Table of Contents Author Guidelines Submit a Manuscript
Mediators of Inflammation
Volume 2016, Article ID 5701959, 9 pages
http://dx.doi.org/10.1155/2016/5701959
Research Article

Adiponectin Inhibits LPS-Induced HMGB1 Release through an AMP Kinase and Heme Oxygenase-1-Dependent Pathway in RAW 264 Macrophage Cells

1Department of Biomedical Sciences, Graduate School of Veterinary Medicine, Hokkaido University, Kita 18, Nishi 9, Kita-ku, Sapporo 060-0818, Japan
2Department of Biochemistry, Faculty of Veterinary Medicine, Alexandria University, Edfina, Behera 22785, Egypt

Received 9 February 2016; Accepted 10 May 2016

Academic Editor: Denis Girard

Copyright © 2016 Mohamed Elfeky et al. This is an open access article distributed under the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original work is properly cited.

Abstract

High mobility group protein B1 (HMGB1) is a late inflammatory mediator that exaggerates septic symptoms. Adiponectin, an adipokine, has potent anti-inflammatory properties. However, possible effects of adiponectin on lipopolysaccharide- (LPS-) induced HMGB1 release are unknown. The aim of this study was to investigate effects of full length adiponectin on HMGB1 release in LPS-stimulated RAW 264 macrophage cells. Treatment of the cells with LPS alone significantly induced HMGB1 release associated with HMGB1 translocation from the nucleus to the cytosol. However, prior treatment with adiponectin suppressed LPS-induced HMGB1 release and translocation. The anti-inflammatory cytokine interleukin- (IL-) 10 similarly suppressed LPS-induced HMGB1 release. Adiponectin treatment decreased toll-like receptor 4 (TLR4) mRNA expression and increased heme oxygenase- (HO-) 1 mRNA expression without inducing IL-10 mRNA, while IL-10 treatment decreased TLR2 and HMGB1 mRNA expression and increased the expression of IL-10 and HO-1 mRNA. Treatment with the HO-1 inhibitor ZnPP completely prevented the suppression of HMGB1 release by adiponectin but only partially inhibited that induced by IL-10. Treatment with compound C, an AMP kinase (AMPK) inhibitor, abolished the increase in HO-1 expression and the suppression of HMGB1 release mediated by adiponectin. In conclusion, our results indicate that adiponectin suppresses HMGB1 release by LPS through an AMPK-mediated and HO-1-dependent IL-10-independent pathway.

1. Introduction

Sepsis, an almost universally fatal clinical syndrome that is caused by microbial infection, results from excess stimulation of the host immune system by pathogen components to produce various proinflammatory cytokines [1]. Overproduction of these cytokines causes systemic inflammation that can lead to tissue damage, multiple organ failure, and death [2, 3]. For example, bacterial lipopolysaccharides (LPS), a cell wall component of gram-negative bacteria, induces an acute inflammatory response initiated by its interaction with toll-like receptor 4 (TLR4) resulting in sequential release of “early” (e.g., tumor necrosis factor- (TNF-) α, interleukin- (IL-) 1, and IL-6) and “late” (e.g., high mobility group protein B1 (HMGB1)) proinflammatory cytokines [46]. However, therapies designed to block early released cytokines such as TNF-α or IL-1β have shown limited efficacy due to the early and transient kinetics of the production of these inflammatory cytokines [7, 8].

HMGB1 is a highly conserved, ubiquitous nonhistone nuclear protein that exhibits diverse functions according to its cellular location. Nuclear HMGB1 participates in DNA replication, recombination, transcription, and repair. In response to infection or injury, HMGB1 is actively secreted by innate immune cells and/or passively released by injured or damaged cells. Once released, HMGB1 binds with cell-surface receptors, such as the receptor for advanced glycation end products (RAGE) and/or TLRs including TLR2 and TLR4 and mediates various cellular responses, infiltration of innate immune cells, and subsequent release of various proinflammatory cytokines [912]. Administration of recombinant HMGB1 to mice is lethal, while administration of anti-HMGB1 antibodies or inhibitors provides protection against LPS-induced acute tissue damage and lethal endotoxaemia [4, 11, 13, 14]. Therefore, targeting HMGB1 release provides a wide window for clinical intervention against systemic inflammatory diseases.

Adiponectin, which is also known as adipocyte complement-related protein (Acrp30), is one of the most abundant ones of the bioactive molecules called adipokines that are secreted from adipose tissue [15]. Adiponectin plays an important role in various physiological processes including lipid metabolism, insulin sensitization, and anti-inflammatory responses [1618]. Evidence indicates that adiponectin suppresses the “early” phase of macrophage inflammatory responses. For example, adiponectin reduces macrophage differentiation and migration [19] and promotes macrophage polarization toward an anti-inflammatory M2 phenotype both in vivo and in cultured macrophages [20, 21]. Adiponectin also inhibits the upregulation of the expression of adhesion molecules and the enhancement of phagocytic activity and cytokine production in LPS-stimulated macrophages [19, 22], whereas it increases the release of anti-inflammatory mediators such as IL-10 and IL-1 receptor antagonist from macrophages [23].

