Histone deacetylase 9 promoter hypomethylation associated with adipocyte dysfunction is a statin-related metabolic effect.

BACKGROUND: Adipogenesis, the process whereby preadipocytes differentiate into mature adipocytes, is crucial for maintaining metabolic homeostasis. Cholesterol-lowering statins increase type 2 diabetes (T2D) risk possibly by affecting adipogenesis and insulin resistance but the (epi)genetic mechanisms involved are unknown. Here, we characterised the effects of statin treatment on adipocyte differentiation using in vitro human preadipocyte cell model to identify putative effective genes.
RESULTS: Statin treatment during adipocyte differentiation caused a reduction in key genes involved in adipogenesis, such as ADIPOQ, GLUT4 and ABCG1. Using Illumina's Infinium '850K' Methylation EPIC array, we found a significant hypomethylation of cg14566882, located in the promoter of the histone deacetylase 9 (HDAC9) gene, in response to two types of statins (atorvastatin and mevastatin), which correlates with an increased HDAC9 mRNA expression. We confirmed that HDAC9 is a transcriptional repressor of the cholesterol efflux ABCG1 gene expression, which is epigenetically modified in obesity and prediabetic states. Thus, we assessed the putative impact of ABCG1 knockdown in mimicking the effect of statin in adipogenesis. ABCG1 KD reduced the expression of key genes involved in adipocyte differentiation and decreased insulin signalling and glucose uptake. In human blood cells from two cohorts, ABCG1 expression was impaired in response to statins, confirming that ABCG1 is targeted in vivo by these drugs.
CONCLUSIONS: We identified an epigenetic link between adipogenesis and adipose tissue insulin resistance in the context of T2D risk associated with statin use, which has important implications as HDAC9 and ABCG1 are considered potential therapeutic targets for obesity and metabolic diseases.

Background

Adipose tissue plays a crucial role in regulating insulin sensitivity and glucose homeostasis [1]. In obesity, adipose expansion occurs as a result of cellular hypertrophy, i.e. the increase in size of the adipocyte and/or de novo adipogenesis, which is the production of new mature adipocytes from residing preadipocytes [2-4]. Dysregulation in the adipogenic process is associated with metabolic diseases and insulin resistance [5] and is an independent risk factor for type 2 diabetes (T2D) [6]. In contrast, appropriate adipocyte expansion is protective against T2D in the context of obesity [6, 7]. Adipogenesis occurs as a result of metabolic cues that trigger the induction of key differentiation regulators, such as ADIPOQ, FASN, PPARg, ABCG1 and GLUT4 [8-11]. Epigenome-wide association studies (EWAS) have found that hypermethylation within one of these genes involved in adipogenesis, ABCG1, was associated with increased body mass index (BMI), insulin resistance and T2D risk [12-15], opening avenues in the elucidation of the links between adipogenesis and metabolic diseases.

One of the most common drugs known to modulate adipogenesis are statins [16]. As a role for statins as a DNA methylation inhibitor has previously been reported [17], we hypothesised that statin treatment modulates adipogenesis by modifying the adipocyte epigenome. In this study, we confirmed the inhibitory effects of statin treatment in human preadipocytes and investigated the methylome to identify potential regulators that may be involved in adipogenesis.

Results

Statin treatment reduced adipogenesis and insulin signalling

The Simpson-Golabi-Behmel syndrome (SGBS) human preadipocyte cell line was used in this study as an in vitro model for adipocyte differentiation. In SGBS cells, lipid droplet formation occurred by 12–14 days of differentiation together with an increase in the expression of key adipogenic markers [18]. We retrieved adequate SGBS cell morphology modification and formation of lipid droplets by day 12 (Additional File 1: Figure S1a), and observed that the expression of key genes involved in adipocyte differentiation and maturation was accordingly upregulated (Additional File 1: Figure S1b).

