OBJECTIVE Chemerin is a recently discovered hepatoadipokine that regulates adipocyte differentiation as well as chemotaxis and activation of dendritic cells and macrophages. Chemerin was reported to modulate insulin sensitivity in adipocytes and skeletal muscle cells in vitro and to exacerbate glucose intolerance in several mouse models in vivo. In humans, chemerin was shown to be associated with multiple components of the metabolic syndrome including BMI, triglycerides, HDL cholesterol, and hypertension. This study aimed to examine the effect of chemerin on weight, glucose and lipid metabolism, as well as atherosclerosis in vivo.
RESEARCH DESIGN AND METHODS We used recombinant adeno-associated virus to express human chemerin in LDL receptor knockout mice on high-fat diet.
RESULTS Expression of chemerin did not significantly alter weight, lipid levels, and extent of atherosclerosis. Chemerin, however, significantly increased glucose levels during the intraperitoneal glucose tolerance test without affecting endogenous insulin levels and the insulin tolerance test. Chemerin reduced insulin-stimulated Akt1 phosphorylation and activation of 5′AMP-activated protein kinase (AMPK) in the skeletal muscle, but had no effect on Akt phosphorylation and insulin-stimulated AMPK activation in the liver and gonadal adipose tissue.
CONCLUSIONS Chemerin induces insulin resistance in the skeletal muscle in vivo. Chemerin is involved in the cross talk between liver, adipose tissue, and skeletal muscle.
Chemerin was initially described in 2003 as a novel chemoattractant protein (1) that, upon enzymatic proteolysis, modulates chemotaxis and activation of dendritic cells and macrophages through distinct G protein-coupled receptors such as CMKLR1, GPR1, and CCRL2 (2–4). More recently, chemerin was reported as a hepatoadipokine that regulates adipocyte differentiation in an autocrine/paracrine manner via CMKLR1 and modulates the expression of adipocyte genes involved in glucose and lipid homeostasis (5,6). Conflicting data exist regarding the effect of chemerin on insulin signaling in adipocytes in vitro. Kralisch et al. (7) demonstrated that chemerin downregulated insulin-stimulated glucose uptake in 3T3-L1 adipocytes, while Takahasi et al. (8) reported the opposite. In skeletal muscle cells, chemerin was shown to impair insulin signaling and glucose uptake, a process partially mediated by activation of the extracellular signal–regulated kinases-1/2 (9). In humans, chemerin correlated with systemic markers of inflammation such as high-sensitivity C-reactive protein, interleukin-6, and tumor necrosis factor-α and was associated with components of the metabolic syndrome including BMI, triglycerides, HDL cholesterol, and hypertension in different populations (5,10–13). In morbidly obese patients undergoing bariatric surgery, weight loss was associated with improvement of various metabolic parameters and a sustained reduction of chemerin levels (14,15). Taken together, available data suggest that chemerin may play a role in glucose and lipid metabolism as well as inflammation. Surprisingly little data, however, are currently available about the potential effects of chemerin on the regulation of these parameters in vivo.
Recently, Ernst et al. (16) reported that acute administration of recombinant human chemerin exacerbated glucose intolerance, lowered serum insulin levels, and decreased tissue glucose uptake in ob/ob, db/db, and diet-induced obese (DIO) but not in normoglycemic wild-type mice. As acute injection of chemerin may not reflect the effect of chronically elevated chemerin levels seen in obesity, we designed the present study to investigate the impact of long-term chemerin overexpression on body weight, glucose and lipid metabolism, as well as atherosclerosis in LDL receptor knockout (LDLRKO) mice on a high-fat diet (HFD). As human chemerin fully binds to and activates murine CMKLR1 (17), we expressed human chemerin using a recombinant adeno-associated virus (AAV)-based vector in this well-established mouse model of diet-induced insulin resistance, dyslipidemia, and atherosclerosis.
RESEARCH DESIGN AND METHODS
Generation of recombinant adeno-associated viral constructs.
