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The metabolic regulator histone deacetylase 9 contributes to glucose homeostasis
abnormality induced by hepatitis C virus infection
Jizheng CHEN2, Ning WANG1, Mei DONG1, Min GUO2, Yang ZHAO3, Zhiyong
ZHUO3, Chao ZHANG3, Xiumei CHI4, Yu PAN4, Jing JIANG4, Hong TANG2, Junqi
NIU4, Dongliang YANG5, Zhong LI1, Xiao HAN1, Qian WANG1* and Xinwen Chen2
1 Jiangsu Province Key Lab of Human Functional Genomics, Department of
Biochemistry and Molecular Biology, Nanjing Medical University, Nanjing, 210029,
China
2 State Key Lab of Virology, Wuhan Institute of Virology, Chinese Academy of
Sciences, Wuhan, 430071, China
3 Key Laboratory of Infection and Immunity, Institute of Biophysics, Chinese
Academy of Sciences, Beijing, 100101, China
4 Department of Hepatology, The First Hospital of Jilin University, Changchun,
130021, China
5 Department of Infectious Diseases, Union Hospital, Tongji Medical College,
Huazhong University of Science and Technology, Wuhan, 430074, China
1
Diabetes Publish Ahead of Print, published online September 29, 2015 Diabetes Page 2 of 53
*Correspondence:
Qian WANG, Ph.D.
Jiangsu Province Key Lab of Human Functional Genomics
Department of Biochemistry and Molecular Biology
Nanjing Medical University
Nanjing 210029, China
E mail: [email protected]
Fax: +86 25 8362 1065
Tel: +86 25 8686 2729
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ABSTRACT
Class IIa histone deacetylases (HDACs), such as HDAC4, HDAC5, and HDAC7
provide critical mechanisms for regulating glucose homeostasis. Here we report
HDAC9, another class IIa HDAC, regulates hepatic gluconeogenesis via
deacetylation of a Forkhead box O (FoxO) family transcription factor, FoxO1,
together with HDAC3. Specifically, HDAC9 expression can be strongly induced upon
hepatitis C virus (HCV) infection. HCV induced HDAC9 upregulation enhances
gluconeogenesis by promoting the expression of gluconeogenic genes, including
phosphoenolpyruvate carboxykinase and glucose 6 phosphatase, indicating a major
role for HDAC9 in the development of HCV associated exaggerated gluconeogenic
responses. Moreover, HDAC9 expression levels and gluconeogenic activities were
elevated in livers from HCV infected patients and persistent HCV infected mice,
emphasizing the clinical relevance of these results. Our results suggest HDAC9 is
involved in glucose metabolism and HCV induced abnormal glucose homeostasis and
type 2 diabetes.
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INTRODUCTION
Hepatitis C virus (HCV) infection is the leading cause of viral hepatitis, which may lead to chronic hepatitis in up to 60–80% of infected adults and can progress to liver fibrosis, cirrhosis, and eventually hepatocellular carcinoma (1; 2). In addition, HCV infection may cause a variety of clinical extrahepatic manifestations (3). It is now widely recognized that chronic HCV infection is a metabolic disease that is associated with the subsequent development of hyperglycemia and type 2 diabetes (T2DM) (4).
The association between HCV and T2DM was recognized over 30 years ago (5).
Since then, many observational studies assessing the association between HCV and
T2DM have been published, which have provided mixed results. However, meta analyses have demonstrated that HCV infection can promote the increased prevalence of T2DM (6). It is generally accepted that glucose intolerance is more prevalent in chronic hepatitis associated with HCV infection than in other chronic liver diseases, including hepatitis B infection (7). HCV infection per se is associated with insulin resistance in the target pathways of endogenous glucose production and total body glucose disposal (8). Thus, chronic HCV infection may directly predispose the host to abnormal glucose metabolism and is thus considered as a risk factor for developing T2DM. However, the precise mechanisms underlying T2DM manifestation are poorly understood.
Glucose homeostasis is maintained physiologically through a balance between
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glucose production by the liver and glucose utilization by the peripheral tissues, via
the gluconeogenic and glycolytic pathways, respectively. Gluconeogenesis is largely
controlled at the transcriptional level by rate limiting enzymes such as
phosphoenolpyruvate carboxykinase (PEPCK) and glucose 6 phosphatase (G6PC).
Expression of these enzymes is controlled by the hormonal modulation of
transcription factors and coactivators, including Forkhead box O (FoxO) proteins (9).
The insulin signaling pathway is a major pathway responsible for suppressing
gluconeogenic transcription. Insulin dependent control of gluconeogenesis is largely
mediated through Akt, which phosphorylates and inactivates FoxO transcription
factors (mainly FoxO1 and FoxO3) in mammalian livers (10). Recent studies indicate
that HCV promotes hepatic gluconeogenesis through a phospho FoxO1 dependent
pathway (11; 12). However, in addition to phosphorylation dependent regulation,
FoxO activity is also modulated through acetylation by histone acetyltransferase
(HAT) enzymes, such as p300. Acetylation of FoxO transcription factors occurs in
response to oxidative stress or DNA binding, and can be reversed by the action of
deacetylases (13).
Four families of deacetylases counteract the activity of HATs: class I (HDAC1, 2, 3,
and 8) and II histone deacetylases (HDACs), class III NAD+ dependent HDACs
known as sirtuins (SIRTs; SIRT1–7), and HDAC 11, the sole class IV HDAC (14).
Class II HDACs are further subdivided into IIa (HDAC4, 5, 7, and 9) and IIb
(HDAC6 and 10) subfamilies. Among the HDACs, HDAC3 and SIRT1 are
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well known regulators of fatty acid and glucose metabolism (15; 16). Recent studies indicate that class IIa HDACs (HDAC4, 5, and 7) are hormone activated regulators of
FoxO and mammalian glucose homeostasis, especially gluconeogenesis (17). It is of great interest and importance to understand the biology of other HDACs in glucose homeostasis regulation and whether HDACs influence glucose metabolism abnormality in HCV infected hepatocytes.
Here, we report HDAC9 regulates hepatic gluconeogenesis via deacetylation of
FoxO1 and HCV induced HDAC9 upregulation caused an exaggerated gluconeogenic response. Moreover, both persistent HCV infected transgenic mice and HCV infected patients exhibited upregulated HDAC9 in liver and induced gluconeogenic activity.
These findings provide a clue to the possible mechanisms underlying the development of HCV induced abnormal glucose homeostasis and T2DM.