For statin treatment, SGBS cells were differentiated for 6 days and then treated with atorvastatin and mevastatin for an additional 6 days until final maturation (Fig. 1a). We found a decrease in lipid in statin-treated SGBS cells (both atorvastatin and mevastatin) when compared to DMSO-vehicle controls (p < 0.05; Fig. 1b). We also found that statin treatment induced a significant downregulation of many key genes associated with adipogenesis reported above (ABCG1, LEPTIN and GLUT4), with the particular exclusion of PPARG, a gene known to play a role only in the early stages of adipocytes differentiation (Fig. 1c). In adipocytes, insulin binds to the insulin receptor, which then activates a signalling cascade through the phosphorylation of Akt and Erk, thereby stimulating the translocation of GLUT4 to the plasma membrane. Therefore, analysing pAkt and pErk is a measure of insulin signalling and sensitivity. We found a decreased efficiency of insulin to activate ERK and AKT (Fig. 1d). Taken together, the data support the inhibitory effects of statin in the human adipocyte differentiation and insulin signalling, a similar effect reported in statin-treated 3T3-L1 mouse adipocyte cells [16].

Fig. 1

Response of SGBS cell line to statin treatment. a The method used in treating the SGBS cell line at day 6 of differentiation for 6 days. b Quantification of lipid by red-oil in DMSO control, compared to mevastatin and atorvastatin-treated SGBS cells, performed in three technical replicates. *p < 0.05. c Expression of key adipose genes for statin-treated cells compared to time-matched DMSO controls (normalised to housekeeping gene B2M). *p < 0.05; **p < 0.01. d Protein expression of insulin signalling proteins pAkt and pErk in statin-treated cells compared to controls using WES

Methylome analysis of statin-treated SGBS cell line

To identify potential regulators involved in statin-induced adipocyte dysregulation, we performed an unbiased methylation analysis in statin-treated SGBS cells using Illumina’s Infinium ‘850K’ Methylation EPIC arrays (Additional File 1: Figure S2). We filtered differentially methylated positions (DMPs) located in the promoter region, annotated as TSS200 or TSS1500 (within 200–1500 bp from the transcription start site), in order to identify DMPs that were likely to have a biological effect. This filtering produced a total of 173,172 CpGs.

We focused our analysis on the “shared” CpGs between the two statin groups, (i.e. reproducible) and found 87 DMPs shared between the mevastatin and atorvastatin treatments (Additional File 2: Table S1, Figure S3). In mevastatin-treated cells, the most significant DMP was cg14566882, located in the promoter of the histone deacetylase (HDAC9) gene (β = 8.28%; p = 5.55 × 10−6) (Fig. 2a). Indeed, this DMP was also significantly hypomethylated in response to atorvastatin treatment, compared to DMSO-vehicle controls (β = 5.53%; p = 1.35 × 10−3) (Fig. 2a, b). Importantly, as HDAC9 has previously been found to be involved in adipocyte differentiation [19], we focused on this gene for further biological validation.

Fig. 2

Methylome analysis of statin-treated SGBS cells. a Volcano plots of methylome results for statin-treated cells (grey indicates log2 fold change < 1). b The hypomethylation of the cg14566882 CpG within the HDAC9 gene in atorvastatin and mevastatin-treated cells compared to vehicle-treated DMSO cells in the 4 biological replicates (raw β-values shown). c The mRNA expression level of HDAC9 in mevastatin and atorvastatin-treated SGSB cell line. *p < 0.05; **p < 0.01. d The protein expression of ABCG1 compared to housekeeping gene p84 shows a reduced expression in atorvastatin and mevastatin-treated SGBS cells. e ChIP qPCR using anti-HDAC9 antibody for the ABCG1 promoter for control (DMSO), mevastatin and atorvastatin-treated cells, normaled to no antibody (mock IgG) control. This experiment was performed in two biological replicates

A significant differentially methylated region (DMR) overlapping this promoter region was also found in response to both treatments (Additional File 1: Figure S4; False discovery rate < 0.05). In order to validate the effect of cg14566882 hypomethylation on the expression of the HDAC9 gene, we performed qPCRs in statin-treated SGBS cell lines and found significant upregulation of the HDAC9 gene at the mRNA level (p < 0.05; atorvastatin 14-fold; mevastatin11-fold) (Fig. 2c).

