold, increase in the integrated density of quantified Oil-Red-O staining relative to cell number was observed compared to the negative control. Vitins et al. demonstrated the triglyceride accumulation as one of the main characteristics in AMD DIS, but only with longer incubation periods. However, after 24 h treatment, only a slight increase was observed [8]. In our current study, triglycerides were increased three-fold. However, considering the much greater increase in lipid accumulation as shown by Oil-Red-O staining, it is possible that accumulation of other lipids in the liver due to AMD occurred as well. Accordingly, in one in vivo study, accumulation of phosphatidylcholine occurred after AMD treatment [8,44]. On the contrary, triglyceride accumulation was significantly increased in OA NAS model as has been reported in previous studies [35].
The histological pattern also differed between these two models. Amiodarone DIS caused a microsteatosis which is consistent with the findings of previous studies [6,9,10,35], while NAS resulted in larger vesicles (macrosteatosis). NAS is usually associated with macrovesicular steatosis, although Tandra et al. demonstrated that microvesicular steatosis can also be present in approximately 10% of biopsies from patients with NAS [45,46]. Both models, NAS and DIS, showed an increase in ACSL1 (protein that converts free long-chain fatty acids into fatty acyl-CoA esters) gene expression. This increase has been demonstrated in several previous studies of NAS models, but from our literature search, this is the first report of an AMD-induced increase in ACSL1 [27]. Accordingly, the increased triglyceride accumulation detected in our models is, at least partly, due to the upregulation of ACSL1 which has been reported to be involved in both the reduction of fatty acid β-oxidation and the induction of lipogenesis in the liver [47,48]. Li at al. demonstrated that this effect was achieved through the PPARγ signaling pathway [47]. Both models, NAS and DIS, also showed significant upregulation of PPARγ expression. Previous studies have also demonstrated an increase in liver PPARγ expression in NAS model [13,49,50]. This may indicate a possible steatogenic role of PPARγ in the liver in triglyceride accumulation and lipid droplet formation in both models of fatty liver [51,52]. A slight increase in C/EBPα and SREBP-1c gene expression was observed in the NAS and DIS models, confirming their role in enhancing fatty changes [27,53].
LIRA concentrations were selected after evaluating other studies, which reported that the maximum clinical dose administered to patients was 3 mg of liraglutide daily. Extension of this figure to a person of 85 kg of weight resulted in a dose of 11.3 nmol/kg. We used 5 nmol/L, 10 nmol/L and 20 nmol/L of LIRA. Accordingly, we chose a mass to volume ratio of water of around 1. It is possible that the selected doses of LIRA used in the current study might have had a hypoglycemic effect when applied to cells. However, LIRA increases insulin secretion, while inhibiting glucagon, only in response to increases in glucose levels [54]. Therefore, the risk of hypoglycemia should be negligible.
In the current model, concentrations higher than 20 nM significantly reduced cell viability (although some studies used even 100 nM and 500 nM), so we decided to use 5, 10, and 20 nM LIRA for the experiments [16,17]. Although the lowest LIRA concentration used in our study, 5 nM, had a slightly positive effect on cell viability, higher concentrations decreased cell viability. However, these concentrations were 2-fold higher than those used in clinical practice. Consistent with other studies, LIRA generally reduced lipid accumulation in NAS model, and exerted an even stronger effect in DIS model [24,55]. The authors found no similar study demonstrating antisteatotic effect of LIRA in DIS model. However, in the current NAS model, LIRA also reduced lipid droplet size, suggesting an inverse effect on macrosteatosis which was supported by a significant decrease in triglyceride content (triglycerides are thought to be the main contributor to lipid droplet enlargement) [56,57]. When applied to the cells treated only with low-glucose DMEM medium, LIRA downregulated ACSL1 gene expression in 5 nM, but increased it in 10 nM and 20 nM groups. These results were unexpected, but reproducible, and we have no data to explain them. It is possible that high-affinity binding to ACSL1 transcription factors or their regulators may have decreased ACSL1 activity while low-affinity binding had the opposite effect. Further research is necessary in order to better understand underlying mechanisms. With the exception of 5 nM LIRA in the DIS model, all other concentrations of LIRA resulted in the downregulation of ACSL1 in both models, suggesting that LIRA achieved its antisteatotic effects in part by affecting the ACSL1 signaling pathway and reducing triglyceride synthesis. Flock et al. demonstrated a similar effect for another drug that enhances the GLP-1R effects, vildagliptin [58].
LIRA upregulated PPARγ in cells incubated only in a low-glucose medium, similar to previous in vivo studies, suggesting that it is responsible for balancing the lipid metabolism in hepatocytes [13]. Decara et al. demonstrated that in lean rats, LIRA upregulated genes involved in lipogenesis including PPARγ, whereas in high-fat-diet-induced obesity rats, the decrease in lipid accumulation by LIRA occurred due to a decreased expression of PPARγ in liver [13]. Accordingly, when added to NAS and DIS models in our study, LIRA mainly reduced PPARγ expression. It is also interesting to note that this effect was not dose-dependent, and some concentrations of LIRA even had the opposite effect. This result could be explained by the diverse role of PPARγ in the liver. Various studies demonstrated an antifibrotic role of PPARγ activation in the liver [59,60,61]. Ni et al. and Liu et al. showed that PPARγ is necessary for the inactivation of human hepatic stellate cells (HSCs), and regression of liver fibrosis in mice [59,60]. Additionally, PPARγ inhibits HSCs proliferation, and decreases extracellular-matrix production by inhibition of the activation of the TGF-β1/Smad signaling pathway [51,59,62]. Finally, PPARγ agonism enhanced sensitivity of adipose tissue, muscle, and liver to insulin, and this effect probably overcame negative effects of PPARγ on fat accumulation in hepatocytes, and resulted in a decrease in fat. Decara et al. showed that LIRA slightly upregulated PPARy in adipose tissue of HFD-induced obesity rats [13,26].
The effect of LIRA on C/EBPα gene expression was variable in our study, and without statistical significance. LIRA cotreatment had a different effect in NAS and DIS models, with a greater reduction in C/EBPα mRNA levels in the DIS model. Guzman et al. demonstrated that C/EBPα represses liver fatty acid binding protein (FABP1) responsible for the prevention of lipotoxicity of FFAs ad regulation of FFA trafficking and partition [53]. C/EBPα was induced or did not change in human NAS or animal models of NAS [53]. However, various studies showed also an antifibrotic role of C/EBPα in the liver achieved by induction of HSCs apoptosis [63,64,65,66]. To date, authors have not studied LIRA effects on C/EBPα expression in the liver, although various studies confirmed its downregulating effect in adipose tissue during longer treatment periods [67,68]. More studies are necessary in order to evaluate the role of C/EBPα in liver.
SREBP-1c gene expression was significantly downregulated with LIRA cotreatment in both models in the current study which confirms the role of SREBP-1c gene pathway in LIRA antisteatotic effect. That is consistent with the findings of Wang et al. who demonstrated the effect of LIRA in decreasing lipid content in liver by the AMPK/SREBP1 pathway [24]. AMPK regulates the long-term adaptation of lipid metabolism in liver by downregulation of SREBP-1c. Therefore, upregulation of SREBP-1c leads to disturbance in lipid metabolism and accumulation of fat in liver [24]. In the current study, gene expression could have been confirmed by protein analyses, in situ hybridization, and confocal microscopy studies, but the issues to be addressed by those methods are beyond the scope of this report.