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RESEARCH DESIGN AND METHODS
Patients and biopsies
Human liver tissue samples from fine needle biopsies were obtained from
HCV infected patients. Normal human liver tissue was obtained from either spare
donor tissue intended for transplantation or from normal liver tissue resected from
patients with benign hepatic tumours. All human tissue samples were collected from
the Liver Unit of the First Hospital of Jilin University and TongJi Hospital, TongJi
Medical College of Huazhong University of Science and Technology with local
research ethics committee approval and informed patient consent. Diagnosis of
chronic HCV infection patients and analysis of all biopsies were based on standard
serological assays and the presence of abnormal serum aminotransferase levels for at
least six months. All HCV patients tested positive for HCV antibody based on a
third generation ELISA test. HCV infection was confirmed by detection of circulating
HCV RNA using HCV PCR based assay (Qiagen). At time of biopsy, liver tissue
(2–3 mm) was immediately frozen in Trizol and stored at 80°C. Fasting glucose and
insulin were measured on the days of biopsy. Insulin resistance was assessed by the
HOMA IR score (homeostasis model assessment, calculated as (fasting insulin ×
fasting glucose)/22.5).
Cells and virus
Human hepatoma cell lines HuH7.5.1 (kindly provided by Frank Chisari) were
cultured as described (18). HuH7.5.1 H77 cells (H77, genotype 1a), HuH7.5.1 Con1
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cells (CON1, genotype 1b), and HuH7.5.1 SGR JFH 1 cells (SGR, genotype 2a), which harbour the subgenomic HCV replicon, were derived from HuH7.5.1 cells and maintained in the same medium as HuH7.5.1 cells supplemented with 0.5 mg/ml
G418 (Gibco). Primary hepatocytes (PHT) cells isolated from C/OTg mice were performed as described (19). The HCV J399EM strain was derived from the JFH 1 virus by insertion of enhanced green fluorescent protein (EGFP) into the HCV NS5A region (20). Virus production and infection was performed as described (21).
Mock infected control was performed in parallel to virus infections, but in the absence of virus. For infection in vitro, PHTTg or HuH7.5.1 cells (1 x 106) were infected with J399EM for the indicated time with indicated multiplicities of infection
(MOI).
Real-time PCR and western blot analysis
RNA isolation, cDNA synthesis, quantitative PCR with indicated primers
(Supplementary Table. 1), and Western blotting were performed as described (21).
The NS5A antibody was a gift from Pro. Rice. All other antibodies were purchased from Abcam (HDAC9, ab18970), Santa Cruz Biotechnology (Acetyl FoxO1, sc49437, phospho FoxO1 (Ser256), sc16307 and ACTIN, sc1616) or Cell Signaling
Technology (FoxO1, 9454, HDAC3, 3949, PEPCK, 12940, GAPDH, 2118).
RNA interference
For knockdown experiments, 50 pmol small interfering RNA (siRNA) specific for
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HDAC9 and negative control (Qiagen, Supplementary Table 1) were transfected into
HuH7.5.1 or SGR cells via the Lipofectamine 2000 (Invitrogen).
Glucose production assay
The production of glucose was measured using an Amplex® Red Glucose/Glucose
oxidase assay kit (Invitrogen) according to the manufacturer’s instructions.
Co-immunoprecipitation and immunofluorescence assay
Co immunoprecipitation and immunofluorescence assay were performed as described
(21).
PEPCK activity assay
PEPCK enzyme activity was assayed using an NADH coupled system as described
(22) .
Transgenic Mice and Animal study design
The transgenic C/OTg mice harboring both human CD81 and OCLN genes were
constructed as described (19). We used 8 12 weeks of age and gender matched mice
for in vivo experiments. The information of HCV infected (n = 36) and mock infected
(n = 12) C/OTg mice raised in synchronization were listed in Supplementary Table 2,
and more information were shown previously (19). The animal studies were approved
by the Institutional Animal Care and Use Committee of Nanjing Medical University.
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Metabolic studies
Glucose and insulin tolerance tests were performed by intraperitoneal injection of mice with glucose (2.0 g/kg), insulin (0.5 U/kg), or pyruvate (2.0 g/kg) according to methods described previously (23). FLEXMAP 3D quantification (Luminex, TX) of concentrations of insulin and C peptide were performed.
Statistical analysis
Data are presented as means ± SEM. Statistical analysis was carried out using
Student’s t test when comparing two groups and ANOVA when comparing multiple groups. Differences were considered significant at P < 0.05 (*, p < 0.05; **, p < 0.01).
Statistical analyses were performed using GraphPad Prism.
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RESULTS
Upregulated HDAC9 and PEPCK expression in liver biopsies from
HCV-infected patients
Previous studies suggest that the class IIa HDAC4, HDAC5, and HDAC7 proteins
play a central role in metabolic homeostasis. A comparison of the transcriptomes of
HCV infected and mock infected HuH7.5.1 cells revealed that HDAC9 expression
was enhanced by 16.25 fold in JFH 1 infected cells, whereas among the other
HDACs, only SIRT1 and HDAC5 expression levels were increased 2.25 and 2.03 fold,
respectively (data not shown). To confirm the results, we examined HDAC9
expression in liver biopsy samples from HCV infected patients. The demographic and
clinicopathological characteristics of 38 biopsies obtained from HCV infected
patients and 10 biopsies from normal control patients included in the study are shown
in supplementary Table 3. We observed a statistically significant elevation of HDAC9
expression in liver biopsies from HCV infected patients (Fig. 1A and B). In the group
of 38 HCV infected patients, HDAC9 mRNA expression levels were positively
associated with HCV viral loads in the liver (Fig. 1C), but not in the serum (data not
shown). PEPCK mRNA levels were also found to be elevated in HCV infected
patients (Fig. 1D). Remarkably, PEPCK enzymatic activity in samples from
HCV infected patients was 3 to 4 fold higher than in parallel samples from normal
control patients (Fig. 1E). In HCV infected subjects, the degree of HDAC9 and
PEPCK gene induction appeared to be positively correlated (Fig. 1F). Further, we
compared the induction of HDAC9 with PEPCK enzymatic activities, and again, a
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significant positive correlation was observed (Fig. 1G). To determine if the HDAC9 overexpression observed in patients infected with HCV correlated with systemic insulin resistance, we measured fasting glucose and insulin levels on the day of the liver biopsy. A positive correlation was found in 38 subjects between the induction of
HDAC9 and their HOMA IR values (Fig. 1H).
HCV infection upregulates host HDAC9 expression in an HCV-dependent manner
We further analyse our clinical findings in vitro. As shown in Fig. 2A, HDAC9 expression is upregulated in time and dose dependent manners following HCV infection, in parallel with increasing HCV RNA levels. Similar HDAC9 upregulation was observed at the protein level (Fig. 2B, Supplementary Fig. 1C and 2A). Moreover, the expression levels of the other HDACs, including HDAC1 7 and SIRT1, were not upregulated (Supplementary Fig. 1). HDAC9 mRNA and protein levels were also increased in H77 cells, CON1 cells, and SGR cells (Fig. 2C and D), which harbor the
HCV 1a, HCV 1b, and HCV 2a subgenomic replicons, respectively, indicating that
HCV dependent HDAC9 upregulation was not genotype specific.