ABCG1 has been reported to be regulated by HDAC9-mediated changes in acetylation [20, 21] and may be targeted by the HDAC9 epigenetic alteration. We confirmed that ABCG1 protein expression is indeed downregulated in response to mevastatin and atorvastatin treatment (Fig. 2d). We confirmed that in response to statin, this effect was independent of the previously reported hypermethylation in cg06500161 (p value > 0.5) and cg27243685 (p value > 0.5) found to be associated with increased BMI and T2D incidence (Additional File 1: Table S2) [13, 14, 22, 23]. In addition, we confirmed that HDAC9 binds to the ABCG1 promoter, and this binding is increased in response to statin-treatment (Fig. 2e). This clearly illustrates that HDAC9 acts as a transcriptional repressor to ABCG1 expression in adipocytes in response to statin.

Knockdown of ABCG1 in SGBS preadipocytes reduced adipocyte differentiation

We performed an ABCG1 knockdown (KD) in SGBS cells to address whether reduced ABCG1 expression mimics the effect of statins in adipogenesis. SGBS preadipocytes were stably transfected with a shRNA targeting ABCG1 mRNA and followed them quantitatively through maturation and differentiation, and this data was compared with cells transfected with a non-targeting shRNA (control). A similar protocol for stably knockdown Abcg1 via shRNA has previously been achieved and described in mouse 3T3-L1 preadipocytes [24]. We initially analysed the expression of ABCG1 protein in normal adipocytes to show that it is positively associated with adipogenesis as ABCG1 starts to become expressed at day 6 of differentiation (Fig. 3a). The efficient silencing of ABCG1 (ABCG1 KD) was confirmed at the protein level (Fig. 3b). ABCG1 KD in SGBS cells was accompanied by a significant reduction in the lipid content (20% reduction, p < 0.05; Fig. 3c), along with the downregulation of the following adipocyte differentiation markers FASN, PPARG and PLIN1 and key adipocyte maturation markers ADIPOQ and GLUT4 (Fig. 3d). As a consequence of impaired adipogenesis, the ABCG1 KD led to a significant reduction in glucose uptake stimulated by insulin (65% reduction, p < 0.001; Fig. 3e). In addition, we found a decreased efficiency of insulin to activate AKT in those cells (Fig. 3f). As a whole, this data indicates that ABCG1 levels are pivotal for the control of human adipocyte differentiation and glucose metabolism.

Fig. 3

Adipogenesis changes in stably transfected ABCG1 KD cells. a Western blot protein expression of ABCG1 a during differentiation b after silencing in SGBS cell lines. c Lipid content analysed by red oil of ABCG1 KD compared to controls. d Expression of key adipose genes at day 12 differentiation in KD ABCG1 cells compared to shRNA controls, normalised to housekeeping gene B2M and compared to DMSO-vehicle controls. Experiments were performed at n = 4 biological replicates. e Glucose uptake in ABCG1 KD compared to controls stimulated with or without 1 μM insulin for 1 h. Fold change in KD and control cells compared to cells not treated with insulin. f Analysis of insulin signalling in SGBS ABCG1 KD cell line through protein expression of phosphorylated AKT at day 12, stimulated with or without 200 nM insulin for 1 h, using western blot analysis. *p < 0.05; **p < 0.001; ***p < 0.0001