5. Conclusions

In conclusion, LIRA has been shown to have hepatoprotective and antisteatotic effects in NAS and DIS cell culture models established by incubating the Huh7 cell line with OA and AMD, respectively. This effect was achieved by downregulation of gene expression of several elements involved in lipid accumulation (ACSL1, C/EBPα, PPARγ, SREBP-1c). However, the role of some of these gene pathways in the liver has not been fully elucidated. Overall, our studies suggest that LIRA may play an important role in the treatment of not only NAS, but also DIS. However, further studies are needed to clarify the exact role of the various gene pathways in the development of fatty liver, not only in hepatocytes, but also in other liver cells in order to confirm the hepatoprotective role of LIRA in various fatty liver models.

Author Contributions

Conceptualization, M.S.; methodology, M.S. and T.K.; data curation, T.O.K., M.Z. and T.K.; investigation, T.O.K., writing—original draft preparation, T.O.K.; writing—review and editing, M.S., G.Y.W. and I.B.-C.; visualization, T.O.K. and V.M.; supervision, M.S.; project administration, T.O.K., L.K. and V.M.; funding acquisition, A.V., R.S. and M.S. All authors have read and agreed to the published version of the manuscript.

Funding

The study was funded by grants from Croatian Ministry of Science, Education and Sports dedicated to multi-year institutional funding of scientific activity at the Josip Juraj Strossmayer University of Osijek, Osijek, Croatia—grant’s numbers: IP10-Mefos-2019 (to Martina Smolic), IP15-Mefos-2021 (to Martina Smolic), and IP8-FDMZ-2021 (to Robert Smolic).

Institutional Review Board Statement

Not applicable.

Informed Consent Statement

Not applicable.

Data Availability Statement

The data presented in this study are available on request from the corresponding authors.

Conflicts of Interest

The authors declare no conflict of interest.