To determine whether the observed HDAC9 induction was HCV dependent,
HCV infected cells were treated with 2mAde (an HCV inhibitor that targets the viral
NS5B protein). As shown in Fig. 2E and F, 2mAde treatment dramatically decreased
HCV levels and HDAC9 upregulation in HCV infected cells, whereas HDAC9
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expression levels in control cells were not affected. Similar results were observed in
HCV replicon cells (Supplementary Fig. 2B and C). Transfection with siHCV, a small
interfering RNA (siRNA) targeting HCV, reduced HDAC9 expression by 80% and
intracellular HCV RNA levels by ~90% (Fig. 2G), consistent with the fact that HCV
infection stimulates HDAC9 expression. Interestingly, HCV infected cells transfected
with siRNAs targeting the HDAC9 sequence (siHDAC9 2~5) decreased both HDAC9
and HCV RNA expression levels (Fig. 2G). siHDAC9 1 did not reduce either the
expression of HDAC9 or HCV RNA levels. Two combinations of siRNAs
(siHDAC9 2+3+4 and siHDAC9 2+4+5) significantly decreased HDAC9 expression
levels to ~30% or 40% of the control level in HCV infected cells (Fig. 2G),
respectively, in agreement with the effect in HuH7.5.1 cells (Supplementary Fig. 2D
and E). These siRNA combinations also reduced HCV RNA levels to 14% or 15%,
respectively, as also suggested by comparable downregulation of the NS3 proteins
(Fig. 2H). Transfection with HDAC9 siRNAs exerted similar effects in HCV replicon
cells (Supplementary Fig. 2F and G). Downregulation of the NS3 proteins was also
observed in HCV infected HDAC9 shRNA cells (Supplementary Fig. 4A).
Furthermore, the small molecule HDAC inhibitors sodium butyrate (NaB) and
trichostatin A (TSA) significantly decreased HCV RNA and NS3 protein levels
(Supplementary Fig. 2H and I), without affecting the viability of HuH7.5.1 cells (data
not shown). These results suggest that, while HCV infection can upregulate HDAC9
expression in an HCV dependent manner, HDAC9 silencing can also inhibit HCV
replication.
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HDAC9 mediates HCV-dependent gluconeogenesis
Recent studies indicate that HCV promotes hepatic gluconeogenesis (12). In agreement, we found that PEPCK mRNA and protein levels were increased in a time and dose dependent manner following HCV infection (Fig. 3A, B and Supplementary
Fig. 3A). In addition, HCV infection induced the expression of another rate limiting enzyme, G6PC (Supplementary Fig. 3B). 2mAde treatment blocked PEPCK (Fig. 3C) and G6PC (Supplementary Fig. 3C) elevation in HCV infected cells, confirming its dependency on the presence of HCV, similar to the effects observed in SGR cells
(Supplementary Fig. 3D). To assess the physiological relevance of HDAC9 and key gluconeogenic enzyme upregulation by HCV infection, we assayed for cellular glucose production, which reflects endogenous gluconeogenesis. The results showed that HCV infection caused elevated glucose production, relative to the mock infected control (Fig. 3D). In contrast, 2mAde treatment in HCV infected cells (Fig. 3D) or
SGR cells (Supplementary Fig. 3E) significantly abrogated the increase in glucose production, suggesting that the elevation in gluconeogenesis was HCV dependent.
Class IIa HDACs are hormone activated regulators of glucose homeostasis, especially gluconeogenesis. We next investigated whether the induction of gluconeogenic enzymes was HDAC9 dependent. Treatment with TSA and NaB reduced PEPCK (Fig.
3C) and G6PC (Supplementary Fig. 3C) mRNA levels relative to the control in mock and HCV infected cells. HDAC9 silencing significantly attenuated PEPCK (Fig. 3E, F
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and Supplementary Fig. 4A) and G6PC (Supplementary Fig. 3F) expression in
HuH7.5.1 cells excluding the function of other HDACs. Furthermore, HDAC9
depletion also resulted in a marked decrease of HCV induced PEPCK expression in
both HCV infected cells (Fig. 3E, F and Supplementary Fig. 4A) and SGR cells
(Supplementary Fig. 3G), similar to the effect on G6PC expression (Supplementary
Fig. 3F). Consistently, glucose production in HuH7.5.1 cells, HCV infected cells, and
SGR cells was dramatically reduced compared to the control following HDAC9
knockdown (Fig. 3G, Supplementary Fig. 3H and I) or treatment with HDAC
inhibitors NaB and TSA (Fig. 3D).
Taken together, these results demonstrate that HDAC9 plays roles in regulating
gluconeogenesis in hepatic cells and in HCV promoted gluconeogenesis.
Involvement of HDAC9-dependent FoxO1 acetylation in HCV-induced
gluconeogenesis
The FoxO1 transcription factor stimulates PEPCK and G6PC expression by binding
directly to their promoters. This binding is controlled by various post translational
modifications, including phosphorylation, ubiquitylation, and acetylation. We
examined whether HDAC9 influences the acetylation of FoxO1.
Immunoblot analysis revealed that FoxO1 acetylation was dramatically decreased in
HCV infected cells compared with the mock infected control, whereas total FoxO1
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protein levels were comparable (Fig. 4A). Conversely, treatment of HCV infected cells with 2mAde restored FoxO1 acetylation to approximately the same level as seen in mock infected cells (Fig. 4A). In addition, HDAC9 depletion led to increased acetylation of endogenous FoxO1 in both HuH7.5.1 (Fig. 4B) and HCV infected cells
(Fig. 4C and Supplementary Fig. 4A). In a parallel experiment, HCV replicon cells exhibited similar result following 2mAde treatment or HDAC9 knockdown
(Supplementary Fig. 4B and C).
We further tested whether HDAC9 and FoxO1 are physically associated. HDAC9 co immunoprecipitated with both the acetylated and non acetylated forms of FoxO1 in both mock and HCV infected cells (Fig. 4D, second and third panel). It has been reported that class IIa HDACs are catalytically inactive and exhibit activity only when associated with the catalytically active class I HDAC family member HDAC3 (17;
24). Consistent with these observations, endogenous HDAC9 co immunoprecipitated with HDAC3 (Fig. 4D, second and forth panel). Of note, HCV infection greatly enhanced the association between endogenous FoxO1 and HDAC3, suggesting that
HDAC9 upregulation stabilizes complex formation between HDAC9, FoxO1, and
HDAC3 (Fig. 4D, third and forth panel).
Data from a previous study showed that HCV infection in human hepatocytes can impair insulin induced FoxO1 translocation from the nucleus to the cytoplasm (25).