ABCG1 is downregulated in response to statin in human blood samples

We next explored whether ABCG1 was also dysregulated in samples from human subjects. We analysed reported transcriptomic data from blood samples from two cohorts. The first consisted of a total of 57 individuals from the ECLIPSE cohort, of which 13 were statin users [25]. A significant reduction in the expression of ABCG1 in the statin group (p = 1.41 × 10−5) was found, compared to non-users (Fig. 4a). In addition, we also analysed data from the YELLOW II study [26], a retrospective study following 85 individuals before and following an extensive 8–12 week statin therapy. In peripheral blood mononuclear cells obtained from blood samples, ABCG1 expression was significantly decreased following statin treatment, compared to baseline levels, for two ABCG1 probes (ILMN_1794782 p = 2.76 × 10−5; ILMN_2329927 p = 4.28 x 10−4) (Fig. 4b). Taken together, this demonstrates that ABCG1 reduction in response to statin is indeed reflected in human blood samples. Of note, no data on HDAC9 expression was available in the ECLIPSE case control study, and no significant change in HDAC9 expression was reported in the intervention YELLOW II study, maybe due to the lack of sufficient statistical power of this study.

Fig. 4

The expression of ABCG1 in human samples. aABCG1 expression was reduced in 13 statin-treated individuals compared to control non-users using transcriptomic data. b Data from a total of 85 samples, after extensive statin treatment for 8–12 weeks, there was a reduction in ABCG1 expression compared to baseline levels in two probes

Discussion

A recent 15-year prospective study found a staggering 38% increased incidence of T2D in statin users, regardless of the type of statin used [27]. Here, we report that two statins, atorvastatin and mevastatin, hamper the differentiation process in the SGBS human preadipocyte cell line and decreased insulin sensitivity.

We focused our analysis on promoter DMPs, which are normally inversely correlated with expression [28, 29]. Therefore, not surprisingly, given the inhibitory effect of statin, our 850K methylation analysis revealed that most DMPs were hypermethylated. This includes the IDI1 gene, which encodes the isopentenyl diphosphate isomerase, a component of the cholesterol synthesising pathway [30, 31].

We report for the first time that statin treatment was associated with a significant hypomethylation of HDAC9 promoter, which is inversely correlated with HDAC9 gene expression. These findings are of particular significance in light of several studies that demonstrated the key role of HDAC9 in adipocytes function: overexpression of Hdac9 in 3T3-L1 preadipocyte mouse cell lines suppressed adipogenesis, and inversely, preadipocytes isolated from Hdac9 knockout mice had an accelerated adipocyte differentiation [32]. Furthermore, Hdac9 knockout mice showed improved metabolic homeostasis and were protected from adipose tissue dysfunction in mice fed on a high-fat feeding [19]. These studies clearly indicate the deleterious role of HDAC9 in maintaining adipocyte homeostasis both in vitro and in vivo.

In a study, it was shown that HDAC9-deficient macrophages and monocytes were directly involved in ABCG1 transcription [20, 21]. Indeed, we confirmed in our adipocyte in vitro model that HDAC9 binds directly to the ABCG1 promoter and acts as a transcriptional repressor for ABCG1 expression. This is of particular interest, as several studies have reported a role of ABCG1 in obesity, insulin resistance and T2D. Elevated ABCG1 expression is associated with increased fat mass from obese individuals, suggesting that ABCG1 is also involved in human adipogenesis [24]. Although genome-wide association studies have not found any single nucleotide polymorphisms (SNPs) within or nearby ABCG1 associated with increased T2D risk, several EWAS have found that hypermethylation in the ABCG1 gene was associated with fasting glucose, HbA1C levels, lipid metabolism, fasting insulin, T2D risk and BMI [13–15, 33–36]. Additional observations in mouse models have shown that Abcg1−/− mice were protected from high-fat diet-induced glucose intolerance [37]. A recent study found that ABCG1 expression is reduced in both subcutaneous and visceral adipose tissue in morbidly obese patients with metabolic syndrome compared to those without metabolic syndrome, providing further evidence for a role of ABCG1 in the maintenance of metabolic homeostasis in adipocytes [38]. In addition, two studies showed that ABCG1 expression was decreased in blood white human cells in response to statins. As ABCG1 was downregulated in response to statin, we hypothesised that ABCG1 plays a role in statin-induced adipocyte dysregulation.