A number of animal studies show that adiponectin has a protective effect against the development of inflammation related disorders. For example, treatment with adiponectin improves atherosclerosis through inhibition of macrophage aggregation [19] and improves nonalcoholic steatohepatitis via inhibition of lipogenic factors and TNF-α [24]. Moreover, adiponectin protects from endotoxin-induced disorders of organs including the liver [25], the lung [26], and the heart [27], although its deficiency is associated with severe polymicrobial sepsis with high mortality [28]. However, there has been no published report regarding the effects of adiponectin on the regulation of endotoxin-mediated release of “late” proinflammatory mediators such as HMGB1. Therefore, in this study, we investigated the effect of adiponectin on LPS-induced HMGB1 release in murine RAW 264 macrophage cells.

2. Materials and Methods

2.1. Materials

Rabbit anti-HMGB1 antibody was purchased from Cell Signaling Technology (CST) (Beverly, MA, USA). Recombinant mouse full length adiponectin expressed in HEK293 cells was purchased from Biovendor (Asheville, NC, USA). Recombinant murine IL-10 was purchased from PeproTech (Rocky Hill, NJ, USA). Zinc protoporphyrin IX (ZnPP) was purchased from Frontier Scientific (Logan, UT, USA). SB203580, compound C (dorsomorphin), wortmannin, and bovine serum albumin (BSA) were purchased from Sigma-Aldrich Fine Chemicals (St. Louis, MO, USA). OPTI-MEM I was purchased from Invitrogen (Carlsbad, CA, USA).

2.2. Cell Culture

Cells of the murine macrophage-like cell line RAW 264 (RCB0535, RIKEN Cell Bank, Japan) were maintained in Dulbecco’s modified Eagle’s medium (DMEM, Wako Pure Chemicals, Osaka, Japan) and supplemented with 10% fetal bovine serum (FBS, Trace Scientific Ltd., Melbourne, Australia), 100 U/mL penicillin, and 100 μg/mL streptomycin in an atmosphere of humidified 5% CO2 at 37°C. When the cells reached 80–90% confluence, they were washed twice with, and subsequently cultured in, serum-free OPTI-MEM I for 12 h before all treatments. The cells were treated with or without increasing concentrations of adiponectin or IL-10 for 18 h and were then stimulated with LPS (Escherichia coli O55:B5, Sigma-Aldrich) dissolved in phosphate buffer saline (PBS) at a concentration of 200 ng/mL for another 24 h. When included, the cells were treated with or without ZnPP, SB203580, compound C, or wortmannin 1 h before adiponectin (10 μg/mL) or IL-10 (100 ng/mL) addition.

2.3. Western Blotting Analysis

The level of HMGB1 in the culture medium was determined by western blotting analysis as previously reported [2932]. Briefly, culture medium samples were centrifuged to remove cellular debris, then concentrated 60-fold with the Amicon Ultra-4-10000 NMWL (Millipore, Billerica, MA, USA). The concentrated samples were mixed with SDS loading buffer (500 mM Tris-HCl, 10% SDS, 0.5% bromophenol blue, and 5% 2-mercaptoethanol), boiled at 100°C for 5 min, separated on 15% SDS-polyacrylamide gels, and transferred onto a polyvinylidene fluoride membrane (Immobilon, Millipore). The membrane was incubated in a blocking buffer (20 mM Tris-HCl (pH 7.5), 150 mM NaCl, 0.1% Tween 20 (TBS-T), and 5% skimmed milk) and then with rabbit anti-HMGB1 polyclonal antibody (1 : 2000 dilution in the blocking buffer) overnight at 4°C. Subsequently, the membrane was washed with TBS-T for 15 min and incubated with horseradish peroxidase-linked goat anti-rabbit immunoglobulin (CST) (1 : 5000 dilution in the blocking buffer) for 1 h at room temperature. The signals were visualized using chemiluminescent HRP Substrate (Millipore) according to the manufacturer’s instructions and were detected using the ImageQuant LAS 500 system (GE Healthcare, Buckinghamshire, UK). The intensity of chemiluminescence of the corresponding bands was quantified using Image J software (v. 1.48, http://imagej.nih.gov/ij/).

2.4. Quantitative Real-Time PCR (qRT-PCR)

Total RNA was extracted from RAW 264 cells using the RNAiso reagent (Takara Bio, Shiga, Japan) according to the manufacturer’s protocol. Total RNA (2 μg) was reverse transcribed using a 15-mer oligo (dT) adaptor primer and M-MLV reverse transcriptase (Invitrogen). Quantitative real-time PCR was performed on a fluorescence thermal cycler (Light Cycler system, Roche Diagnostics, Mannheim, Germany) using FastStart Essential DNA Green Master PCR kits (Roche Diagnostics). Expression levels were determined using the standard curve method with respective cDNA fragments as standards. The levels are reported relative to Gapdh expression as an internal control. The primer sequences used in this study and the length of each PCR product are listed in Table 1.