References

  1. Li, M.; Luo, Q.; Tao, Y.; Sun, X.; Liu, C. Pharmacotherapies for Drug-Induced Liver Injury: A Current Literature Review. Front. Pharmacol. 2021, 12, 806249. [Google Scholar] [CrossRef] [PubMed]
  2. Chalasani, N.P.; Maddur, H.; Russo, M.W.; Wong, R.J.; Reddy, K.R.; Gastroenterology PPCotACo. ACG Clinical Guideline: Diagnosis and Management of Idiosyncratic Drug-Induced Liver Injury. Am. J. Gastroenterol. 2021, 116, 878–898. [Google Scholar] [CrossRef] [PubMed]
  3. Benić, M.S.; Nežić, L.; Vujić-Aleksić, V.; Mititelu-Tartau, L. Novel Therapies for the Treatment of Drug-Induced Liver Injury: A Systematic Review. Front. Pharmacol. 2021, 12, 785790. [Google Scholar] [CrossRef] [PubMed]
  4. Hoofnagle, J.H.; Björnsson, E.S. Drug-Induced Liver Injury—Types and Phenotypes. N. Engl. J. Med. 2019, 381, 264–273. [Google Scholar] [CrossRef] [PubMed]
  5. Kleiner, D.E.; Chalasani, N.P.; Lee, W.M.; Fontana, R.J.; Bonkovsky, H.L.; Watkins, P.B.; Hayashi, P.H.; Davern, T.J.; Navarro, V.; Reddy, R.; et al. Hepatic histological findings in suspected drug-induced liver injury: Systematic evaluation and clinical associations. Hepatology 2014, 59, 661–670. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  6. Miele, L.; Liguori, A.; Marrone, G.; Biolato, M.; Araneo, C.; Vaccaro, F.G.; Gasbarrini, A.; Grieco, A. Fatty liver and drugs: The two sides of the same coin. Eur. Rev. Med. Pharmacol. Sci. 2017, 21 (Suppl. S1), 86–94. [Google Scholar]
  7. Akbay, E.; Erdem, B.; Ünlü, A.; Durukan, A.B.; Onur, M.A. Effects of N-acetyl cysteine, vitamin E and vitamin C on liver glutathione levels following amiodarone treatment in rats. Kardiochir. Torakochirurgia. Pol. 2019, 16, 88–92. [Google Scholar] [CrossRef] [PubMed]
  8. Vitins, A.P.; Kienhuis, A.S.; Speksnijder, E.N.; Roodbergen, M.; Luijten, M.; van der Ven, L.T. Mechanisms of amiodarone and valproic acid induced liver steatosis in mouse In Vivo act as a template for other hepatotoxicity models. Arch. Toxicol. 2014, 88, 1573–1588. [Google Scholar] [CrossRef]
  9. Anthérieu, S.; Rogue, A.; Fromenty, B.; Guillouzo, A.; Robin, M.A. Induction of vesicular steatosis by amiodarone and tetracycline is associated with up-regulation of lipogenic genes in HepaRG cells. Hepatology 2011, 53, 1895–1905. [Google Scholar] [CrossRef]
  10. Rabinowich, L.; Shibolet, O. Drug Induced Steatohepatitis: An Uncommon Culprit of a Common Disease. Biomed Res. Int. 2015, 2015, 168905. [Google Scholar] [CrossRef] [Green Version]
  11. Massart, J.; Begriche, K.; Buron, N.; Porceddu, M.; Borgne-Sanchez, A.; Fromenty, B. Drug-Induced Inhibition of Mitochondrial Fatty Acid Oxidation and Steatosis. Curr. Pathobiol. Rep. 2013, 1, 147–157. [Google Scholar] [CrossRef] [Green Version]
  12. Kim, G.; Choi, H.K.; Lee, H.; Moon, K.S.; Oh, J.H.; Lee, J.; Shin, J.G.; Kim, D.H. Increased hepatic acylcarnitines after oral administration of amiodarone in rats. J. Appl. Toxicol. 2020, 40, 1004–1013. [Google Scholar] [CrossRef] [PubMed]
  13. Decara, J.; Arrabal, S.; Beiroa, D.; Rivera, P.; Vargas, A.; Serrano, A.; Pavón, F.J.; Ballesteros, J.; Dieguez, C.; Nogueiras, R.; et al. Antiobesity efficacy of GLP-1 receptor agonist liraglutide is associated with peripheral tissue-specific modulation of lipid metabolic regulators. Biofactors 2016, 42, 600–611. [Google Scholar] [CrossRef] [PubMed]
  14. Attia, S.L.; Softic, S.; Mouzaki, M. Evolving Role for Pharmacotherapy in NAFLD/NASH. Clin. Transl. Sci. 2021, 14, 11–19. [Google Scholar] [CrossRef] [PubMed]
  15. Mahjoubin-Tehran, M.; De Vincentis, A.; Mikhailidis, D.P.; Atkin, S.L.; Mantzoros, C.S.; Jamialahmadi, T.; Sahebkar, A. Non-alcoholic fatty liver disease and steatohepatitis: State of the art on effective therapeutics based on the gold standard method for diagnosis. Mol. Metab. 2021, 50, 101049. [Google Scholar] [CrossRef] [PubMed]
  16. He, Y.; Ao, N.; Yang, J.; Wang, X.; Jin, S.; Du, J. The preventive effect of liraglutide on the lipotoxic liver injury via increasing autophagy. Ann. Hepatol. 2020, 19, 44–52. [Google Scholar] [CrossRef]
  17. Yu, P.; Xu, X.; Zhang, J.; Xia, X.; Xu, F.; Weng, J.; Lai, X.; Shen, Y. Liraglutide Attenuates Nonalcoholic Fatty Liver Disease through Adjusting Lipid Metabolism via SHP1/AMPK Signaling Pathway. Int. J. Endocrinol. 2019, 2019, 1567095. [Google Scholar] [CrossRef]
  18. Ji, J.; Feng, M.; Huang, Y.; Niu, X. Liraglutide inhibits receptor for advanced glycation end products (RAGE)/reduced form of nicotinamide-adenine dinucleotide phosphate (NAPDH) signaling to ameliorate non-alcoholic fatty liver disease (NAFLD) In Vivo and Vitro. Bioengineered 2022, 13, 5091–5102. [Google Scholar] [CrossRef]
  19. Ghazanfar, H.; Kandhi, S.D.; Nawaz, I.; Javed, N.; Abraham, M.C.; Farag, M.; Mahasamudram, J.; Patel, V.B.; Altaf, F.; Patel, H. Role of Glucagon-Like Peptide-1 Receptor Agonists in the Management of Non-Alcoholic Steatohepatitis: A Clinical Review Article. Cureus 2021, 13, e15141. [Google Scholar] [CrossRef]
  20. Armstrong, M.J.; Hull, D.; Guo, K.; Barton, D.; Hazlehurst, J.M.; Gathercole, L.L.; Nasiri, M.; Yu, J.; Gough, S.C.; Newsome, P.N. Glucagon-like peptide 1 decreases lipotoxicity in non-alcoholic steatohepatitis. J. Hepatol. 2016, 64, 399–408. [Google Scholar] [CrossRef] [Green Version]