Indeed, we showed that ABCG1 expression increases during human SGBS adipocyte differentiation and through ABCG1 silencing, confirm that the level of ABCG1 expression is crucial for the appropriate expression of lipid metabolism markers, which include FASN, FABP4, PLIN1 and PPARG, for correct human adipocyte differentiation. Our findings are consistent with previous data showing variation in these four genes following Abcg1 silencing in mouse 3T3-L1 pre-adipocyte cells [24]. The downregulation of GLUT4 in ABCG1 KD suggested a decrease in insulin-induced glucose uptake. Indeed, we confirmed a downregulation of phosphorylation of AKT and ERK. Collectively, this data indicates that normal ABCG1 function is required for adipogenesis and insulin signalling. In addition, we have confirmed using two separate datasets that statin use was indeed correlated with a reduction in ABCG1 expression in human blood samples. Other studies have reported a link between ABCG1 downregulation and diabetes incidence [39] and high fasting glycaemia [40]. Taken together, our human cellular data is consistent with human observational studies, in which the inhibition of ABCG1 expression was deleterious for metabolism in adipose tissue.

Our results focused on the effects of cg14566882 hypomethylation on HDAC9 expression; however, it is important to note that these changes could be mediated by other indirect CpG changes. Furthermore, despite the fact that we show that HDAC9 directly binds to the ABCG1 promoter as a statin effect, the relationship between cg14566882 hypomethylation and HDAC9 expression is correlative.

Conclusions

The model proposed based on our data from statin-induced insulin resistance is that hypomethylation of the HDAC9 promoter is correlated with HDAC9 gene expression, which acts as a transcriptional repressor to ABCG1 expression and thereby adipocyte differentiation and metabolic dysfunction (Fig. 5). Adipocyte turnover by adipogenesis is crucial for the maintenance of metabolic homeostasis and insulin sensitivity [41]. Our data provides a novel epigenetic link between adipogenesis dysfunction and insulin resistance, mediated by statins. The increased understanding of adipogenesis provides a promising new avenue for the treatment of metabolic disease in obesity [8, 41]. Both HDAC9 and ABCG1 have been proposed as therapeutic targets for patients with obesity in separate previous studies [19, 24]; however, our data support a mechanistic pathway linking them to metabolic diseases.

Fig. 5

A schematic representation of the role of adipocyte turnover in health and disease. In healthy individuals, preadipocytes differentiate into mature adipocytes, which have a role in maintaining insulin sensitivity. However, in response to statins, epigenetic changes in HDAC9 cause acetylation changes in ABCG1 and other crucial adipogenesis genes, which in-turn lead to an obstruction of differentiation and metabolic dysfunction

Methods

Cell culture and differentiation of SGBS cell line

For all the in vitro experiments, we used the SGBS cell line, a pre-adipocyte cell line that has not been transformed or immortalised and has the capacity to retain adipocyte differentiation in up to 50 passages [18]. This cell line was kindly provided by Prof. Dr. M. Wabitsch (University of Ulm, Germany) and maintained in DMEM/F12 supplemented with 10% foetal bovine serum and 0.01% penicillin/streptomycin (15140-122 - Life Technologies), as previously described [18]. Confluent preadipocytes were differentiated under serum-free culture conditions by washing twice with phosphate-buffered saline (PBS) and then exposing to DMEM/F12 supplemented with 2 μmol/l rosiglitazone, 25 nmol/l dexamethasone, 0.5 mmol/l methylisobuthylxantine, 0.1 μmol/l cortisol, 0.01 mg/ml transferrin, 0.2 nmol/l triiodotyronin and 20 nmol/l human insulin for 4 days. The cells were then cultured for a further 8 days in fresh DMEM/F12 supplemented with 0.1 μmol/l cortisol, 0.01 mg/ml transferrin, 0.2 nmol/l triiodotyronin and 20 nmol/l human insulin. Microscopic images of SGBS cells were taken under a microscope (IT404; VWR) using the Motic Image plus version 2.0 (Motic Europe).