Table 1: Primer sequences for quantitative real-time PCR and the length of each PCR product.
2.5. Immunofluorescence

The cellular localization of HMGB1 was investigated using an immunofluorescence staining assay. RAW 264 cells (5 × 104 cells/well) were cultured on glass coverslips in 6-well plates. The cells were washed twice with PBS and then fixed with 4% paraformaldehyde for 30 min at room temperature. Subsequently, the cells were permeabilized with 10% Triton X-100 in PBS supplemented with 0.5% BSA and 0.15% glycine for 10 min, following which they were blocked in PBS containing 5% BSA and 0.3% Triton X-100 for 60 min. The glass coverslips were then incubated with rabbit anti-HMGB1 antibody (1 : 100 dilution in PBS containing 1% BSA and 0.3% Triton X-100) overnight at 4°C, followed by goat anti-rabbit Alexa flour 488 (1 : 400 dilution) (Invitrogen) in the dark for 1 h at room temperature. Cells were washed with PBS containing 0.1% Triton X-100 between all incubations steps, followed by a final wash in PBS. Nuclei were labeled by incubation with 4′,6-diamidino-2-phenylindole (DAPI, Invitrogen) for 10 min. The cells were washed three times for 5 min with PBS. The coverslips were mounted on slides using Prolong® Antifade Reagents (Invitrogen). Images were captured using a fluorescence microscope (Biorevo BZ-9000, Keyence Japan, Osaka, Japan) with a ×100 oil-immersion lens. No fluorescence was detected in control cells processed without the primary antibody. The fluorescence intensities of cytosolic and nuclear HMGB1 were quantified using Image J software.

2.6. Statistical Analysis

IBM SPSS Statistics version 22.0 software (SPSS, Chicago, IL, USA) was used for statistical analysis. Data are presented as means ± standard error (SE). Statistical comparisons between multiple groups were performed with one-way analysis of variance (ANOVA) followed by either Dunnett’s or a Tukey HSD post hoc test. A value of < 0.05 was considered statistically significant.

3. Results

RAW 264 cells released a small amount of HMGB1 into the medium under the culture conditions without any stimulation. The amount of HMGB1 that was released increased 6-fold upon stimulation of the cells with 200 ng/mL of LPS (Figure 1(a)). Cell viability was almost 100% even after treatment with 1 μg/mL of LPS (data not shown). The increased release of HMGB1 with LPS treatment was accompanied by HMGB1 translocation from the nucleus to the cytosol (Figures 1(b) and 1(c)). These results suggested that HMGB1 release was under the control of LPS signaling rather than being passive release due to LPS cytotoxicity. Prior treatment of the cells with full length adiponectin failed to affect basal HMGB1 release but dose dependently suppressed LPS-induced HMGB1 release and was accompanied by nuclear localization of most of the HMGB1 (Figures 1(a)1(c)).

Figure 1: Effect of recombinant adiponectin on LPS-induced HMGB1 release and HMGB1 cellular translocation. Raw 264 cells were cultured in DMEM supplemented with 10% FBS and were cultured in serum-free OPTI-MEM I medium for additional 12 h. The cells were treated with increasing concentrations of adiponectin for 18 h, then stimulated with LPS (200 ng/mL) for another 24 h. (a) Culture medium was collected and analyzed by HMGB1 western blotting, followed by quantification of the intensity of the chemiluminescent HMGB1 band. The results are expressed as means ± SE of three independent experiments ( significance compared with control; significance compared with LPS treated cells). (b and c) Cellular HMGB1 was immunostained with an anti-HMGB1 rabbit primary and Alexa Fluor 488 anti-rabbit secondary antibodies. The nucleus was stained with DAPI. Merge indicates the combination of both HMGB1 (Green) and nuclear (Blue) fluorescence. The fluorescence intensities of cytosolic and nuclear HMGB1 in (b) were separately analyzed and the ratio of cytosolic HMGB1 to nuclear HMGB1 is shown in (c) ( significance compared with control; significance compared with LPS treated cells).

As it has been reported that globular adiponectin exerts its anti-inflammatory actions through induction of IL-10 [21], we next examined the effect of IL-10 on LPS induction of HMGB1 release. Prior treatment of the cells with IL-10 also failed to enhance basal HMGB1 release. However, IL-10 at doses of 50 and 100 ng/mL greatly decreased the HMGB1 release into the medium that was induced by LPS (Figure 2).

Figure 2: Effect of recombinant IL-10 on LPS-induced HMGB1 release. Raw 264 cells were cultured as described in Figure 1 legend and were treated with IL-10 for 18 h, then stimulated with LPS (200 ng/mL) for another 24 h. Culture medium was collected and analyzed by HMGB1 western blotting followed by quantification of the intensity of the chemiluminescent HMGB1 band. The results are expressed as means ± SE of three independent experiments ( significance compared with control; and significance compared with LPS treated cells).

To further examine the mechanism behind the suppressive effect of adiponectin on LPS-induced HMGB1 release, we compared mRNA expression in cells treated with either full length adiponectin or IL-10. Among the genes quantified, RAW 264 cells constitutively expressed TLR4 mRNA, TLR2 mRNA, and myeloid differentiation factor 2 (MD2) mRNA (Figures 3(a)3(c)), all of which are plasma membrane components responsible for LPS binding and signaling. Treatment of the cells with adiponectin selectively decreased expression of TLR4 mRNA, while IL-10 treatment reduced only TLR2 mRNA expression. Distinct differences between full length adiponectin and IL-10 treatments were also observed in the expression of HMGB1 and IL-10 genes. The cells constitutively expressed HMGB1 mRNA, which was suppressed only by IL-10 treatment and not by adiponectin treatment (Figure 3(d)). On the other hand, the cells expressed very low levels of IL-10 mRNA, which was enhanced only by IL-10 treatment, but not by full length adiponectin treatment (Figure 3(e)). Thus, it was unlikely that full length adiponectin exerted its suppressive effect on LPS-induced HMGB1 release through induction of IL-10.