All constructs were expressed under control of the thyroxine-binding globulin promoter (18,19). Transgenes were full-length human chemerin (preprochemerin, aa 1–163) and β-galactosidase (LacZ) as control. To produce AAV vectors encapsidated in an AAV8 capsid (AAV2.8), a pseudotyping strategy was performed. Vectors (AAV.chemerin, AAV.lacZ) were purified using a standard cesium sedimentation method, and titers were determined via TaqMan analysis using probes and primers targeting the bovine GH poly(A+) region of the vectors (18,19).
Male LDLRKO (B6.12957-LDLrtm1Her/J) mice were obtained from Charles River Laboratories (Sulzfeld, Germany). Mice (5 weeks of age) were injected intravenously via the tail vein with 1 × 1013 particles of AAV.chemerin or AAV.lacZ. LDLRKO mice (n = 13 per group) were kept on a HFD (0.21% cholesterol, 21% butterfat; ssniff, Soest, Germany) for 16 weeks. After 12 h of overnight fasting, blood was drawn before and several time points after virus injection. The study was approved by the District Government of Upper Bavaria.
The intraperitoneal glucose tolerance test (ipGTT) and the insulin tolerance test (ITT) were performed 12 and 14 weeks after AAV injection, respectively (detailed description in the supplement available online at http://diabetes.diabetesjournals.org/cgi/content/full/db10-0362/DC1).
At the end of the study (16 weeks after injection), mice (n = 12 per group; one death per group during the study) were injected intraperitoneally with insulin (n = 6 per group) (0.02 units/g body weight) or saline (n = 6) to determine protein levels and phosphorylation of Akt1 and 5′AMP-activated protein kinase (AMPK)-α. Mice were killed 15 min after injection and organs were harvested. Liver, skeletal muscle, and gonadal adipose tissue were freeze-clamped in liquid nitrogen in situ and stored at −80°C for further analysis. Aortas of LDLRKO mice were harvested for en face quantification of atherosclerotic lesions.
Blood sample assays.
Human and murine serum chemerin levels were determined using commercially available enzyme-linked immunosorbent assays (ELISAs) (R&D Systems, Wiesbaden, Germany). Plasma insulin levels were measured with an ultrasensitive insulin immunoassay (Alpco, Salem, MA). Serum total cholesterol, triglyceride, and HDL cholesterol levels were measured enzymatically on an Alcyon 300 analyzer (Abbott GmbH, Wiesbaden, Germany) using commercial reagents (Diasys, Holzheim, Germany).
Analysis of mRNA expression.
Total RNA was extracted as previously described (19). Real-time PCR was performed using the Realplex4 Mastercycler (Eppendorf, Hamburg, Germany). Expression levels of genes of interest were determined using the Assays-On-Demand TaqMan primers and probes (Applied Biosystems, Carlsbad, CA) according to the manufacturer's instructions (supplemental data in the online appendix).
One μl of murine and human serum samples were subjected to 10% BisTris gel and transferred to a polyvinylidene fluoride (PVDF) membrane (Immobilon-P, Zefa-Laborservice, Germany). Human chemerin was detected with goat anti-human chemerin antibody (concentration 1:1,000; R&D Systems, Wiesbaden, Germany) and peroxidase-conjugated AffiniPureRabbit anti-goat IgG (H+L) (concentration 1:10.000; Jackson ImmunoResearch, Baltimore, MD) as the secondary antibody.
Insulin signaling and activation of AMPK-α.
Liver, skeletal muscle, and adipose tissue samples were homogenized in radioimmunoprecipitation assay-buffer (50 mmol/l Tris-HCl, pH 7.4; 1% NP-40; 0,25% Na-deoxycholate; 150 mmol/l NaCl; 1 mmol/l EDTA; 1 mmol/l phenylmethylsulfonyl fluoride; 1 μg/ml of each aprotinin, leupeptin, pepstatin; 1 mmol/l Na3VO4; 1 mmol/l NaF), and lysates were subjected to 10% BisTris gel and transferred to PVDF membrane (Immobilon-P; Zefa-Laborservice, Germany). Anti Akt1 (C73H10) (concentration 1:1,000), phospho-Akt (Thr308) (C31E5) (concentration 1:1,000), AMPK-α (23A3) (concentration 1:1,000), phospho-AMPK-α (Thr172) (D79.5E) (concentration 1:1,000), and anti-rabbit IgG horseradish peroxidase-linked antibodies (concentration 1:10.000) were obtained from Cell Signaling (Danvers, MA). Anti-actin antibody was purchased from Sigma (Sigma, St. Louis, MO).