We tested whether HDAC9 is involved in HCV promoted FoxO1 nuclear
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accumulation. Mock infected HuH7.5.1 cells were treated similarly for comparison
purposes (Fig. 4E and Supplementary Fig. 4D). Consistent with the decreased levels
of endogenous FoxO1 acetylation observed in HCV infected cells, most HCV infected
cells displayed nuclear FoxO1 localization, whereas treatment with 2mAde induced
FoxO1 translocation to the cytoplasm (Fig. 4E). HDAC9 knockdown increased
endogenous FoxO1 acetylation (Fig. 4C), which was excluded from the nuclei in
these cells (Fig. 4E and Supplementary Fig. 4E). Similar results were observed
following NaB and TSA treatment (Fig. 4E). A cell fractionation study further
indicated that HDAC9 depletion reduced nuclear FoxO1 in HCV infected cells, and
the acetylation form of FoxO1 was significantly reduced in both cytoplasmic and
nuclear fractions (Fig. 4C). Moreover, HDAC9 accumulated in the nuclear fraction in
both mock and HCV infected cells (Fig. 4C and E).
Taken together, these results suggest that HDAC9 can control FoxO1 acetylation in
hepatocytes and that HCV induced nuclear HDAC9 upregulation suppressed FoxO1
acetylation, leading to the nuclear accumulation of FoxO1.
Exaggerated gluconeogenic response via HDAC9 upregulation in persistent
HCV-infected mice
We further demonstrated the relevance of our clinical and in vitro findings in
transgenic ICR mice (C/OTg) that specifically expressed human CD81 and OCLN in
their hepatocytes. The same cohort of transgenic mice, which can support persistent
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infection by HCV particles derived from either cell cultures or chronically infected patients, was described previously (19). Elevated fasting plasma glucose (FPG) levels were observed in chronically HCV infected C/OTg mice during the 10 months post infection (mpi) period, compared with mock infected control mice
(supplementary Table 2). Administration of glucose to HCV infected transgenic mice revealed a significant impairment of glucose tolerance at 1 mpi, compared with control mice of the same age (Fig. 5A). The insulin tolerance test conducted at 1 mpi revealed that the reduction in plasma glucose concentrations after intraperitoneal (IP) insulin administration was impaired in chronic HCV infected C/OTg mice, which displayed higher plasma glucose levels than did control mice at all time points measured (Fig. 5B). Accordingly, the homeostatic model assessment insulin resistance (HOMA IR) values, a measure of systemic insulin resistance, were also elevated in HCV infected mice compared to controls (Supplementary Table 2).
We then determined the effect of HCV infection on gluconeogenesis in vivo by examining blood glucose levels in mice following IP injection of pyruvate, a major gluconeogenic substrate. HCV infection induced pyruvate tolerance in C/OTg mice, as represented by a significant elevation in the area under the curve (AUC; Fig. 5C), suggestive of an increased hepatic glucose output in HCV infected C/OTg mice.
Furthermore, PEPCK enzymatic activities in liver samples of C/OTg mice were significant increased over time following HCV infection for over 10 months (Fig.
5D).
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HDAC9 expression levels were analyzed to assess the correlation between HDAC9
expression and glucose homeostasis abnormality in HCV infected mice. In contrast to
mock infected mice, HDAC9 expression at both mRNA and protein levels increased
continuously during the 10 mpi period in chronical HCV infected C/OTg mice (Fig. 5E,
F and Supplementary Fig. 5). This result was confirmed by in vitro studies showing
that infection of primary hepatocytes isolated from C/OTg mice with HCV induced
HDAC9 expression (Fig. 5G and H). Consistent with the in vitro findings, FoxO1
acetylation and phosphorylation dramatically decreased in both HCV infected C/OTg
mice (Fig. 5F) and primary hepatocytes (Fig. 5H) compared with the controls,
whereas total FoxO1 protein levels were comparable.
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DISCUSSION
HDACs regulate acetylation of histones and transcriptional factors involved in glucose homeostasis and play a central role in the regulation of glucose metabolism
(26). In this study, we demonstrated that HDAC9, a class IIa HDAC, is involved in gluconeogenesis in liver via deacetylation of the FoxO1 transcription factor together with HDAC3. In particular, HDAC9 can be strongly induced upon stimulation, such as HCV infection. HDAC9 upregulation induced by HCV infection promoted the expression of gluconeogenic genes such as PEPCK and enhanced gluconeogenesis.
These results suggest a plausible molecular mechanism for HCV induced abnormal glucose homeostasis and T2DM.
Previous studies showed that class IIa HDACs such as HDAC4, 5, and 7 regulate
FoxO and glucose homeostasis responses to fasting hormone glucagon in the liver
(17). Glucagon induced dephosphorylation of HDAC4, 5, and 7 results in the nuclear translocation and deacetylation of FoxO, enhancing its association with gluconeogenic gene promoters. We found that HDAC9 showed a predominant nuclear localization in hepatocytes. Within the nuclei, HDAC9 may act as a scaffold to recruit
HDAC3, similar to its mode of action in regulatory T cells (27). The resulting catalytically active HDAC complex can deacetylate nuclear FoxO1, leading to the acute transcriptional induction of gluconeogenic enzymes. HDAC9 suppression in hepatocytes results in the inhibition of gluconeogenic genes and gluconeogenesis.
These results indicate HDAC9 may regulate glucose homeostasis under normal
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physiological conditions. Unlike other class IIa HDACs that are regulated by
post translational modification responses to fasting in liver (17), HDAC9 regulates
gluconeogenesis specifically via eliciting gene expression level changes. HCV
infection only significantly upregulated the expression of HDAC9, but not other
HDACs, suggesting that class IIa HDACs may be induced via different mechanisms.
It is of interest to identify the stimulus for HDAC9 induction under physiological
conditions and to investigate the mechanism whereby HDAC9 responds to a given
stimulus to maintain normal glucose homeostasis. Knockdown of HDAC9 expression
in vivo completely protected mice from the consequences of high fat feeding,
including elevated blood sugar, cholesterol levels, and fatty liver disease (28). Thus,
HDAC9 may play a role in regulating gluconeogenesis and glucose homeostasis
during high fat feeding.
It has been reported that increased oxidative stress may be an initial key event that
triggers high fat diet induced insulin resistance (29; 30). Hepatic oxidative stress is a
prominent feature of chronic HCV infection, and oxidative stress upregulates HDAC
activity (31; 32). We found that HCV induced oxidative stress increased HDAC9
expression, whereas the antioxidant N acetyl L cysteine restored HDAC9 expression
in HCV infected cells (Supplementary Fig. 6A and B) and HCV replicon cells
(Supplementary Fig. 6D and E). However, while antioxidant treatment markedly
reduced glucose production and gluconeogenesis following HCV infection
(Supplementary Fig. 6C and F), its effect on gluconeogenesis was weaker than that of
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an HDAC9 siRNA or a HDAC inhibitor, suggesting that HDAC expression is regulated by other factors in addition to reactive oxygen species. However, the individual expression of each HCV protein could not enhance HDAC9 expression
(data not shown). HCV replication is associated with the endoplasmic reticulum (ER), where the virus causes stress. It is reported that ER stress is emerging as a potential contributor to the onset of type 2 diabetes by making cells insulin resistant.