Figure 3: Effects of adiponectin and IL-10 on mRNA expression in RAW 264 cells. Raw 264 cells were cultured as described in Figure 1 legend and were treated with adiponectin (APN, 10 μg/mL) and IL-10 (100 ng/mL) for 18 h. RNA was extracted, and expressions of (a) TLR4, (b) TLR2, (c) MD2, (d) HMGB1, (e) IL-10, (f) HO-1, (g) Nrf2, (h) Sirt1, (i) Sirt6, and Gapdh (control) mRNAs were measured using qRT-PCR. The results are expressed as means ± SE of three independent experiments ( and significance compared with control (Cont)).

Interestingly, both IL-10 and full length adiponectin treatments enhanced the mRNA expression of HO-1, a downstream anti-inflammatory effector of IL-10 signaling (Figure 3(f)), while neither treatment affected the mRNA expression of nuclear factor erythroid-derived 2 related factor 2 (Nrf2), a transcription factor related with HO-1 gene expression (Figure 3(g)). In addition, neither IL-10 nor full length adiponectin treatment increased the mRNA expression of Sirt1 or Sirt6, which are histone deacetylases that function as a chromatin silencer to regulate recombination and genomic stability (Figures 3(h) and 3(i)). We therefore next examined the involvement of HO-1 in the suppressive effect of full length adiponectin on LPS-induced HMGB1 release. Treatment of the cells with zinc protoporphyrin (ZnPP), a HO-1 inhibitor, did not have any effect on HMGB1 release from either LPS-stimulated or control cells (Figure 4). However, treatment with ZnPP for 1 h before full length adiponectin treatment almost completely abolished adiponectin suppression of LPS-induced HMGB1 release, although it only slightly inhibited the suppression by IL-10. These results indicate that increased expression of HO-1 in response to full length adiponectin is necessary for adiponectin-mediated prevention of LPS-induced HMGB1 release.

Figure 4: Effect of an HO-1 inhibitor on the anti-inflammatory action of adiponectin or IL-10 on LPS-induced HMGB1 release. Raw 264 cells were cultured as described in Figure 1 legend and were treated with dimethyl sulfoxide (DMSO, control) or ZnPP (1 μM) for 1 h before treatment with adiponectin (10 μg/mL) or IL-10 (100 ng/mL) for 18 h. Cells were then stimulated with LPS (200 ng/mL) for another 24 h. Culture medium was collected and analyzed by HMGB1 western blotting followed by quantification of the intensity of the chemiluminescent HMGB1 band. The results are expressed as means ± SE of three independent experiments ( significance compared with control; and significance compared with LPS treated cells; significance compared with LPS plus ZnPP treated cells).

We then examined whether increased expression of HO-1 mRNA by full length adiponectin was mediated through AMP-activated kinase (AMPK), a main signaling pathway of adiponectin action [3335]. Treatment of the cells with compound C, an AMPK inhibitor, abolished the increase in expression of HO-1 mRNA by full length adiponectin, whereas treatment of the cells with wortmannin, a phosphatidylinositol-3-kinase (PI3K) inhibitor, or with SB203580, a p38 mitogen-activated protein kinase (p38MAPK) inhibitor, did not affect this increase (Figure 5). Consistent with these results, treatment of the cells with compound C, but not with SB203580, abolished adiponectin-mediated suppression of LPS-induced HMGB1 release (Figure 6).

Figure 5: Effect of kinase inhibitors on adiponectin-induced HO-1 mRNA expression in RAW 264 cells. Raw 264 cells were cultured as described in Figure 1 legend and were treated with adiponectin (10 μg/mL) for 18 h in the presence of DMSO (control), compound C (10 μM), wortmannin (1 μM), or SB203580 (10 μM). RNA was extracted, and expressions of Hmox1 (HO-1) and Gapdh mRNAs were measured using qRT-PCR. The results are expressed as means ± SE of three independent experiments ( and significance compared with control).
Figure 6: Effect of kinase inhibitors on the suppression by adiponectin of LPS-induced HMGB1 release. Raw 264 cells were cultured as described in Figure 1 legend and were treated with compound C (a) or SB203580 (b) for 1 h before treatment with adiponectin (10 μg/mL) for 18 h, following which they were stimulated with LPS (200 ng/mL) for another 24 h. Culture media were collected and analyzed by HMGB1 western blotting followed by quantification of the intensity of the chemiluminescent HMGB1 band. The results are expressed as means ± SE of three independent experiments ( and significance compared with control; significance compared with LPS treated cells; significance compared with LPS plus SB203580 treated cells).

4. Discussion

In the present study, we demonstrated for the first time that full length adiponectin prevents LPS-induced HMGB1 translocation from the nucleus to the cytosol and its subsequent release from Raw 264 mouse macrophage cells. This process is most probably mediated by AMPK-dependent HO-1 induction, as evidenced by the following results. Both AMPK and HO-1 inhibitors prevented the suppression of LPS-induced HMGB1 release by full length adiponectin and the AMPK inhibitor also prevented induction of HO-1 mRNA by full length adiponectin. Furthermore, the mechanism of the full length adiponectin effect is supported by previous reports that showed that full length adiponectin activates AMPK activity [3335], that activation of AMPK by metformin or dehydrodiconiferyl alcohol enhances HO-1 expression and its activity [36, 37], and that HO-1 is indispensable for the prevention of HMGB1 release [38, 39]. Of course, other events such as selective reduction in TLR4 mRNA expression by full length adiponectin might contribute, at least in part, to the suppression of LPS-induced HMGB1 release, since TLR4 is the predominant receptor for LPS [40, 41] and a similar decrease in cell-surface TLR4 expression is seen in macrophage cells treated with globular adiponectin [42]. However, other intracellular signaling pathways related to p38MAPK, PI3K, and the nuclear histone deacetylase sirtuin are unlikely to be involved in the mechanism, although they have been reported to be involved in some adiponectin functions [4346] or in the processes of HO-1 induction and LPS-induced HMGB1 release [4749].

