Advertisement

Molecular Medicine

, Volume 19, Issue 1, pp 387–398 | Cite as

Activation of AMPK Enhances Neutrophil Chemotaxis and Bacterial Killing

  • Dae Won Park
  • Shaoning Jiang
  • Jean-Marc Tadie
  • William S. Stigler
  • Yong Gao
  • Jessy Deshane
  • Edward Abraham
  • Jaroslaw W. Zmijewski
Open Access
Research Article

Abstract

An inability of neutrophils to eliminate invading microorganisms is frequently associated with severe infection and may contribute to the high mortality rates associated with sepsis. In the present studies, we examined whether metformin and other 5′ adenosine monophosphate-activated protein kinase (AMPK) activators affect neutrophil motility, phagocytosis and bacterial killing. We found that activation of AMPK enhanced neutrophil chemotaxis in vitro and in vivo, and also counteracted the inhibition of chemotaxis induced by exposure of neutrophils to lipopolysaccharide (LPS). In contrast, small interfering RNA (siRNA)-mediated knockdown of AMPKα1 or blockade of AMPK activation through treatment of neutrophils with the AMPK inhibitor compound C diminished neutrophil chemotaxis. In addition to their effects on chemotaxis, treatment of neutrophils with metformin or aminoimidazole carboxamide ribonucleotide (AICAR) improved phagocytosis and bacterial killing, including more efficient eradication of bacteria in a mouse model of peritonitis-induced sepsis. Immunocytochemistry showed that, in contrast to LPS, metformin or AICAR induced robust actin polymerization and distinct formation of neutrophil leading edges. Although LPS diminished AMPK phosphorylation, metformin or AICAR was able to partially decrease the effects of LPS/toll-like receptor 4 (TLR4) engagement on downstream signaling events, particularly LPS-induced IκBα degradation. The IκB kinase (IKK) inhibitor PS-1145 diminished IκBα degradation and also prevented LPS-induced inhibition of chemotaxis. These results suggest that AMPK activation with clinically approved agents, such as metformin, may facilitate bacterial eradication in sepsis and other inflammatory conditions associated with inhibition of neutrophil activation and chemotaxis. Online address: https://doi.org/www.molmed.org

Introduction

Neutrophils are an essential component of the innate immune system, with a primary role in the clearance of extracellular pathogens (1). Both localization and neutralization of microorganisms are important neutrophil functions that are orchestrated by specific inflammatory mediators released from the site of infection (2,3). In particular, chemoattractants and chemokine gradients are major neutrophil guidance signals, whereas the migration of neutrophils from the vasculature to inflammatory sites is mediated by adhesion proteins, including P- and E-selectins and integrin ligands such as vascular cell adhesion molecule 1 (VCAM-1), intracellular adhesion molecule 1 (ICAM-1) and ICAM-2 on endothelium (2,4). Several mechanisms are involved in bacterial killing by neutrophils. For example, release of antimicrobial peptides, generation of reactive nitrogen and oxygen species (ROS/RNS), as well as production of hypochlorous acid by myeloperoxidase, are utilized by neutrophils to kill invading microorganisms (5,6). In addition to phagocytosis and killing internalized microorganisms, neutrophils also can release DNA and DNA-associated proteins to form extracellular traps to prevent bacterial dissemination (7,8).

Although killing of microorganisms is apparently a beneficial function of neutrophil activation, exaggerated activation of neutrophils can result in collateral damage to tissues and also contribute to the development of organ failure in sepsis (9,10). However, impairment of neutrophil activation also can lead to serious complications in infected patients. In particular, diminished neutrophil activation or decreased neutrophil numbers are associated with a high mortality rate in sepsis (11). Neutrophil dysfunction also commonly occurs with bacterial pneumonia in critically ill patients after trauma and hemorrhage (12, 13, 14, 15).