Understanding the role of ER stress that HCV exerts will provide insight. Moreover, as the best characterized 14 3 3 target chromatin modifying enzymes are class IIa
HDACs (33; 34), it will be interesting to determine whether HCV also regulates
HDAC regulators, such as the 14 3 3 proteins.
FoxO1 regulates multiple metabolic pathways in the liver, including gluconeogenesis, glycolysis, and lipogenesis (9). HCV infection may promote FoxO1 activation by a
2 pronged mechanism, wherein diminished insulin signaling results in dephosphorylation of the Akt sites in FoxO1, allowing its re entry into the nucleus (12;
25). In addition, HCV induced expression of HDAC9 may cause deacetylation of nuclear FoxO1, enhancing FoxO1 DNA binding activity and association with gluconeogenic gene promoters, thereby enhancing the transcription of rate controlling gluconeogenic enzymes. HDAC9 knockdown in both hepatic cells and HCV replicon cells resulted in increased acetylation and phosphorylation of endogenous FoxO1 (Fig.
4B and Supplementary Fig. 4C). These results support the observation that FoxO acetylation renders FoxO phosphorylation sites more accessible to Akt and other
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inactivating kinases (35). Our findings therefore suggest a mechanism by which
aberrant HDAC9 induction may contribute to the development of HCV induced
glucose homeostasis abnormality.
Our recent study showed that transgenic ICR mice expressing both the human CD81
and occludin genes (C/OTg) are permissive to HCV infection (19). Persistent HCV
infection in this mice model further exhibited disease manifestations, including
chronic viral hepatitis, steatosis, and fibrosis. Herein, we report that persistent
hepatitis C virus infection in this model also resulted in insulin resistance and
hyperglycemia, as reported in HCV infected chronic patients (Supplementary Table 2
and 3). Furthermore, both HDAC9 expression levels and gluconeogenic activity were
elevated in liver tissues from chronic HCV infected rodent models and HCV infected
patients. Thus, HCV infection may lead to abnormal glucose homeostasis through
HDAC9 upregulation which results in deacetylation of nuclear FoxO1, enhancement
of FoxO1 DNA binding activity and association with gluconeogenic gene promoters,
and finally increased hepatic gluconeogenesis. This potential mechanism indicates
that HDAC9 may be potential therapeutic targets for suppressing hepatic
gluconeogenesis and lowering blood glucose, and small molecule inhibitors of class
I/IIa HDACs may be useful as HCV associated T2DM therapeutics. Currently, several
pan HDAC inhibitors are in phase I–III clinical trials. Vorinostat, the first HDAC
inhibitor developed, has already been approved for treatment of a malignant disease
(36; 37). The potential utility of HDAC inhibitors for treating metabolic disease
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therefore merits consideration.
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ACKNOWLEDGEMENTS
We are grateful to Drs T Wakita (National Institute of Infectious Diseases, Japan) for
pJFH 1 clone, F Chisari (The Scripps Research Institute) for HuH7.5.1 cell line, and
C Rice (The Rockefeller University) for NS5A antibody. This work was supported by
grants from the National Natural Sciences Foundation of China [grant number
81271828, 31101011, 31271268], the National Basic Research Program of China
[grant number 2015CB554304], and a Project Funded by the Priority Academic
Program Development of Jiangsu Higher Education. The authors who have taken part
in this study declared that they do not have anything to disclose regarding funding or
conflict of interest with respect to this manuscript.
The authors who have taken part in this study declared that they do not have anything
to disclose regarding funding or conflict of interest with respect to this manuscript.
The study was designed by Q.W. and JZ.C.; Experiments in HCV infected cells were
performed by JZ.C., M.D. and M.G.. Experiments in replicon cells were performed by
Q.W. and N.W.. Patients’ studies were performed by JZ.C., XM.C, Y.P., J.J..
Transgenic mice and animal study was performed by JZ.C., Z.Y., ZY.Z, C.Z.
Experimental analysis was performed by Q.W., XW.C., JZ.C., Z.L., X.H., H.T., DL.
Y., and JQ. N.; and the manuscript was written by Q.W.. Q.W. is the guarantor of this
work and, as such, had full access to all the data in the study and takes responsibility
for the integrity of the data and the accuracy of the data analysis.
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FIGURE LEGENDS
Figure 1. HDAC9 expression and PEPCK enzymatic activity is upregulated in liver biopsies from HCV-infected patients. Box plot diagram showing the HDAC9 mRNA (A), PEPCK mRNA (D) levels and PEPCK enzymatic activity (E) in liver biopsies of 10 normal control patients and 38 patients with chronic hepatitis C.
Representative example of a western blot of HDAC9 showing samples of liver biopsy homogenate from normal control and HCV patients (B). Positive correlation between
HDAC9 mRNA levels in liver and PEPCK mRNA levels in liver (C), HCV virus load in liver (F), PEPCK enzymatic activity in liver (G), or HOMA IR score (H). Data are represented as mean ± SEM.
Figure 2. HCV infection upregulates host HDAC9 expression. HCV RNA,
HDAC9 mRNA (A), and HDAC9 protein (B) levels in mock or
HCV infected HuH7.5.1 cells at indicated multiplicities of infection (MOI) and time points (Hours post infection, hpi). HCV RNA, HDAC9 mRNA (C), and HDAC9 protein (D) levels in H77, CON1, and SGR cells, compared with HuH7.5.1 control cells. HCV RNA and relative intracellular HDAC9 mRNA (E) and HDAC9 protein levels (F) in mock or HCV infected (1.0 MOI) cells treated with 2mAde (10 mM, 96 h). HCV RNA and relative intracellular HDAC9 mRNA levels (G) and HDAC9 protein levels (H) in mock or HCV infected (1.0 MOI) cells pretransfected with
HDAC9 siRNAs for 48 h at 96 hpi. Data are represented as mean ± SEM. # indicates undetectable levels. *p<0.05; **p<0.001.
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Figure 3. HDAC9 mediates HCV-dependent gluconeogenesis. Relative
intracellular PEPCK mRNA (A) and protein (B) levels in mock or
HCV infected HuH7.5.1 cells at indicated MOI and time points. Relative intracellular
PEPCK mRNA levels (C) and cellular glucose production (D) in mock or HCV
J399EM infected HuH7.5.1 cells treated with 2mAde (10 mM, 96 h), NaB (10 mM,
72 h), or TSA (400 nM, 24 h), respectively. Relative intracellular PEPCK mRNA
levels (E), protein levels (F), and cellular glucose production (G) as in Figure 2G.
Data are represented as mean ± SEM. *p<0.05; **p<0.001.