We have also demonstrated that IL-10 is a potent inhibitor of LPS-induced HMGB1 release. However, the fact that full length adiponectin failed to induce IL-10 mRNA suggested that the suppression by full length adiponectin might not be attributed to IL-10 production. This hypothesis is supported by previous findings that the effects of full length adiponectin on macrophage function are independent of IL-10 [42, 44], although anti-inflammatory effects of globular adiponectin are mediated by IL-10 [21, 23, 5052]. The discrepancy between the role of IL-10 in the effects of full length and globular adiponectin has not been explored but is possibly due to different signals mediated through adipoR2 and adipoR1, respectively [42].

Accumulating evidence indicates that HO-1 plays a pivotal role in the anti-inflammatory cytoprotective effects of a wide variety of compounds including statins, phytochemicals such as resveratrol, and aspirin [53]. HO-1 is a microsomal enzyme that catalyzes the degradation of proinflammatory free heme and produces equimolar amounts of carbon monoxide, bilirubin, and iron [54]. The mechanisms that mediate the anti-inflammatory effects of HO-1 are not fully understood, but the potent antioxidant activity of bilirubin and the signaling gas activity of carbon monoxide are reported to suppress apoptosis, necrosis, inflammation, and oxidative stress. Interestingly, HO-1 is induced by pathophysiological stimuli including LPS and hemodynamic changes, but in most cases pathophysiological activation of HO-1 results in only a transient or marginal increase in HO-1 that falls below the threshold necessary to activate downstream components such as carbon monoxide [53]. In the present study, a fourfold increase in HO-1 mRNA expression compared to its basal expression was induced by full length adiponectin, whereas only a twofold increase was induced by IL-10. Combined with the result that the HO-1 inhibitor only partially abrogated the suppression by IL-10 of LPS-induced HMGB1 release, these findings suggested that IL-10 induces only a marginal increase in HO-1 mRNA and mainly utilizes an HO-1-independent pathway for the suppression of HMGB1 release.

In summary, we provide the novel finding that full length adiponectin suppresses HMGB1 release by LPS through an AMPK-HO-1-dependent pathway. Therefore, adiponectin plays an important role as a regulator of inflammation through inhibition of both early and late proinflammatory mediators under pathological conditions such as sepsis. Thus, it is possible that adiponectin might be a target for development of therapeutic agents against sepsis and other systemic inflammatory disorders.

Competing Interests

The authors declare that there are no competing interests regarding the publication of this paper.