  21. Gastaldelli, A.; Cusi, K. From NASH to diabetes and from diabetes to NASH: Mechanisms and treatment options. JHEP Rep. 2019, 1, 312–328. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  22. Daniels, S.J.; Leeming, D.J.; Detlefsen, S.; Bruun, M.F.; Hjuler, S.T.; Henriksen, K.; Hein, P.; Karsdal, M.A.; Brockbank, S.; Cruwys, S. Biochemical and histological characterisation of an experimental rodent model of non-alcoholic steatohepatitis—Effects of a peroxisome proliferator-activated receptor gamma (PPAR-γ) agonist and a glucagon-like peptide-1 analogue. Biomed. Pharmacother. 2019, 111, 926–933. [Google Scholar] [CrossRef] [PubMed]
  23. Armstrong, M.J.; Gaunt, P.; Aithal, G.P.; Barton, D.; Hull, D.; Parker, R.; Hazelhurst, J.M.; Guo, K.; Abouda, G.; Aldersley, M.A.; et al. Liraglutide safety and efficacy in patients with non-alcoholic steatohepatitis (LEAN): A multicentre, double-blind, randomised, placebo-controlled phase 2 study. Lancet 2016, 387, 679–690. [Google Scholar] [CrossRef] [Green Version]
  24. Wang, Y.G.; Yang, T.L. Liraglutide reduces fatty degeneration in hepatic cells via the AMPK/SREBP1 pathway. Exp. Ther. Med. 2015, 10, 1777–1783. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  25. Zhu, C.G.; Luo, Y.; Wang, H.; Li, J.Y.; Yang, J.; Liu, Y.X.; Qu, H.Q.; Wang, B.L.; Zhu, M. Liraglutide Ameliorates Lipotoxicity-Induced Oxidative Stress by Activating the NRF2 Pathway in HepG2 Cells. Horm. Metab. Res. 2020, 52, 532–539. [Google Scholar] [CrossRef] [PubMed]
  26. Kim, K.S.; Lee, B.W. Beneficial effect of anti-diabetic drugs for nonalcoholic fatty liver disease. Clin. Mol. Hepatol. 2020, 26, 430–443. [Google Scholar] [CrossRef] [PubMed]
  27. Kawano, Y.; Cohen, D.E. Mechanisms of hepatic triglyceride accumulation in non-alcoholic fatty liver disease. J. Gastroenterol. 2013, 48, 434–441. [Google Scholar] [CrossRef] [Green Version]
  28. Yasmin, T.; Rahman, M.M.; Khan, F.; Kabir, F.; Nahar, K.; Lasker, S.; Islam, M.D.; Hossain, M.M.; Hasan, R.; Rana, S.; et al. Metformin treatment reverses high fat diet- induced non-alcoholic fatty liver diseases and dyslipidemia by stimulating multiple antioxidant and anti-inflammatory pathways. Biochem. Biophys. Rep. 2021, 28, 101168. [Google Scholar] [CrossRef]
  29. Kuna, L.; Bozic, I.; Kizivat, T.; Bojanic, K.; Mrso, M.; Kralj, E.; Smolic, R.; Wu, G.Y.; Smolic, M. Models of Drug Induced Liver Injury (DILI)—Current Issues and Future Perspectives. Curr. Drug Metab. 2018, 19, 830–838. [Google Scholar] [CrossRef] [PubMed]
  30. Gupta, N.A.; Mells, J.; Dunham, R.M.; Grakoui, A.; Handy, J.; Saxena, N.K.; Anania, F.A. Glucagon-like peptide-1 receptor is present on human hepatocytes and has a direct role in decreasing hepatic steatosis in vitro by modulating elements of the insulin signaling pathway. Hepatology 2010, 51, 1584–1592. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  31. Chavez, C.P.; Cusi, K.; Kadiyala, S. The Emerging Role of Glucagon-like Peptide-1 Receptor Agonists for the Management of NAFLD. J. Clin. Endocrinol. Metab. 2022, 107, 29–38. [Google Scholar] [CrossRef] [PubMed]
  32. Fang, Y.; Ji, L.; Zhu, C.; Xiao, Y.; Zhang, J.; Lu, J.; Yin, J.; Wei, L. Liraglutide Alleviates Hepatic Steatosis by Activating the TFEB-Regulated Autophagy-Lysosomal Pathway. Front. Cell Dev. Biol. 2020, 8, 602574. [Google Scholar] [CrossRef]
  33. Li, X.; Wu, X.; Jia, Y.; Fu, J.; Zhang, L.; Jiang, T.; Liu, J.; Wang, G. Liraglutide Decreases Liver Fat Content and Serum Fibroblast Growth Factor 21 Levels in Newly Diagnosed Overweight Patients with Type 2 Diabetes and Nonalcoholic Fatty Liver Disease. J. Diabetes Res. 2021, 2021, 3715026. [Google Scholar] [CrossRef]
  34. Song, T.; Jia, Y.; Li, Z.; Wang, F.; Ren, L.; Chen, S. Effects of Liraglutide on Nonalcoholic Fatty Liver Disease in Patients with Type 2 Diabetes Mellitus: A Systematic Review and Meta-Analysis. Diabetes Ther. 2021, 12, 1735–1749. [Google Scholar] [CrossRef] [PubMed]
  35. Ricchi, M.; Odoardi, M.R.; Carulli, L.; Anzivino, C.; Ballestri, S.; Pinetti, A.; Fantoni, L.I.; Marra, F.; Bertolotti, M.; Banni, S.; et al. Differential effect of oleic and palmitic acid on lipid accumulation and apoptosis in cultured hepatocytes. J. Gastroenterol. Hepatol. 2009, 24, 830–840. [Google Scholar] [CrossRef] [PubMed]
  36. Van Summeren, A.; Renes, J.; Bouwman, F.G.; Noben, J.P.; van Delft, J.H.; Kleinjans, J.C.; Mariman, E.C. Proteomics investigations of drug-induced hepatotoxicity in HepG2 cells. Toxicol. Sci. 2011, 120, 109–122. [Google Scholar] [CrossRef] [Green Version]
  37. Volarevic, M.; Wu, C.H.; Smolic, R.; Andorfer, J.H.; Wu, G.Y. A novel G418 conjugate results in targeted selection of genetically protected hepatocytes without bystander toxicity. Bioconjug. Chem. 2007, 18, 1965–1971. [Google Scholar] [CrossRef] [PubMed]
  38. Zjalić, M.; Mustapić, M.; Glumac, Z.; Prološčić, I.; Blažetić, S.; Vuković, A.; Masud, M.; Billah, M.; Khan, A.; Šegota, S.; et al. Construction of AC/DC magnetic syringe device for stimulated drug release, injection and ejection of nanocarriers and testing cytotoxicity. MethodsX 2021, 8, 101312. [Google Scholar] [CrossRef] [PubMed]