Treatment with statins

At 6 days of differentiation, SGBS cells were treated with 10 μM mevastatin (M2537, Sigma Aldrich) or atorvastatin (PZ0001, Sigma Aldrich) and compared to a dimethyl sulfoxide (DMSO)-vehicle control (D2650, Sigma Aldrich). The cells were then incubated for a further 6 days. On day 12 of differentiation, cells were collected for further analysis.

850K Illumina methylation analysis

DNA was extracted from SGBS cells treated with atorvastatin and mevastatin at day 6 for 6 days and collected the cells at day 12. DNA was extracted using the NucleoSpin Tissue kit (Takara Bio). Bisulfite conversion of 500 ng genomic DNA was performed using the EZ-96 DNA Methylation kit (Zymo Research) following the manufacturer’s protocol. Bisulfite-converted DNA was subjected to genome-wide DNA methylation analysis using Illumina’s Infinium ‘850K’ Methylation EPIC array to identify differentially methylated positions (DMPs). The 850K methylationEPIC array was carefully designed to include a total of 850,000 CpGs from ENCODE open chromatin and enhancer, DNase hypersensitive sites and CpG islands. The resulting DNA methylation IDAT files were imported using the minfi R package for further processing and quality control [42]. The following CpG probes were excluded from further analysis: probes on sex chromosomes, cross-hybridising probes, non-cg probes and probes that lie near single nucleotide polymorphisms (SNPs). Probe-design biases and batch effects were normalised using R packages ENmix [43] and SVA (ComBat) [44], respectively.

To identify DMPs, the R package limma was used [45]. The model included treatment (atorvastatin, mevastatin or DMSO-vehicle) as a categorical variable and replicates/day of experiment as a covariate. Methylation levels denoted by beta-values, where 0 indicates 0% methylation and 1 indicates 100% methylation, were transformed to M values [46]. All statistical significance is based on the nominal p values. To identify differentially methylated regions (DMRs), the R package DMRcate was used [47], which uses Gaussian kernel smoothing based on the DMPs. All DMRs throughout the genome were tested.

RNA extraction, cDNA conversion and RT-PCR

Total RNA was extracted from cultured cells using a RiboPure RNA Purification Kit (AM1924; Invitrogen), according to the manufacturer’s instructions and quantified on a NanoDrop Spectrophotometer (Thermo Scientific). RNA was reverse transcribed using a High-Capacity RNA-to-cDNA Kit (4387406; Applied Biosystems), according to the manufacturer’s instructions. qPCRs were conducted on an Applied Biosystems 7900HT Fast Real-Time PCR System, and quantitative expression levels were obtained using the SDS v2.3 Software (Applied Biosystems) using Taqman Gene Expression Assays (ThermoFisher Scientific). The following probes were used: ABCG1 (Hs01555193_m1), CEBPB (Hs00270923_s1), LPL (Hs00173425_m1), ACACA (Hs01046047_m1) FABP4 (Hs01086177_m1), GLUT4 (Hs00168966_m1), ACACB (Hs00153715_m1), PPARG (Hs01115513_m1), CEBPA (Hs00269972_s1), ADIPOQ (Hs00605917_m1), FASN (Hs01005622_m1), SREBF1 (Hs01088691_m1) and PLIN1 (Hs00160173_m1) (Life Technologies). Each reaction was normalised to a beta-2-microglobulin (B2M) control (Hs00984230_m1; Applied Biosystems). For quantifications using SYBR-green, qPCRs were performed using (SsoAdvanced Universal SYBR Green Supermix, BioRad) using the BioRad CFX96 Real-Time PCR Detection System (Biorad). HDAC9 gene primer sequences were forward: AGTGGCAGAGAGGAGAAGCA and reverse: CAGTTCTCCAGGCTCTGGTC. At least three biological replicates were performed, and the data represents the means ± SEM. A two-tailed t test was performed using GraphPad Prism (GraphPad software Inc., La Jolla, USA), and p value < 0.05 was considered to be statistically significant.