Figure 4. HDAC9-dependent FoxO1 acetylation is involved in HCV-induced
gluconeogenesis. FoxO1 and acetyl FoxO1 (Ac FoxO1) protein levels in mock or
HCV J399EM infected (1.0 MOI) HuH7.5.1 cells treated with 2mAde (10 mM) for
96 h (A). HDAC9, FoxO1, Ac FoxO1, and phospho FoxO1 (P FoxO1, Ser256)
protein levels in HuH7.5.1 cells transfected with HDAC9 siRNAs (B). HDAC9,
FoxO1, Ac FoxO1, and HDAC3 protein levels in whole cell lysate (WCL) or
cytoplasmic and nuclear fractions from mock or HCV infected (1.0 MOI) cells
pretransfected with combination of siHDAC9 2 + 3 + 4 for 48 h at 96 hpi (C). (D)
Endogenous HDAC9 (second panel), FoxO1 (third panel), or HDAC3 (forth panel)
was immunoprecipitated from mock or HCV J399EM (1.0 MOI) infected cell lysates,
and immunoblotted with indicated antibodies. The whole cell lysate for
immunoprecipitation was trisected and immunoblotted with indicated antibodies (first
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panel). Goat anti rabbit IgG or Rabbit anti mouse was used as the negative control.
(G) Endogenous FoxO1 protein was detected by immunofluorescence in mock or
HCV J399EM infected (1.0 MOI) HuH7.5.1 cells treated with 2mAde, NaB, TSA, or
HDAC9 siRNA, repectively. Scale bars: 10 µm.
Figure 5. HDAC9 upregulation induced exaggerated gluconeogenic response in persistent HCV-infected mice. Male and female chronic HCV infected C/OTg mice
(1 mpi) and mock infected mice were fasted overnight. Blood glucose was monitored following intraperitoneal administration of glucose (2.0 g/kg, A), insulin (0.5 U/kg, B), or pyruvate (2.0 g/kg, C). Total AUC is expressed as mean SEM relative to average mock infected control values. (n=6–12) (D) PEPCK enzymatic activity in liver after
C/OTg mice infected with HCV J399EM for the indicated time. Mock infected C/OTg control mice were collected from different time post infection at random. (n=3–7). (E)
Intracellular HDAC9 mRNA levels in liver of C/OTg mice mock infected or infected with HCV J399EM for the indicated time. (n=3–6). (F) HDAC9, FoxO1, and
Ac FoxO1 protein levels as in Figure 5D. The data shown are representative of three independent experiments. Line charts below represent densitometric analysis performed to quantify the relative intensity of HDAC9 , Ac FoxO1/FoxO1 immunoreactive bands detected by western immunoblotting. HCV RNA and intracellular HDAC9 mRNA levels (G) and HDAC9, FoxO1, Ac FoxO1, and
P FoxO1 (Ser256) protein levels (H) in HCV (1.0 MOI) infected C/OTg primary hepatocytes at indicated times. Data are represented as mean ± SEM. *p<0.05;
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**p<0.001.
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Supplementary Figures
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Supplementary Figure 1. HCV infection upregulates host HDAC9 expression.
HCV RNA (A), and HDAC1, HDAC2, HDAC3, HDAC4, HDAC5, HDAC7,
HDAC9, HDAC11, and SIRT1 mRNA (B) and HDAC1, HDAC2, HDAC3, HDAC4,
HDAC5, HDAC6, HDAC7, HDAC9, and SIRT1 protein (C) levels in mock- or
HCV-infected-HuH7.5.1 cells at indicated multiplicities of infection (MOI) and time points (Hours post infection, hpi). All antibodies were purchased from Cell Signaling
Technology (HDAC1, HDAC2, HDAC3, HDAC6, 9928; SIRT1, 8469) or Abcam
(HDAC4, ab12172, HDAC5, ab1439, HDAC7, ab12174). Data are represented as mean ± SEM. *p<0.05; **p<0.001. NS indicates no significant difference.
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Supplementary Figure 2. HCV infection upregulates host HDAC9 expression. (A)
HDAC9 protein levels in HCV J399EM-infected (0.01 and 0.1 MOI) or mock-infected HuH7.5.1 cells at indicated time points (Hours post infection, hpi).
(B-C) HCV RNA, relative intracellular HDAC9 mRNA (B), HDAC9 protein, and
NS3 protein (C) levels in HuH7.5.1 and SGR cells treated with 2mAde (10 mM, 96 h).
(D-E) Relative intracellular HDAC9 mRNA levels (D) and HDAC9 protein levels (E) in HuH7.5.1 cells transfected with HDAC9 siRNA for 48 h. (F-G) Relative intracellular HDAC9 mRNA (F) and HDAC9 protein levels (G) in HuH7.5.1 and SGR cells transfected with specific HDAC9 siRNA for 48 h. (H-I) HCV J399EM-infected
(0.1 MOI) or mock-infected HuH7.5.1 cells were treated with NaB (10 mM, 72 h),
TSA (400 nM, 24 h), respectively. HCV RNA (H) and NS3 protein (I) levels in cells.
Data are represented as mean ± SEM. # indicates undetectable levels. *p<0.05;
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Supplementary Figure 3. HDAC9 mediates HCV-dependent gluconeogenesis. (A)
PEPCK protein levels in HCV J399EM-infected or mock-infected HuH7.5.1 cells at the indicated MOI and time points (Hours post infection, hpi). (B) Relative intracellular G6PC mRNA levels in HCV J399EM-infected or mock-infected
HuH7.5.1 cells at the indicated MOI and time points. (C) Relative intracellular G6PC mRNA levels in HCV J399EM-infected or mock-infected HuH7.5.1 cells treated with
2mAde (10 mM, 96 h), NaB (10 mM, 72 h), TSA (400 nM, 24 h), respectively. (D-E)
PEPCK mRNA levels (D) and cellular glucose production normalized to total cellular protein content (E) in HuH7.5.1 and SGR cells treated with 2mAde. (F) HuH7.5.1 cells were pretransfected with siRNA for 48 h. Relative intracellular G6PC mRNA levels in mock-infected cells or cells infected with HCV J399EM (1.0 MOI) at 96 hpi.