For the quantification of the aortic plaques, the mouse aorta was carefully harvested and stained with Sudan IV (Sigma, Germany) as previously described (18,19). The extent of the lesion area was determined using Nikon Nis Elements D3.0 (Nikon, Düsseldorf, Germany). Data are reported as the percentage of the aortic surface covered by lesions (total surface area of the atherosclerotic lesions divided by the total surface area of the aorta).
Data are expressed as the mean ± SEM. Analysis of the data was performed using the unpaired Student t test. Statistical significance for all comparisons was assigned at P < 0.05.
To examine the effect of chemerin expression on body weight, glucose and lipid metabolism, as well as atherosclerosis in vivo, LDLRKO mice on HFD were injected with 1 × 1013 particles of AAV.chemerin or control (AAV.lacZ). Injection of AAV.chemerin resulted in specific and sustained chemerin expression over the course of the study with serum levels comparable with those seen in healthy human volunteers (Fig. 1A and B). Expression of human chemerin did not alter murine chemerin serum levels (Fig. 1C).
Mice injected with AAV.chemerin or AAV.lacZ had a similar change in body weight over the 16-week study period (supplemental Fig. 1, found in the online appendix). Compared with control mice, chemerin-expressing mice showed significantly increased glucose levels during both the ipGTT (without affecting endogenous insulin levels) and the ITT (Fig. 2), indicating that overexpression of human chemerin induces insulin resistance in LDLRKO mice. To determine whether expression of chemerin resulted in a tissue-specific pattern of insulin resistance, insulin signaling was examined in liver, adipose tissue, and skeletal muscle. Expression of chemerin substantially reduced insulin-stimulated Akt1 phosphorylation and AMPK-α activation in the skeletal muscle (Fig. 3). In contrast, mice injected with AAV.chemerin showed no effect on basal and insulin-stimulated hepatic Akt1 phosphorylation, AMPK-α activation, and the mRNA expression of the gluconeogenic enzymes G6P and PEPCK (supplemental Fig. 2, found in the online appendix). In gonadal adipose tissue, expression of chemerin slightly decreased phospho-AMPK-α levels in the absence of insulin but did not alter insulin-stimulated AMPK-α activation and Akt1 signaling (supplemental Fig. 3, found in the online appendix). In conclusion, expression of chemerin induced glucose intolerance via induction of insulin resistance in the skeletal muscle.
Mice-expressing chemerin did not show significantly altered total cholesterol, triglyceride, HDL cholesterol, and non-HDL cholesterol levels compared with controls (supplemental Fig. 4, found in the online appendix). Likewise, expression of chemerin did not change the mean atherosclerotic lesion area as determined by en face analysis of the entire aorta (Fig. 4).
Our study aimed to determine the effect of human chemerin on weight, glucose and lipid metabolism, as well as atherosclerosis in vivo in LDLRKO mice on HFD. We demonstrated that expression of chemerin with serum levels comparable with those seen in healthy human volunteers induced insulin resistance in the skeletal muscle with increased glucose levels during both the ipGTT and the ITT. Expression of chemerin, however, did not significantly alter weight, lipid levels, and extent of atherosclerotic lesion area.
Ernst et al. (16) reported that acute administration of recombinant human chemerin exacerbated glucose intolerance and lowered serum insulin levels in ob/ob and db/db mice but had no effect on glucose tolerance in wild-type mice on chow diet. Chemerin injection of DIO mice also resulted in impaired glucose tolerance but (except for the 2-h time point) did not reduce insulin levels during GTT. Chemerin significantly decreased liver but not skeletal muscle glucose uptake in db/db mice. Consistent with Ernst et al. (16), long-term expression of human chemerin in our diet-induced mouse model of insulin resistance and atherosclerosis resulted in glucose intolerance without altering insulin levels. We did not assess the effect of chemerin on glucose uptake in different tissues. However, given the results of the present study, we would have expected decreased glucose uptake in the skeletal muscle consistent with data from Sell et al. (9) demonstrating that chemerin impaired insulin signaling and glucose uptake in skeletal muscle cells in vitro. Unfortunately, Ernst et al. (16) did not report the effect of acute chemerin administration on glucose uptake in DIO mice. Further studies, including clamp techniques, are necessary to better characterize the effect of chemerin on glucose metabolism in vivo and to address the mechanism by which chemerin reduced insulin-stimulated Akt1 phosphorylation and AMPK-α activation in the skeletal muscle. In vitro, Sell et al. (9) identified activation of p38 MAP kinase, extracellular signal–regulated kinases-1/2, and p56 as potential mechanisms that might mediate the effect of chemerin on insulin resistance in skeletal muscle cells.