  39. Rueden, C.T.; Schindelin, J.; Hiner, M.C.; DeZonia, B.E.; Walter, A.E.; Arena, E.T.; Eliceiri, K.W. ImageJ2: ImageJ for the next generation of scientific image data. BMC Bioinform. 2017, 18, 529. [Google Scholar] [CrossRef]
  40. Zhao, F.; Xie, P.; Jiang, J.; Zhang, L.; An, W.; Zhan, Y. The effect and mechanism of tamoxifen-induced hepatocyte steatosis In Vitro. Int. J. Mol. Sci. 2014, 15, 4019–4030. [Google Scholar] [CrossRef] [Green Version]
  41. Felser, A.; Lindinger, P.W.; Schnell, D.; Kratschmar, D.V.; Odermatt, A.; Mies, S.; Jenö, P.; Krähenbühl, S. Hepatocellular toxicity of benzbromarone: Effects on mitochondrial function and structure. Toxicology 2014, 324, 136–146. [Google Scholar] [CrossRef] [PubMed]
  42. Allard, J.; Bucher, S.; Massart, J.; Ferron, P.J.; Le Guillou, D.; Loyant, R.; Daniel, Y.; Launay, Y.; Buron, N.; Begriche, K.; et al. Drug-induced hepatic steatosis in absence of severe mitochondrial dysfunction in HepaRG cells: Proof of multiple mechanism-based toxicity. Cell Biol. Toxicol. 2021, 37, 151–175. [Google Scholar] [CrossRef] [PubMed]
  43. Zhou, Y.; Hua, J.; Barritt, G.; Liu, Y.; Tang, B.Z.; Tang, Y. Live Imaging and Quantitation of Lipid Droplets and Mitochondrial Membrane Potential Changes with Aggregation-Induced Emission Luminogens in an In Vitro Model of Liver Steatosis. Chembiochem 2019, 20, 1256–1259. [Google Scholar] [CrossRef]
  44. Sanoh, S.; Yamachika, Y.; Tamura, Y.; Kotake, Y.; Yoshizane, Y.; Ishida, Y.; Tateno, C.; Ohta, S. Assessment of amiodarone-induced phospholipidosis in chimeric mice with a humanized liver. J. Toxicol. Sci. 2017, 42, 589–596. [Google Scholar] [CrossRef] [Green Version]
  45. Takahashi, Y.; Fukusato, T. Histopathology of nonalcoholic fatty liver disease/nonalcoholic steatohepatitis. World J. Gastroenterol. 2014, 20, 15539–15548. [Google Scholar] [CrossRef]
  46. Tandra, S.; Yeh, M.M.; Brunt, E.M.; Vuppalanchi, R.; Cummings, O.W.; Ünalp-Arida, A.; Wilson, L.A.; Chalasani, N. Presence and significance of microvesicular steatosis in nonalcoholic fatty liver disease. J. Hepatol. 2011, 55, 654–659. [Google Scholar] [CrossRef] [Green Version]
  47. Li, T.; Li, X.; Meng, H.; Chen, L.; Meng, F. ACSL1 affects Triglyceride Levels through the PPARγ Pathway. Int. J. Med. Sci. 2020, 17, 720–727. [Google Scholar] [CrossRef] [Green Version]
  48. Li, L.O.; Ellis, J.M.; Paich, H.A.; Wang, S.; Gong, N.; Altshuller, G.; Thresher, R.J.; Koves, T.R.; Watkins, S.M.; Muoio, D.M.; et al. Liver-specific loss of long chain acyl-CoA synthetase-1 decreases triacylglycerol synthesis and beta-oxidation and alters phospholipid fatty acid composition. J. Biol. Chem. 2009, 284, 27816–27826. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  49. Zeng, S.; Wu, F.; Chen, M.; Li, Y.; You, M.; Zhang, Y.; Yang, P.; Wei, L.; Ruan, X.Z.; Zhao, L.; et al. Inhibition of Fatty Acid Translocase (FAT/CD36) Palmitoylation Enhances Hepatic Fatty Acid β-Oxidation by Increasing Its Localization to Mitochondria and Interaction with Long-Chain Acyl-CoA Synthetase 1. Antioxid. Redox Signal. 2022, 36, 1081–1100. [Google Scholar] [CrossRef]
  50. Yang, Z.; Yu, G.L.; Zhu, X.; Peng, T.H.; Lv, Y.C. Critical roles of FTO-mediated mRNA m6A demethylation in regulating adipogenesis and lipid metabolism: Implications in lipid metabolic disorders. Genes Dis. 2022, 9, 51–61. [Google Scholar] [CrossRef] [PubMed]
  51. Wang, Y.; Nakajima, T.; Gonzalez, F.J.; Tanaka, N. PPARs as Metabolic Regulators in the Liver: Lessons from Liver-Specific PPAR-Null Mice. Int. J. Mol. Sci. 2020, 21, 2061. [Google Scholar] [CrossRef] [PubMed] [Green Version]
  52. Szalowska, E.; van der Burg, B.; Man, H.Y.; Hendriksen, P.J.; Peijnenburg, A.A. Model steatogenic compounds (amiodarone, valproic acid, and tetracycline) alter lipid metabolism by different mechanisms in mouse liver slices. PLoS ONE 2014, 9, e86795. [Google Scholar] [CrossRef] [Green Version]
  53. Guzmán, C.; Benet, M.; Pisonero-Vaquero, S.; Moya, M.; García-Mediavilla, M.V.; Martínez-Chantar, M.L.; Gonzállez-Gallego, J.; Castell, J.V.; Sánchez-Campos, S.; Jover, R. The human liver fatty acid binding protein (FABP1) gene is activated by FOXA1 and PPARα; and repressed by C/EBPα: Implications in FABP1 down-regulation in nonalcoholic fatty liver disease. Biochim. Biophys. Acta 2013, 1831, 803–818. [Google Scholar] [CrossRef]
  54. Jackson, S.H.; Martin, T.S.; Jones, J.D.; Seal, D.; Emanuel, F. Liraglutide (victoza): The first once-daily incretin mimetic injection for type-2 diabetes. P T 2010, 35, 498–529. [Google Scholar]
  55. Ao, N.; Ma, Z.; Yang, J.; Jin, S.; Zhang, K.; Luo, E.; Du, J. Liraglutide ameliorates lipotoxicity-induced inflammation through the mTORC1 signalling pathway. Peptides 2020, 133, 170375. [Google Scholar] [CrossRef]
  56. Petit, J.M.; Cercueil, J.P.; Loffroy, R.; Denimal, D.; Bouillet, B.; Fourmont, C.; Chevallier, O.; Duvillard, L.; Vergés, B. Effect of Liraglutide Therapy on Liver Fat Content in Patients with Inadequately Controlled Type 2 Diabetes: The Lira-NAFLD Study. J. Clin. Endocrinol. Metab. 2017, 102, 407–415. [Google Scholar] [CrossRef] [PubMed]