References

  1. G. S. Martin, D. M. Mannino, S. Eaton, and M. Moss, “The epidemiology of sepsis in the United States from 1979 through 2000,” The New England Journal of Medicine, vol. 348, no. 16, pp. 1546–1554, 2003. View at Publisher · View at Google Scholar · View at Scopus
  2. N. C. Riedemann, R.-F. Guo, and P. A. Ward, “The enigma of sepsis,” The Journal of Clinical Investigation, vol. 112, no. 4, pp. 460–467, 2003. View at Publisher · View at Google Scholar · View at Scopus
  3. A. Oberholzer, C. Oberholzer, and L. L. Moldawer, “Sepsis syndromes: understanding the role of innate and acquired immunity,” Shock, vol. 16, no. 2, pp. 83–96, 2001. View at Publisher · View at Google Scholar · View at Scopus
  4. H. Wang, O. Bloom, M. Zhang et al., “HMG-1 as a late mediator of endotoxin lethality in mice,” Science, vol. 285, no. 5425, pp. 248–251, 1999. View at Publisher · View at Google Scholar · View at Scopus
  5. M. Guha and N. Mackman, “LPS induction of gene expression in human monocytes,” Cellular Signalling, vol. 13, no. 2, pp. 85–94, 2001. View at Publisher · View at Google Scholar · View at Scopus
  6. B. Beutler and E. T. Rietschel, “Innate immune sensing and its roots: the story of endotoxin,” Nature Reviews Immunology, vol. 3, no. 2, pp. 169–176, 2003. View at Publisher · View at Google Scholar · View at Scopus
  7. E. Abraham, A. Anzueto, G. Gutierrez et al., “Double-blind randomised controlled trial of monoclonal antibody to human tumour necrosis factor in treatment of septic shock. NORASEPT II Study Group,” The Lancet, vol. 351, no. 9107, pp. 929–933, 1998. View at Publisher · View at Google Scholar · View at Scopus
  8. A. Leelahavanichkul, H. Yasuda, K. Doi et al., “Methyl-2-acetamidoacrylate, an ethyl pyruvate analog, decreases sepsis-induced acute kidney injury in mice,” American Journal of Physiology—Renal Physiology, vol. 295, no. 6, pp. F1825–F1835, 2008. View at Publisher · View at Google Scholar · View at Scopus
  9. U. Andersson, H. Wang, K. Palmblad et al., “High mobility group 1 protein (HMG-1) stimulates proinflammatory cytokine synthesis in human monocytes,” Journal of Experimental Medicine, vol. 192, no. 4, pp. 565–570, 2000. View at Publisher · View at Google Scholar · View at Scopus
  10. J. S. Park, D. Svetkauskaite, Q. He et al., “Involvement of toll-like receptors 2 and 4 in cellular activation by high mobility group box 1 protein,” The Journal of Biological Chemistry, vol. 279, no. 9, pp. 7370–7377, 2004. View at Publisher · View at Google Scholar · View at Scopus
  11. M. T. Lotze and K. J. Tracey, “High-mobility group box 1 protein (HMGB1): nuclear weapon in the immune arsenal,” Nature Reviews Immunology, vol. 5, no. 4, pp. 331–342, 2005. View at Publisher · View at Google Scholar · View at Scopus
  12. A. Rouhiainen, S. Tumova, L. Valmu, N. Kalkkinen, and H. Rauvala, “Pivotal Advance: analysis of proinflammatory activity of highly purified eukaryotic recombinant HMGB1 (amphoterin),” Journal of Leukocyte Biology, vol. 81, no. 1, pp. 49–58, 2007. View at Publisher · View at Google Scholar · View at Scopus
  13. H. Wang, H. Yang, and K. J. Tracey, “Extracellular role of HMGB1 in inflammation and sepsis,” Journal of Internal Medicine, vol. 255, no. 3, pp. 320–331, 2004. View at Publisher · View at Google Scholar · View at Scopus
  14. H. Yang, M. Ochani, J. Li et al., “Reversing established sepsis with antagonists of endogenous high-mobility group box 1,” Proceedings of the National Academy of Sciences of the United States of America, vol. 101, no. 1, pp. 296–301, 2004. View at Publisher · View at Google Scholar · View at Scopus
  15. Y. Arita, S. Kihara, N. Ouchi et al., “Paradoxical decrease of an adipose-specific protein, adiponectin, in obesity,” Biochemical and Biophysical Research Communications, vol. 257, no. 1, pp. 79–83, 1999. View at Publisher · View at Google Scholar · View at Scopus
  16. H. Tilg and A. M. Wolf, “Adiponectin: a key fat-derived molecule regulating inflammation,” Expert Opinion on Therapeutic Targets, vol. 9, no. 2, pp. 245–251, 2005. View at Publisher · View at Google Scholar · View at Scopus
  17. N. Ouchi and K. Walsh, “A novel role for adiponectin in the regulation of inflammation,” Arteriosclerosis, Thrombosis, and Vascular Biology, vol. 28, no. 7, pp. 1219–1221, 2008. View at Publisher · View at Google Scholar · View at Scopus
  18. N. Ouchi, J. L. Parker, J. J. Lugus, and K. Walsh, “Adipokines in inflammation and metabolic disease,” Nature Reviews Immunology, vol. 11, no. 2, pp. 85–97, 2011. View at Publisher · View at Google Scholar · View at Scopus
  19. T. Yokota, K. Oritani, I. Takahashi et al., “Adiponectin, a new member of the family of soluble defense collagens, negatively regulates the growth of myelomonocytic progenitors and the functions of macrophages,” Blood, vol. 96, no. 5, pp. 1723–1732, 2000. View at Google Scholar · View at Scopus
  20. K. Ohashi, J. L. Parker, N. Ouchi et al., “Adiponectin promotes macrophage polarization toward an anti-inflammatory phenotype,” Journal of Biological Chemistry, vol. 285, no. 9, pp. 6153–6160, 2010. View at Publisher · View at Google Scholar · View at Scopus