(G-H) PEPCK mRNA levels (G) and cellular glucose production normalized to total cellular protein content (H) in HuH7.5.1 and SGR cells transfected with siHDAC9. (I)
Cellular glucose production normalized to total cellular protein content in mock or
HCV J399EM (1.0 MOI)-infected HDAC9 shRNA cells at 96 hpi. Data are represented as mean ± SEM. *p<0.05; **p<0.001. Page 47 of 53 Diabetes
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Supplementary Figure 4. HDAC9 controls acetylation of FoxO1. (A) HDAC9,
FoxO1, acetyl-FoxO1 (Ac-FoxO1), PEPCK, NS3 protein levels in mock infected-
(left panel), or HCV J399EM (1.0 MOI)-infected (right panel) HDAC9 shRNA cells at 96 hpi. (B) FoxO1 and acetyl-FoxO1 (Ac-FoxO1) protein levels in HuH7.5.1 and
SGR cells treated with 2mAde (10 mM) for 96 h. (C) FoxO1, Ac-FoxO1, phospho-FoxO1 (P-FoxO1), and NS3 protein levels in HuH7.5.1 and SGR cells transfected with siHDAC9. (D) Endogenous FoxO1, HDAC9, NS5A protein was detected by immunofluorescence in mock-infected HuH7.5.1 cells treated with NaB,
TSA, or siHDAC9, repectively. Scale bars: 10 µm. (E) Endogenous FoxO1, HDAC9,
NS5A protein was detected by immunofluorescence in HCV J399EM (1.0
MOI)-infected HDAC9 shRNA cells. Page 49 of 53 Diabetes
Supplementary Figure 5. HDAC9, FoxO1, and Ac-FoxO1 protein levels in liver of
mock-infected C/OTg mice for the indicated time. Histograms below represent
densitometric analysis performed to quantify the relative intensity of HDAC9-,
Ac-FoxO1/FoxO1-immunoreactive bands detected by western immunoblotting. Diabetes Page 50 of 53
Supplementary Figure 6. Oxidative stress contributes to HDAC9 induction and gluconeogenesis in HCV infected cells. (A-C) Levels of HCV RNA and HDAC9 mRNA (A), HDAC9 protein (B), and cellular glucose production (C) in HCV
J399EM-infected (1.0 MOI) or mock-infected HuH7.5.1 cells treated with or without
N-acetyl-L-cysteine (NAC). (D-F) Levels of HCV RNA and HDAC9 mRNA (D),
HDAC9 protein (E), and cellular glucose production (F) in HuH7.5.1 and SGR cells treated with or without NAC. Data are represented as mean ± SEM. *p<0.05;
**p<0.001. Page 51 of 53 Diabetes
Supplementary Tables
Supplementary Table 1. Primers and siRNA used in this study.
Strand/Gene Primer Sequence(5’-3’) HDAC9 (human) HDAC9F GCTGGTGGAGTTCCCTTACA HDAC9R GCAGACTGGGTTCGGTTCA PEPCK (human) PEPCKF TGAGATCAGAGGCCACAGC PEPCKR GCCAGGTATTTGCCGAAG FoxO1 (human) FOXO1F GAGGGTTAGTGAGCAGGTTAC FOXO1R AGTCCTTATCTACAGCAGCAC HCV (human) HCVF CCCTATCAGGCAGTACCACAAGG HCVR ACCTGCCCCTAATAGGGGCG Actin (human) ActinF GAAATCGTGCGTGACATTAA ActinR AAGGAAGGCTGGAAGAGTG G6PC (human) G6PCF CCTCAGGAATGCCTTCTACG G6PCR TCTCCAATCACAGCTACCCA hdac9 (mouse) HDAC9MF GCTGGTGGAGTTCCATTACA HDAC9MR GCAGACTGGGTTCGATTCA actin (mouse) ActinMF GAAATTGTTCGTGACATAAA ActinMR AAGGAAGGCTGGAAGAGTG siHDAC9-1 AAAGACACCCAACAAAATT siHDAC9-2 CAGCAACGCATTCTAATTCAT siHDAC9-3 CCAACTGGAAGTGTTACTGAA siHDAC9-4 TTGGCTCAGCTGGTCATTCAA siHDAC9-5 CAGCAACGAAAGACACTCCAA HCV siRNA GGUCUCGUAGACCGUGCAC
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Supplementary Table 2. Information pertaining to the mice used in Figure 5.
Blood Liver PEPCK Glucose Insulin C-peptide HOMA hdac9 Gender Age Timepoint IU/mL IU/mg (mU/mg (mmol/L) (mIU/L) (pg/ml) -IR (fold) (Log10) (Log10) protein) 1 F 7 w mock # # 4.2 8.05 1402.07 1.5 1.42 5.9 2 F 9 w mock # # 4.4 9.24 1306.41 1.81 1.29 4.2 3 F 11 w mock # # 5 8.34 1086.75 1.85 0.76 3.1 4 F 15w mock # # 4.7 9.68 963.72 2.02 1.12 6.7 5 F 42 w mock # # 4.9 11.86 1057.5 2.58 0.74 6.4 6 M 7 w mock # # 4.8 10.03 1017.06 2.14 1.01 7.1 7 M 9 w mock # # 5.2 10.2 1156.86 2.36 0.84 3.5 8 M 11 w mock # # 4.4 6.41 788.78 1.25 1.24 4.4 9 M 15 w mock # # 4.2 10.9 949.44 2.03 0.68 3.9 10 M 30 w mock # # 5.2 7.21 773.61 1.67 0.84 4.7 11 M 30 w mock # # 4.8 9.17 841.36 1.96 0.89 5.2 12 M 42 w mock # # 4 8.55 988.78 1.52 1.16 6.1 13 F 7 w 2d 6.53 4.94 5 8.98 543.86 2 4.01 14 F 7 w 2d 6.23 4.99 4 14.47 2304.18 2.57 3.16 15 M 7 w 2d 5.75 4.55 4.5 12.72 1901.19 2.54 1.29 16 M 7 w 2d 5.87 4.59 4.5 12.05 1367.92 2.41 4.07 17 F 7 w 4d 5.45 4.7 5.5 10.9 1098.91 2.66 1.84 18 F 7 w 4d 5.65 4.62 4.4 10.68 1255.34 2.09 0.24 19 M 7 w 4d 5.01 4.25 7 10.32 979.72 3.21 2.94 20 M 7 w 4d 4.9 4.16 7.2 13.77 1887.11 4.41 0.84 21 F 8 w 1w 5.11 4.3 4.4 8.05 1539.54 1.57 0.24 22 F 8 w 1w 5.08 4.15 5 9.24 1681.86 2.05 0.46 23 F 8 w 1w 4.29 4.7 8.34 1633.68 1.74 0.35 24 M 8 w 1w 3.89 4.11 4.9 9.68 1454.41 2.11 0.67 25 M 8 w 1w 3.5 5.08 4.8 11.86 2048.44 2.53 0.8 26 M 8 w 1w 5 5.1 12.04 1937.82 2.73 0.35 27 F 9 w 2w 4.79 3.78 5.4 8.72 1397.58 2.09 0.68 11 28 F 9 w 2w 4.82 3.63 4.9 12.34 1512.22 2.69 2.06 11.3 29 F 9 w 2w 3.78 4.8 6.88 990.93 1.47 0.15 6.6 30 M 9 w 2w 4.84 3.68 5.2 10.02 1233.72 2.31 0.68 9.4 31 M 9 w 2w 4.86 3.76 6.1 19.81 2289.44 5.37 1.55 11.3 32 M 9 w 2w 3.65 7.5 18.55 1938.76 6.18 1.47 8.2 33 F 11 w 1m 4.07 3.65 7 19.77 2483.21 4.13 4.78 8.8 34 F 11 w 1m 3.97 3.68 4.6 10.94 1517.38 2.24 3.13 11.8 35 M 11 w 1m 3.54 3.77 5.2 6.95 810.96 1.61 1.14 22.1 36 M 11 w 1m 3.5 3.57 4.74. 8.34 1050.29 1.74 3.43 8 37 M 11 w 1m 4.39 3.57 7.1 4.57 597.3 1.44 2.43 12.3 38 F 11 w 1m 4.43 3.33 7 13.05 2089.06 4.06 3.78 11.4 39 M 11 w 1m 4.73 3.87 6.5 10.68 1233.3 3.09 2.5 9.7 40 M 11 w 1m 4.47 4.11 5.3 22.12 2227.02 5.21 4.57 11.2 41 F 15 w 2m 4.12 3.11 4.3 14.35 1022.42 2.74 3.49 11.6 42 M 15 w 2m 3.89 3.77 4.2 6.48 839.08 1.21 4.57 17.1 43 M 15 w 2m 3.5 3.11 4.1 16.31 1625.73 2.97 2.34 19.1 44 M 15 w 2m 3.46 3.67 8.6 10.86 1416.79 4.15 3.48 18 45 F 30 w 6m 3.09 4.13 7.7 16.07 1948.49 5.5 4.01 19.7 46 M 30 w 6m 3.18 3.9 7.6 12.72 1554.61 4.3 4.44 21.8 47 M 42 w 10m 3.17 4.11 10 9.24 1270.89 4.11 4.32 17.4 48 M 42 w 10m 3.2 4.19 8.2 15.58 1257.88 5.68 4.56 20
Page 53 of 53 Diabetes
Supplementary Table 3. Patients and liver biopsy data.