In contrast to epidemiological data (5,12,13), chemerin had no significant effect on triglyceride and HDL cholesterol levels in our study. Studies in mice with a more human-like lipoprotein metabolism (e.g., APOE*3-Leiden.CETP transgenic mice) may be required to reproduce the lipid phenotype seen in humans.
Lack of chemerin on the atherosclerotic lesion area does not contradict previous studies demonstrating that chemerin modulates activation of immune cells in inflamed tissues of patients with skin disorders (20,21) or mouse models of peritonitis and lung disease (3,17). One could speculate that chemerin may affect early atherosclerotic plaque development and/or plaque morphology rather than extent of atherosclerotic lesion area. In patients with stable chest pain, however, chemerin was not associated with coronary atherosclerotic plaque morphology as determined by computed tomography-angiography (12).
Chemerin is synthesized as a secreted precursor, prochemerin, which is poorly active on the chemerin receptor CMKLR1 (1). Prochemerin can be rapidly converted into inactive, proinflammatory, or anti-inflammatory chemerin variants by proteolytic removal of carboxy-terminal peptides mediated by distinct proteases of the coagulation and inflammation cascades (3,22–24). Unfortunately, the antibodies used in our study for Western blot analysis, human and murine chemerin ELISAs, detect prochemerin, chemerin, and other proteolytically processed forms but do not allow us to distinguish between these peptides. Since distinct chemerin forms differ substantially in their bioactivity, the significance for total chemerin assessment is limited thus complicating the interpretation of our results. It is reasonable to speculate that since both human and murine chemerin activate the murine chemerin receptor CMKLR1 (17), overall increased chemerin levels resulted in glucose intolerance and insulin resistance in the skeletal muscle of LDLRKO mice on HFD. However, it is also conceivable that expression of chemerin altered its enzymatic proteolysis thus modulating both murine and human chemerin bioactivity.
In summary, we determined in this present study the effect of human chemerin on weight, glucose and lipid metabolism, as well as atherosclerosis in vivo. We demonstrated that expression of chemerin induced insulin resistance in the skeletal muscle of LDLRKO mice on HFD. Expression of chemerin, however, did not significantly alter weight, lipid levels, and extent of atherosclerotic lesion area.
This research did not receive any specific grant from any funding agency in the public, commercial, or not-for-profit sector. No potential conflicts of interest relevant to this article were reported.
M.B. wrote the manuscript, researched the data, and revised the manuscript. K.R. researched the data and reviewed/edited the manuscript. C.L. researched the data, contributed to the discussion, and reviewed/edited the manuscript. J.Z. researched the data and reviewed/edited the manuscript. B.G. contributed to the discussion and reviewed/edited the manuscript. K.G.P contributed to the discussion and reviewed/edited the manuscript. M.L. designed the study, contributed to the discussion, and reviewed/edited the manuscript. U.C.B designed the study, wrote the manuscript, and revised the manuscript.
Parts of this study were presented in poster form at the 46th annual meeting of the European Association for the Study of Diabetes, Stockholm, Sweden, 20–24 September 2010.
We are indebted to Elisabeth Fleischer-Brielmaier, Inge Biller-Friedmann, Daniela Bureik, and Kerstin Henze from the Department of Internal Medicine II, University of Munich, Munich, Germany, for their expert technical assistance.
The costs of publication of this article were defrayed in part by the payment of page charges. This article must therefore be hereby marked “advertisement” in accordance with 18 U.S.C. Section 1734 solely to indicate this fact.
- Received March 13, 2010.
- Accepted July 30, 2010.
- © 2010 by the American Diabetes Association.
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