Lipid quantification

Culture medium was removed, and the cells were washed twice with PBS and then fixed with 4% PFA for 10 min. Fixed cells were washed twice with water and incubated in 60% isopropanol twice. The alcohol was discarded, and the cells were then incubated in an Oil Red O (Sigma) and water solution (3:2) for 5 min. Cells were rinsed three times with water, and then 100% isopropanol was added to extract the red oil. The absorbance was measured at 5490 nm on a microplate reader.

Western blotting

Cells were washed twice in ice-cold PBS and harvested in RIPA buffer (ThermoFisher Scientific) supplemented with protease inhibitors. Cell lysates were centrifuged at 20,000×g for 20 min at 4 °C, and the total protein lysate was quantified using Bradford Reagent (B6916; Sigma). Then, 40 μg of total protein lysate was separated on a 4–12% Bis-Tris Plus Gel (Life Technologies) and transferred to a nitrocellulose membrane using the iBlot2 Gel Transfer Device (Life Technologies). Membranes were blocked in 0.5% non-fat dry milk and probed with anti-ABCG1 (1:1000; ab52617, abcam) and antinuclear matrix protein p84 (1:5000; ab487, abcam) primary antibodies anti-rabbit IgG (1:20,000; Ab205718, abcam), and anti-mouse IgG (1:5000; A4416, Sigma Aldrich) secondary antibodies for 1 h at room temperature. Membranes were exposed using Clarity Western ECL Substrate (Bio-Rad), and protein bands were detected on a LI-COR Imaging system with the C-DiGit Image Studio 4.0 software (LI-COR Biosciences, Ltd., UK).

Phosphorylated AKT analysis

Differentiated cells cultured in DMEM/F12 medium were serum starved overnight and then washed with PBS and stimulated with or without 200 nM insulin for 1 h in DMEM/F12 (without glucose or serum) at 37 °C in 5% CO2. The total protein was harvested in RIPA buffer supplemented with protease and phosphatase inhibitors, as described above. The primary antibodies (all used at 1:1000 dilution unless otherwise stated) used were anti pAKT (S473; Cell Signaling) and anti Akt (9272 - 1:5,000 dilution; Cell Signaling), and the secondary antibody used was goat pAb to Rb igG (Ab205718 - 1:20,000 dilution; Abcam). Protein expression studies were also performed by WES, an automated capillary-based size separation and nano-immunoassay system (ProteinSimple, San Jose CA, USA—a Bio-Techne Brand), according to manufacturer’s protocol, for analysis performed using the Compass for Simple Western software v.4.0. The WES was performed on SGBS samples (1:100) for anti pAKT (S473; Cell Signaling), anti Akt (9272 - 1:100 dilution; Cell Signaling), anti pERK (9102; Cell Signaling) and anti ERK (9101 - 1:100 dilution; Cell Signaling).