Blood Liver PEPCK Glucose Insulin C-peptide HOMA- Hdac9 Pepck Gender BMI IU/mL IU/mg (mU/mg (mmol/L) (mIU /L) (pg/ml) IR (fold) (fold) (Log10) (Log10) protein) 1 F 23.48 N N 4.30 8.06 1002.07 1.54 1.00 1.00 5.90 2 F 30.86 N N 5.12 7.26 863.71 1.65 1.25 1.12 3.10 3 F 20.73 N N 3.89 8.34 1169.29 1.44 1.74 0.74 6.70 4 F 35.06 N N 4.90 7.20 920.46 1.57 0.65 0.84 3.50 5 F 26.68 N N 5.02 8.16 1003.40 1.82 0.54 1.15 4.70 6 M 29.02 N N 4.46 8.55 1125.90 1.69 1.05 1.22 3.90 7 M 34.20 N N 4.29 13.38 1209.80 2.55 0.69 0.77 5.00 8 M 24.24 N N 4.17 10.19 1019.04 1.89 0.57 0.85 4.40 9 M 22.18 N N 4.05 6.40 960.74 1.15 1.21 1.05 3.20 10 M 22.68 N N 3.84 10.89 1488.78 1.86 1.37 1.23 5.10 11 F 24.24 6.53 8.12 5.76 11.68 1634.50 2.99 8.34 3.34 13.00 12 F 27.06 6.23 8.23 6.70 11.85 1573.61 3.53 7.85 2.85 12.30 13 F 24.22 5.75 8.39 10.60 12.03 1823.76 5.66 12.46 4.01 21.80 14 F 28.89 5.87 8.65 5.30 15.70 1388.30 3.67 6.79 2.89 17.60 15 F 26.95 6.08 8.04 5.80 25.25 2569.92 6.52 9.47 3.46 19.70 16 F 23.53 6.59 8.19 4.00 15.21 1543.86 2.71 6.66 2.99 12.40 17 M 24.26 5.63 8.63 5.20 12.42 1304.18 2.90 8.74 4.00 9.90 18 M 20.28 5.39 8.42 5.40 19.66 2001.65 4.71 10.48 3.37 15.30 19 M 24.22 6.42 8.00 4.07 10.41 2006.37 1.88 6.77 3.01 8.70 20 M 20.83 6.03 8.14 6.40 28.82 3399.21 8.15 14.38 5.01 14.30 21 M 25.61 5.81 8.38 6.10 9.83 1483.26 2.67 9.23 3.00 9.60 22 M 24.80 6.68 8.19 4.10 8.63 1073.24 1.58 7.41 2.89 14.50 23 F 24.49 6.41 8.16 4.60 10.81 952.62 2.22 8.55 3.42 13.00 24 M 24.49 6.58 8.10 4.00 13.60 1345.64 2.39 7.82 2.55 12.30 25 M 21.13 6.61 8.33 7.00 28.99 4248.51 9.07 11.79 4.32 21.80 26 F 17.96 7.00 8.64 5.70 16.07 1997.16 4.05 11.43 2.56 17.60 27 F 23.81 6.67 8.75 5.50 16.07 1779.60 3.90 6.65 3.67 19.70 28 F 23.44 6.41 8.09 6.70 22.72 3638.61 6.78 14.76 3.06 6.30 29 M 18.37 6.51 8.43 4.30 17.24 1771.91 3.26 6.44 4.00 7.40 30 F 23.26 6.65 7.80 5.00 9.52 1143.97 2.12 5.32 3.37 6.60 31 M 18.37 6.53 8.13 5.40 15.52 2980.46 3.76 9.77 3.01 11.10 32 M 23.74 5.75 8.37 5.10 8.97 1955.33 2.04 6.67 3.01 7.90 33 F 20.55 5.87 8.81 9.50 18.22 1598.91 7.73 5.49 2.88 8.40 34 F 22.89 4.83 7.04 4.60 11.22 887.11 2.30 4.31 1.22 6.30 35 M 22.49 6.68 8.30 5.50 14.46 1239.89 3.53 8.87 2.13 9.40 36 M 31.11 6.99 8.37 7.50 6.09 1281.86 2.05 7.96 1.98 10.20 37 M 27.34 6.89 8.17 6.50 35.42 3220.94 10.28 10.45 4.55 11.30 38 M 22.15 6.37 8.28 7.00 25.22 2383.44 7.91 9.96 3.14 9.60 39 M 20.76 5.08 8.14 7.10 21.90 2896.86 6.91 11.23 5.22 8.00 40 M 20.01 4.99 7.87 5.30 6.80 869.48 1.60 8.74 3.22 5.50 41 M 25.39 6.74 8.93 6.30 15.54 1833.70 4.37 5.34 2.78 7.90 42 M 29.41 4.89 6.30 6.60 22.14 2274.35 6.47 5.44 2.02 7.10 43 M 19.38 4.94 6.37 4.80 28.99 3325.84 6.21 6.67 1.98 6.70 44 M 27.43 5.08 7.39 7.20 23.45 2691.70 7.46 5.49 3.15 6.60 45 M 18.34 5.03 7.65 5.60 13.69 1836.55 3.39 7.23 4.55 8.00 46 M 27.68 4.98 6.14 5.80 20.49 1907.86 5.31 4.31 3.56 5.90 47 M 19.84 5.16 7.26 7.50 15.68 1304.51 5.22 8.45 4.32 6.20 48 M 24.49 5.20 6.38 6.40 14.56 1112.68 4.12 4.41 3.41 7.40 BMI = weight (kg) / height (m) square