  57. Yang, M.; Ma, X.; Xuan, X.; Deng, H.; Chen, Q.; Yuan, L. Liraglutide Attenuates Non-Alcoholic Fatty Liver Disease in Mice by Regulating the Local Renin-Angiotensin System. Front. Pharmacol. 2020, 11, 432. [Google Scholar] [CrossRef] [Green Version]
  58. Flock, G.; Baggio, L.L.; Longuet, C.; Drucker, D.J. Incretin receptors for glucagon-like peptide 1 and glucose-dependent insulinotropic polypeptide are essential for the sustained metabolic actions of vildagliptin in mice. Diabetes 2007, 56, 3006–3013. [Google Scholar] [CrossRef]
  59. Ni, X.X.; Li, X.Y.; Wang, Q.; Hua, J. Regulation of peroxisome proliferator-activated receptor-gamma activity affects the hepatic stellate cell activation and the progression of NASH via TGF-β1/Smad signaling pathway. J. Physiol. Biochem. 2021, 77, 35–45. [Google Scholar] [CrossRef]
  60. Liu, X.; Xu, J.; Rosenthal, S.; Zhang, L.J.; McCubbin, R.; Meshgin, N.; Shang, L.; Koyama, Y.; Ma, H.Y.; Sharma, S.; et al. Identification of Lineage-Specific Transcription Factors That Prevent Activation of Hepatic Stellate Cells and Promote Fibrosis Resolution. Gastroenterology 2020, 158, 1728–1744.e14. [Google Scholar] [CrossRef] [Green Version]
  61. Li, J.; Guo, C.; Wu, J. The Agonists of Peroxisome Proliferator-Activated Receptor-γ for Liver Fibrosis. Drug Des. Devel Ther. 2021, 15, 2619–2628. [Google Scholar] [CrossRef]
  62. Quintero, P.; Arrese, M. Nuclear control of inflammation and fibrosis in nonalcoholic steatohepatitis: Therapeutic potential of dual peroxisome proliferator-activated receptor alpha/delta agonism. Hepatology 2013, 58, 1881–1884. [Google Scholar] [CrossRef] [PubMed]
  63. Tao, L.L.; Ding, D.; Yin, W.H.; Peng, J.Y.; Hou, C.J.; Liu, X.P.; Chen, Y.I. TSA increases C/EBP-α expression by increasing its lysine acetylation in hepatic stellate cells. Mol. Med. Rep. 2017, 16, 6088–6093. [Google Scholar] [CrossRef] [Green Version]
  64. Mei, S.; Wang, X.; Zhang, J.; Qian, J.; Ji, J. In Vivo transfection of C/EBP-alpha gene could ameliorate CCL(4)-induced hepatic fibrosis in mice. Hepatol. Res. 2007, 37, 531–539. [Google Scholar] [CrossRef]
  65. Tao, L.L.; Cheng, Y.Y.; Ding, D.; Mei, S.; Xu, J.W.; Yu, J.; Ou-Yang, Q.; Deng, L.; Chen, Q.; Li, Q.Q.; et al. C/EBP-α ameliorates CCl(4)-induced liver fibrosis in mice through promoting apoptosis of hepatic stellate cells with little apoptotic effect on hepatocytes in vitro and In Vivo. Apoptosis 2012, 17, 492–502. [Google Scholar] [CrossRef]
  66. Wang, X.; Huang, G.; Mei, S.; Qian, J.; Ji, J.; Zhang, J. Over-expression of C/EBP-alpha induces apoptosis in cultured rat hepatic stellate cells depending on p53 and peroxisome proliferator-activated receptor-gamma. Biochem. Biophys. Res. Commun. 2009, 380, 286–291. [Google Scholar] [CrossRef]
  67. Liu, H.; Zhan, Y.L.; Luo, G.J.; Zou, L.L.; Li, Y.; Lu, H.Y. Liraglutide and Insulin Have Contrary Effects on Adipogenesis of Human Adipose-Derived Stem Cells via Wnt Pathway. Diabetes Metab. Syndr. Obes. 2020, 13, 3075–3087. [Google Scholar] [CrossRef]
  68. Sanz, C.; Vázquez, P.; Blázquez, C.; Barrio, P.A.; Alvarez, M.e.M.; Blázquez, E. Signaling and biological effects of glucagon-like peptide 1 on the differentiation of mesenchymal stem cells from human bone marrow. Am. J. Physiol. Endocrinol. Metab. 2010, 298, E634–E643. [Google Scholar] [CrossRef] [Green Version]
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Figure 1. Determination of cell viability by MTT assay after exposure to varying amiodarone (AMD) and oleic acid (OA) concentrations and varying time periods in the Huh7 cell line. MTT measurements were done by spectrophotometry at 595 nm. Results are shown as a percentage relative to the negative control of at least three biological replicates. Two-way ANOVA Time period F (2, 71) = 88.8; p = 7.41 × 10−17, Treatment F (7, 71) = 741.1; p = 1.23 × 10−46; post-hoc Tukey HSD. Bars assigned with asterisks are statistically significantly different (*** p < 0.001) compared to the negative control. Dulbecco’s modified Eagle’s medium (DMEM), oleic acid (OA/mM), amiodarone (AMD/µM).
Figure 1. Determination of cell viability by MTT assay after exposure to varying amiodarone (AMD) and oleic acid (OA) concentrations and varying time periods in the Huh7 cell line. MTT measurements were done by spectrophotometry at 595 nm. Results are shown as a percentage relative to the negative control of at least three biological replicates. Two-way ANOVA Time period F (2, 71) = 88.8; p = 7.41 × 10−17, Treatment F (7, 71) = 741.1; p = 1.23 × 10−46; post-hoc Tukey HSD. Bars assigned with asterisks are statistically significantly different (*** p < 0.001) compared to the negative control. Dulbecco’s modified Eagle’s medium (DMEM), oleic acid (OA/mM), amiodarone (AMD/µM).
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Figure 2. Determination of cell viability by MTT assay after exposure of Huh7 cells to OA, AMD and different LIRA concentrations for 24 h. MTT measurements were done by spectrophotometry at 595 nm. Results are shown as a percentage relative to the negative control of at least three biological replicates. One-way ANOVA F (11, 71) = 37.61; p = 8.38 × 10−23 Mann-Whitney pairwise. Bars assigned with asterisks indicate statistically significant differences (* p < 0.05, ** p < 0.01). Dulbecco’s modified Eagle’s medium (DMEM) as a negative control, liraglutide (LIRA/nM), oleic acid (OA/mM), amiodarone (AMD/µM).