Glucose uptake assay

A Glucose Uptake-Glo Assay (J1342; Promega) was used to measure glucose uptake in differentiated cells (day 12), according to the manufacturer’s protocol. A total of 20,000 cells in 100 μl media were plated in each well of a 96-well white plate. Differentiated cells were cultured overnight in DMEM/F12 media with no serum. On the day of the assay, the media was replaced with 100 μl DMEM/F12 (without glucose or serum) supplemented with or without 1 μM insulin and incubated for 1 h at 37 °C in 5% CO2. Cells were washed with PBS and 50 μl 1 mM 2-Deoxy-D-glucose (2DG) was added to each well and incubated for 10 min at room temperature. Next, 25 μl Stop Buffer was added followed by 25 μl Neutralization Buffer per well. Finally, 100 μl 2DG6P Detection Reagent was added and incubated for 4.5 h at room temperature. The luminescence was recorded on a Mithras LB 940 luminometer (Berthold Technologies) and analysed using the MicroWin Software (Berthold Technologies).

Chromatin immunoprecipitation

Following differentiation and statin treatment, chromatin immunoprecipitation was performed using a ChIP assay (Abcam, ab500). A total of 3 × 106 cells per condition (DMSO, mevastatin and atorvastatin-treatment) were sheared to 200–700 bp using the Covaris AFATM (Adaptive Focused Acoustics) technology (200 cycles per burst and 8 min processing time). The sheared cells were incubated overnight with anti-HDAC9 antibody (ab59718) or negative control (no antibody). DNA-purified samples were analysed using SYBR green RT-PCR to amplify the ABCG1 promoter region using the forward primer 5′ GAGCCTCGCCAGCTCATTAT 3′ and the reverse primer 5′ TCCCAAGTGTTGCCCAAAGA 3′.

ABCG1 silencing using shRNA lentiviral vector

Undifferentiated SGBS cells were plated at 50% confluence in 6-well plates and infected with commercial lentiviral particles targeting either human ABCG1 (TRCN0000420907; Sigma) (TAGGAAGATGTAGGCAGATTG) or non-target controls (SHC202) (CCGGCAACAAGATGAAGAGCACCAACTC) and (TRCN0000158395; CCTACAGTGGATGTCCTACAT) (Sigma Aldrich). The transduced cells were selected in media containing 1 μg/ml puromycin for 6 days. Stable ABCG1 KD and control cells were then cultured and differentiated into mature adipocytes, as described above.

Analysis of transcriptomic data from human samples

Transcriptomic data (Affymetrix Human Gene 1.1 ST Array) from the GSE71220 dataset was downloaded from the GEO database. The subjects analysed were the 57 control samples from the Evaluation of COPD Longitudinally to Identify Predictive Surrogate Endpoints (ECLIPSE) study, of which 13 were statin-users [25]. In addition, transcriptomic data (Illumina HumanHT-12 WG-DASL V4.0 R2 expression beadchip) from peripheral blood mononuclear cells from the YELLOW II retrospective study (GSE86216) was also downloaded from the GEO dataset. This included blood samples from a total of 85 patients that were analysed before and after an extensive 8–12 week statin treatment [26]. For both datasets, the data was downloaded and analysed using the R packages GEOquery [42] and limma [45].

Additional file 1 – Supplementary Figures. Fig. S1: Differentiation of SGBS cell line. (a) Micorscopic mages of lipid droplets in pre-adipocytes (day 0) and differentiated mature adipocytes (day 12) visualised using microscopy (x10 magnification - scale bar 10 μM) (b) Expression of key adipose genes during a 12-day differentiation period (normalised to housekeeping gene B2M). For each gene, the fold-change compared to the day expression is first observed is presented. Data represent three biological replicates and plotted as the mean ± SEM. Fig. S2: All DMPs identified in response to a) mevastatin and b) atorvastatin treatment. Fig. S3: DMPs annotated to the promoter region that were also shared between mevastatin and atorvastatin treatments. Grey indicates log2 fold change < 1. Fig. S4: Differentially methylated region (DMR) in HDAC9 promoter shared between mevastatin and atorvastatin treatments.

Additional file 2 – Supplementary Tables. Table S1: Details of shared DMPs between mevastatin and atorvastatin-treated SGBS cells. Table S2: Details of CpG results in SGBS statin-treated cells in already reported to be associated wih BMI and T2D incidence.