  21. P. Mandal, B. T. Pratt, M. Barnes, M. R. McMullen, and L. E. Nagy, “Molecular mechanism for adiponectin-dependent m2 macrophage polarization: link between the metabolic and innate immune activity of full-length adiponectin,” The Journal of Biological Chemistry, vol. 286, no. 15, pp. 13460–13469, 2011. View at Publisher · View at Google Scholar · View at Scopus
  22. M. C. Wulster-Radcliffe, K. M. Ajuwon, J. Wang, J. A. Christian, and M. E. Spurlock, “Adiponectin differentially regulates cytokines in porcine macrophages,” Biochemical and Biophysical Research Communications, vol. 316, no. 3, pp. 924–929, 2004. View at Publisher · View at Google Scholar · View at Scopus
  23. A. M. Wolf, D. Wolf, H. Rumpold, B. Enrich, and H. Tilg, “Adiponectin induces the anti-inflammatory cytokines IL-10 and IL-1RA in human leukocytes,” Biochemical and Biophysical Research Communications, vol. 323, no. 2, pp. 630–635, 2004. View at Publisher · View at Google Scholar · View at Scopus
  24. A. Xu, Y. Wang, H. Keshaw, L. Y. Xu, K. S. L. Lam, and G. J. S. Cooper, “The fat-derived hormone adiponectin alleviates alcoholic and nonalcoholic fatty liver diseases in mice,” Journal of Clinical Investigation, vol. 112, no. 1, pp. 91–100, 2003. View at Publisher · View at Google Scholar · View at Scopus
  25. T. Masaki, S. Chiba, H. Tatsukawa et al., “Adiponectin protects LPS-induced liver injury through modulation of TNF-α in KK-Ay obese mice,” Hepatology, vol. 40, no. 1, pp. 177–184, 2004. View at Publisher · View at Google Scholar · View at Scopus
  26. J. M. Konter, J. L. Parker, E. Baez et al., “Adiponectin attenuates lipopolysaccharide-induced acute lung injury through suppression of endothelial cell activation,” Journal of Immunology, vol. 188, no. 2, pp. 854–863, 2012. View at Publisher · View at Google Scholar · View at Scopus
  27. Y. Watanabe, R. Shibata, N. Ouchi et al., “Adiponectin ameliorates endotoxin-induced acute cardiac injury,” BioMed Research International, vol. 2014, Article ID 382035, 6 pages, 2014. View at Publisher · View at Google Scholar · View at Scopus
  28. Y. Uji, H. Yamamoto, H. Tsuchihashi et al., “Adiponectin deficiency is associated with severe polymicrobial sepsis, high inflammatory cytokine levels, and high mortality,” Surgery, vol. 145, no. 5, pp. 550–557, 2009. View at Publisher · View at Google Scholar · View at Scopus
  29. W. Jiang and D. S. Pisetsky, “The role of IFN-alpha; and nitric oxide in the release of HMGB1 by RAW 264.7 cells stimulated with polyinosinic-polycytidylic acid or lipopolysaccharide,” Journal of Immunology, vol. 177, no. 5, pp. 3337–3343, 2006. View at Publisher · View at Google Scholar · View at Scopus
  30. K. Tsoyi, H. J. Jang, I. T. Nizamutdinova et al., “Metformin inhibits HMGB1 release in LPS-treated RAW 264.7 cells and increases survival rate of endotoxaemic mice,” British Journal of Pharmacology, vol. 162, no. 7, pp. 1498–1508, 2011. View at Publisher · View at Google Scholar · View at Scopus
  31. C. K. Zetterström, W. Jiang, H. Wähämaa et al., “Pivotal Advance: inhibition of HMGB1 nuclear translocation as a mechanism for the anti-rheumatic effects of gold sodium thiomalate,” Journal of Leukocyte Biology, vol. 83, no. 1, pp. 31–38, 2008. View at Publisher · View at Google Scholar · View at Scopus
  32. A. Chorny and M. Delgado, “Neuropeptides rescue mice from lethal sepsis by down-regulating secretion of the late-acting inflammatory mediator high mobility group box 1,” American Journal of Pathology, vol. 172, no. 5, pp. 1297–1307, 2008. View at Publisher · View at Google Scholar
  33. T. Kadowaki and T. Yamauchi, “Adiponectin and adiponectin receptors,” Endocrine Reviews, vol. 26, no. 3, pp. 439–451, 2005. View at Publisher · View at Google Scholar · View at Scopus
  34. T. Yamauchi, J. Kamon, Y. Ito et al., “Cloning of adiponectin receptors that mediate antidiabetic metabolic effects,” Nature, vol. 423, pp. 762–769, 2003. View at Publisher · View at Google Scholar
  35. T. Kadowaki, T. Yamauchi, N. Kubota, K. Hara, K. Ueki, and K. Tobe, “Adiponectin and adiponectin receptors in insulin resistance, diabetes, and the metabolic syndrome,” Journal of Clinical Investigation, vol. 116, no. 7, pp. 1784–1792, 2006. View at Publisher · View at Google Scholar · View at Scopus
  36. G. Ashabi, L. Khalaj, F. Khodagholi, M. Goudarzvand, and A. Sarkaki, “Pre-treatment with metformin activates Nrf2 antioxidant pathways and inhibits inflammatory responses through induction of AMPK after transient global cerebral ischemia,” Metabolic Brain Disease, vol. 30, no. 3, pp. 747–754, 2015. View at Publisher · View at Google Scholar · View at Scopus
  37. J. Lee and S. Kim, “Upregulation of heme oxygenase-1 expression by dehydrodiconiferyl alcohol (DHCA) through the AMPK-Nrf2 dependent pathway,” Toxicology and Applied Pharmacology, vol. 281, no. 1, pp. 87–100, 2014. View at Publisher · View at Google Scholar · View at Scopus