Figure 2. Determination of cell viability by MTT assay after exposure of Huh7 cells to OA, AMD and different LIRA concentrations for 24 h. MTT measurements were done by spectrophotometry at 595 nm. Results are shown as a percentage relative to the negative control of at least three biological replicates. One-way ANOVA F (11, 71) = 37.61; p = 8.38 × 10−23 Mann-Whitney pairwise. Bars assigned with asterisks indicate statistically significant differences (* p < 0.05, ** p < 0.01). Dulbecco’s modified Eagle’s medium (DMEM) as a negative control, liraglutide (LIRA/nM), oleic acid (OA/mM), amiodarone (AMD/µM).
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Figure 3. Quantification and visualization of the lipid accumulation with Oil-Red O-dye. (a) Visualization of lipid accumulation with Oil-Red-O dye. Lipid accumulation in Huh7 cells was visualized with Oil-Red-O dye, while DAPI (blue color) was used to stain nuclei. (A)—DMEM (negative control), (B)—5 nM LIRA, (C)—10 nM LIRA, (D)—20 nM LIRA, (E)—0.5 mM OA, (F)—0.5 mM OA and 5 nM LIRA, (G)—0.5 mM OA and 10 nM LIRA, (H)—0.5 mM OA and 20 nM LIRA, (I)—20 µM AMD, (J)—20 µM AMD and 5 nM LIRA, (K)—20 µM AMD and 10 nM LIRA, (L)—20 µM AMD and 20 nM LIRA. Size bar represents 10 µm. Dulbecco’s modified Eagle’s medium (DMEM), liraglutide (LIRA/nM), oleic acid (OA/mM), amiodarone (AMD/µM). (b) Levels of lipids stained with Oil-Red-O dye in the Huh7 cells treated with OA, AMD, and LIRA. Data represent the integrated density of red color relative to the cell count. A higher number equals a more intense stain. Results are shown as a percentage relative to the negative control. One way ANOVA F (11, 130) = 66.2; p = 2.54 × 10−45; Mann-Whitney U (Bonferroni-corrected p-value). Bars assigned with asterisks are statistically significantly different (* p < 0.05, ** p < 0.01). The data are shown as the means ± SD (standard deviation) from at least three biological replicates. Dulbecco’s modified Eagle’s medium (DMEM), liraglutide (LIRA/nM), oleic acid (OA/mM), amiodarone (AMD/µM).
Figure 3. Quantification and visualization of the lipid accumulation with Oil-Red O-dye. (a) Visualization of lipid accumulation with Oil-Red-O dye. Lipid accumulation in Huh7 cells was visualized with Oil-Red-O dye, while DAPI (blue color) was used to stain nuclei. (A)—DMEM (negative control), (B)—5 nM LIRA, (C)—10 nM LIRA, (D)—20 nM LIRA, (E)—0.5 mM OA, (F)—0.5 mM OA and 5 nM LIRA, (G)—0.5 mM OA and 10 nM LIRA, (H)—0.5 mM OA and 20 nM LIRA, (I)—20 µM AMD, (J)—20 µM AMD and 5 nM LIRA, (K)—20 µM AMD and 10 nM LIRA, (L)—20 µM AMD and 20 nM LIRA. Size bar represents 10 µm. Dulbecco’s modified Eagle’s medium (DMEM), liraglutide (LIRA/nM), oleic acid (OA/mM), amiodarone (AMD/µM). (b) Levels of lipids stained with Oil-Red-O dye in the Huh7 cells treated with OA, AMD, and LIRA. Data represent the integrated density of red color relative to the cell count. A higher number equals a more intense stain. Results are shown as a percentage relative to the negative control. One way ANOVA F (11, 130) = 66.2; p = 2.54 × 10−45; Mann-Whitney U (Bonferroni-corrected p-value). Bars assigned with asterisks are statistically significantly different (* p < 0.05, ** p < 0.01). The data are shown as the means ± SD (standard deviation) from at least three biological replicates. Dulbecco’s modified Eagle’s medium (DMEM), liraglutide (LIRA/nM), oleic acid (OA/mM), amiodarone (AMD/µM).
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Figure 4. Triglyceride content in DIS and NAS cell culture models, incubated with varying concentrations of LIRA. One-way ANOVA F (11, 35) = 579.2; p = 2.62 × 10−26 post-hoc Tukey HSD. Bars assigned with asterisks are statistically significantly different (*** p < 0.001). The data are shown as the means ± SD (standard deviation) from at least three biological replicates. Dulbecco’s modified Eagle’s medium (DMEM), LIRA (LIRA/nM), oleic acid (OA/mM), amiodarone (AMD/µM).
Figure 4. Triglyceride content in DIS and NAS cell culture models, incubated with varying concentrations of LIRA. One-way ANOVA F (11, 35) = 579.2; p = 2.62 × 10−26 post-hoc Tukey HSD. Bars assigned with asterisks are statistically significantly different (*** p < 0.001). The data are shown as the means ± SD (standard deviation) from at least three biological replicates. Dulbecco’s modified Eagle’s medium (DMEM), LIRA (LIRA/nM), oleic acid (OA/mM), amiodarone (AMD/µM).
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Figure 5. Expression of ACSL1, C/EBPα, PPARγ and SREBP-1c in cell culture models of NAS and DIS. The gene expression was determined by RT-PCR. PCR results were visualized on a 1.6% agarose gel stained with Diamond™ Nucleic Acid Dye (Promega, Madison, WI, USA) according to the manufacturer’s instructions, visualized by Gel Imaging System (ChemiDocTM Imaging System, Bio-Rad, Hercules, CA, USA). The images were semi-quantified by Image Lab 6.0.1 build 34 Bio-Rad Laboratories (normalized to the housekeeping gene β-actin mRNA levels) (39). Results are shown as a percentage relative to the negative control of at least three biological replicates. (A) ACSL1 gene expression in Huh7 cells. One-way ANOVA F (11, 35) = 12.8 p = 1.63 × 10−07 post-hoc Tukey HSD test; * p < 0.05, *** p < 0.001. (B) C/EBPα gene expression in Huh7 cells. One-way ANOVA F (11, 47) = 2.661, p = 0.01317; post-hoc Tukey HSD test. (C) PPARγ gene expression in Huh7 cells. One-way ANOVA F (11, 59) = 4.415, p = 0.000142; Mann-Whitney U test * p < 0.05. (D) SREBP-1c gene expression in Huh7 cells. One-way ANOVA F (11, 59) = 4.241, p = 0.000212; post-hoc Tukey HSD test; * p < 0.05, ** p < 0.01. Dulbecco’s modified Eagle’s medium (DMEM), LIRA (LIRA/nM), oleic acid (OA/mM), amiodarone (AMD/µM), Acyl-CoA Synthetase Long Chain Family Member 1 (ACSL1), CCAAT/enhancer-binding protein α (C/EBPα), peroxisome proliferator-activated receptor gamma (PPARγ), sterol regulatory element binding transcription factor 1c (SREBP-1c).
Figure 5. Expression of ACSL1, C/EBPα, PPARγ and SREBP-1c in cell culture models of NAS and DIS. The gene expression was determined by RT-PCR. PCR results were visualized on a 1.6% agarose gel stained with Diamond™ Nucleic Acid Dye (Promega, Madison, WI, USA) according to the manufacturer’s instructions, visualized by Gel Imaging System (ChemiDocTM Imaging System, Bio-Rad, Hercules, CA, USA). The images were semi-quantified by Image Lab 6.0.1 build 34 Bio-Rad Laboratories (normalized to the housekeeping gene β-actin mRNA levels) (39). Results are shown as a percentage relative to the negative control of at least three biological replicates. (A) ACSL1 gene expression in Huh7 cells. One-way ANOVA F (11, 35) = 12.8 p = 1.63 × 10−07 post-hoc Tukey HSD test; * p < 0.05, *** p < 0.001. (B) C/EBPα gene expression in Huh7 cells. One-way ANOVA F (11, 47) = 2.661, p = 0.01317; post-hoc Tukey HSD test. (C) PPARγ gene expression in Huh7 cells. One-way ANOVA F (11, 59) = 4.415, p = 0.000142; Mann-Whitney U test * p < 0.05. (D) SREBP-1c gene expression in Huh7 cells. One-way ANOVA F (11, 59) = 4.241, p = 0.000212; post-hoc Tukey HSD test; * p < 0.05, ** p < 0.01. Dulbecco’s modified Eagle’s medium (DMEM), LIRA (LIRA/nM), oleic acid (OA/mM), amiodarone (AMD/µM), Acyl-CoA Synthetase Long Chain Family Member 1 (ACSL1), CCAAT/enhancer-binding protein α (C/EBPα), peroxisome proliferator-activated receptor gamma (PPARγ), sterol regulatory element binding transcription factor 1c (SREBP-1c).
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Table
Table 1. PCR conditions for amplification of different genes.
Table 1. PCR conditions for amplification of different genes.
GeneDenaturationAnnealingElongation
β-actin94 °C for 3 min56.7 °C for 45 s72 °C for 1 min in 30 cycles
ACSL194 °C for 3 min61 °C for 45 s72 °C for 1 min in 30 cycles
C/EBPα94 °C for 3 min61 °C for 45 s72 °C for 1 min in 30 cycles
PPARγ94 °C for 3 min61 °C for 45 s72 °C for 1 min in 30 cycles
SREBP-1c94 °C for 3 min61 °C for 45 s72 °C for 1 min in 30 cycles
Table
Table 2. Primer sequences used for RT (Reverse transcription)-PCR.
Table 2. Primer sequences used for RT (Reverse transcription)-PCR.
GenePrimer Sequences (5′-3′)
β-actinForward GCACCACACCTTCTACAATG
Reverse TGCTTGCTGATCCACATCTG
ACSL1Forward GGAGTGGGCTGCAGTGAC
Reverse GGGCTTGCATTGTCCTGT
C/EBPαForward CGCCTTCAACGACGAGTTCCTG
Reverse CGCCTTGGCCTTCTCCTGCT
PPARγForward ACCAAAGTGCAATCAAAGTGGA
Reverse ATGAGGGAGTTGGAAGGCTCT
SREBP-1cForward CGGAACCATCTTGGCAACAGT
Reverse CGCTTCTCAATGGCGTTGT
ACSL1—Acyl-CoA Synthetase Long Chain Family Member 1, C/EBPα—CCAAT/enhancer-binding protein α, PPAR γ—peroxisome proliferator-activated receptor gamma, SREBP-1c—sterol regulatory element binding transcription factor 1c [40,41].
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Omanovic Kolaric, T.; Kizivat, T.; Mihaljevic, V.; Zjalic, M.; Bilic-Curcic, I.; Kuna, L.; Smolic, R.; Vcev, A.; Wu, G.Y.; Smolic, M. Liraglutide Exerts Protective Effects by Downregulation of PPARγ, ACSL1 and SREBP-1c in Huh7 Cell Culture Models of Non-Alcoholic Steatosis and Drug-Induced Steatosis. Curr. Issues Mol. Biol. 2022, 44, 3465-3480. https://doi.org/10.3390/cimb44080239

AMA Style

Omanovic Kolaric T, Kizivat T, Mihaljevic V, Zjalic M, Bilic-Curcic I, Kuna L, Smolic R, Vcev A, Wu GY, Smolic M. Liraglutide Exerts Protective Effects by Downregulation of PPARγ, ACSL1 and SREBP-1c in Huh7 Cell Culture Models of Non-Alcoholic Steatosis and Drug-Induced Steatosis. Current Issues in Molecular Biology. 2022; 44(8):3465-3480. https://doi.org/10.3390/cimb44080239

Chicago/Turabian Style

Omanovic Kolaric, Tea, Tomislav Kizivat, Vjera Mihaljevic, Milorad Zjalic, Ines Bilic-Curcic, Lucija Kuna, Robert Smolic, Aleksandar Vcev, George Y. Wu, and Martina Smolic. 2022. "Liraglutide Exerts Protective Effects by Downregulation of PPARγ, ACSL1 and SREBP-1c in Huh7 Cell Culture Models of Non-Alcoholic Steatosis and Drug-Induced Steatosis" Current Issues in Molecular Biology 44, no. 8: 3465-3480. https://doi.org/10.3390/cimb44080239

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