  38. K. Tsoyi, T. Y. Lee, Y. S. Lee et al., “Heme-oxygenase-1 induction and carbon monoxide-releasing molecule inhibit lipopolysaccharide (LPS)-induced high-mobility group box 1 release in vitro and improve survival of mice in LPS- and cecal ligation and puncture-induced sepsis model in vivo,” Molecular Pharmacology, vol. 76, no. 1, pp. 173–182, 2009. View at Publisher · View at Google Scholar · View at Scopus
  39. H.-G. Chen, K.-L. Xie, H.-Z. Han et al., “Heme oxygenase-1 mediates the anti-inflammatory effect of molecular hydrogen in LPS-stimulated RAW 264.7 macrophages,” International Journal of Surgery, vol. 11, no. 10, pp. 1060–1066, 2013. View at Publisher · View at Google Scholar · View at Scopus
  40. C. N. Lumeng, “Innate immune activation in obesity,” Molecular Aspects of Medicine, vol. 34, no. 1, pp. 12–29, 2013. View at Publisher · View at Google Scholar · View at Scopus
  41. D. M. Rocha, A. P. Caldas, L. L. Oliveira, J. Bressan, and H. H. Hermsdorff, “Saturated fatty acids trigger TLR4-mediated inflammatory response,” Atherosclerosis, vol. 244, pp. 211–215, 2016. View at Publisher · View at Google Scholar
  42. P. Mandal, S. Roychowdhury, P.-H. Park, B. T. Pratt, T. Roger, and L. E. Nagy, “Adiponectin and heme oxygenase-1 suppress TLR4/MyD88-independent signaling in rat Kupffer cells and in mice after chronic ethanol exposure,” The Journal of Immunology, vol. 185, no. 8, pp. 4928–4937, 2010. View at Publisher · View at Google Scholar · View at Scopus
  43. M. J. Yoon, G. Y. Lee, J.-J. Chung et al., “Adiponectin increases fatty acid oxidation in skeletal muscle cells by sequential activation of AMP-activated protein kinase, p38 mitogen-activated protein kinase, and peroxisome proliferator-activated receptor α,” Diabetes, vol. 55, no. 9, pp. 2562–2570, 2006. View at Publisher · View at Google Scholar
  44. E. J. Folco, V. Z. Rocha, M. López-Ilasaca, and P. Libby, “Adiponectin inhibits pro-inflammatory signaling in human macrophages independent of interleukin-10,” The Journal of Biological Chemistry, vol. 284, no. 38, pp. 25569–25575, 2009. View at Publisher · View at Google Scholar · View at Scopus
  45. M. E. Grossmann, K. J. Nkhata, N. K. Mizuno, A. Ray, and M. P. Cleary, “Effects of adiponectin on breast cancer cell growth and signaling,” British Journal of Cancer, vol. 98, no. 2, pp. 370–379, 2008. View at Publisher · View at Google Scholar · View at Scopus
  46. N. T. Pun, A. Subedi, M. J. Kim, and P.-H. Park, “Globular adiponectin causes tolerance to LPS-induced TNF-α expression via autophagy induction in RAW 264.7 macrophages: involvement of SIRT1/FoxO3A axis,” PLoS ONE, vol. 10, no. 5, Article ID e0124636, 2015. View at Publisher · View at Google Scholar · View at Scopus
  47. Y. M. Kim, H. J. Kim, and K. C. Chang, “Glycyrrhizin reduces HMGB1 secretion in lipopolysaccharide-activated RAW 264.7 cells and endotoxemic mice by p38/Nrf2-dependent induction of HO-1,” International Immunopharmacology, vol. 26, no. 1, pp. 112–118, 2015. View at Publisher · View at Google Scholar · View at Scopus
  48. J. Wang, X. Hu, J. Xie, W. Xu, and H. Jiang, “Beta-1-adrenergic receptors mediate Nrf2-HO-1-HMGB1 axis regulation to attenuate hypoxia/reoxygenation-induced cardiomyocytes injury in vitro,” Cellular Physiology and Biochemistry, vol. 35, no. 2, pp. 767–777, 2015. View at Publisher · View at Google Scholar
  49. T. D. Walko III, V. Di Caro, J. Piganelli, T. R. Billiar, R. S. Clark, and R. K. Aneja, “Poly(ADP-ribose) polymerase 1-sirtuin 1 functional interplay regulates LPS-mediated high mobility group box 1 secretion,” Molecular Medicine, vol. 20, pp. 612–624, 2014. View at Publisher · View at Google Scholar
  50. M. Kumada, S. Kihara, N. Ouchi et al., “Adiponectin specifically increased tissue inhibitor of metalloproteinase-1 through interleukin-10 expression in human macrophages,” Circulation, vol. 109, no. 17, pp. 2046–2049, 2004. View at Publisher · View at Google Scholar · View at Scopus
  51. P.-H. Park, M. R. McMullen, H. Huang, V. Thakur, and L. E. Nagy, “Short-term treatment of RAW264.7 macrophages with adiponectin increases tumor necrosis factor-α (TNF-α) expression via ERK1/2 activation and Egr-1 expression: role of TNF-α in adiponectin-stimulated interleukin-10 production,” The Journal of Biological Chemistry, vol. 282, no. 30, pp. 21695–21703, 2007. View at Publisher · View at Google Scholar · View at Scopus
  52. P. Mandal, P.-H. Park, M. R. McMullen, B. T. Pratt, and L. E. Nagy, “The anti-inflammatory effects of adiponectin are mediated via a heme oxygenase-1-dependent pathway in rat kupffer cells,” Hepatology, vol. 51, no. 4, pp. 1420–1429, 2010. View at Publisher · View at Google Scholar · View at Scopus
  53. J. F. Ndisang, “Role of the heme oxygenase-adiponectin-atrial natriuretic peptide axis in renal function,” Current Pharmaceutical Design, vol. 21, no. 30, pp. 4380–4391, 2015. View at Publisher · View at Google Scholar · View at Scopus
  54. A. Paine, B. Eiz-Vesper, R. Blasczyk, and S. Immenschuh, “Signaling to heme oxygenase-1 and its anti-inflammatory therapeutic potential,” Biochemical Pharmacology, vol. 80, no. 12, pp. 1895–1903, 2010. View at Publisher · View at Google Scholar · View at Scopus