Beside the central roles that NADPH-oxidase and ROS occupy in killing microorganisms, enhanced propagation and dissemination of bacteria are associated with loss of neutrophil ability to reach the site of infection (16,17). In sepsis, such alterations in neutrophil function are a result of disrupted chemokine signaling and expression of adhesion molecules (16, 17, 18, 19, 20, 21). For example, the appearance of detectable levels of the bacterial products lipopolysaccharide (LPS) or lipoteichoic acid in the circulation of severely infected patients is associated with diminished neutrophil chemotaxis, including neutrophil response to interleukin 8 (IL-8), macrophage inflammatory protein 2 (MIP-2), or keratinocyte-derived chemokine (KC). In spite of progress in understanding mechanisms responsible for the inhibition of neutrophil chemotaxis, pharmacologic approaches to prevent or restore neutrophil chemotaxis and bacterial eradication are not available.

Metformin is commonly used in patients with non-insulin-dependent diabetes mellitus to lower blood glucose concentrations and to improve insulin sensitivity (22). Metformin has been shown to prevent cardiovascular complications associated with diabetes and obesity through mechanisms that presumably involve inhibition of adipose tissue lipolysis, reduction of circulating levels of free fatty acids, and inhibition of low density lipoprotein production (23,24). Although metformin has a broad spectrum of effects, inhibition of mitochondrial complex I and activation of 5′ adenosine monophosphate-activated protein kinase (AMPK) appear to be major mechanisms of its action (25,26). Recent studies have shown that besides their ability to regulate cellular metabolism (27), metformin and other AMPK activators can decrease the severity of organ injury in acute inflammatory states (28), including LPS-induced liver injury or acute lung injury (29,30). Metformin, berberine or aminoimidazole carboxamide ribonucleotide (AICAR) were all shown to diminish activation of the tolllike receptor 4 (TLR4)/NF-κB signaling cascade, as well as to release of proin-flammatory mediators of neutrophils and macrophages, and also to enhance endothelial integrity in vitro and in models for sepsis (31, 32, 33, 34, 35, 36). In addition, metformin enhances host defense mechanisms by facilitating the chemotaxis and maturation of T cells (37,38). Besides its antiinflammatory actions, activated AMPK was recently shown to increase the phagocytic ability of macrophages (39). Although these studies revealed a beneficial effect of metformin in acute inflammatory conditions, there is little information concerning the ability of metformin or other AMPK activators to alter primary innate immune responses, and particularly bacterial eradication. In this study, we examined the hypothesis that AMPK activation may affect fundamental neutrophil functions, including chemotaxis and bacterial killing.

Materials and Methods

Mice

Male C57BL/6 mice were purchased from the National Cancer Institute-Frederick (Frederick, MD, USA). Male mice, 8 to 10 wks of age, were used for experiments. The mice were kept on a 12-h light:dark cycle with free access to food and water. All experiments were conducted in accordance with protocols approved by the University of Alabama at Birmingham Animal Care and Use Committee.

Reagents and Antibodies

W-peptide was purchased from Phoenix Pharmaceuticals (Burlingame, CA, USA). Metformin, berberine and IκB kinase (IKK) inhibitor PS-1145 were obtained from Sigma-Aldrich (St. Louis, MO, USA). Compound C and rapamycin were purchased from Calbiochem (La Jolla, CA, USA). Antibodies for phospho-Thr172-AMPK, total AMPK, phospho-Ser240/244-rpS6, total rpS6, 4E-BP1, and IκBα were purchased from Cell Signaling Technology (Danvers, MA, USA). β-actin antibody was from Santa Cruz Biotechnology (Santa Cruz, CA, USA). Custom antibody mixtures and negative selection columns for neutrophil isolation were obtained from Stem Cell Technologies (Vancouver, BC, Canada). Fluorescein isothiocyanate (FITC)-labeled E. coli, S. aureus and Alexa Fluor 594-conjugated phalloidin were from Invitrogen/Life Technologies (Carlsbad, CA, USA). Mounting oil solution containing DAPI was from Vector laboratories (Burlingame, CA, USA). The µ-slide for chemotaxis assay was obtained from Ibidi (Mt. Prospect, IL, USA); and transmigration chambers that we used are available from BD Biosciences (San Jose, CA, USA).

Neutrophil Isolation and Culture

Bone marrow neutrophils were isolated as described previously (31,40). Neutrophil purity was consistently greater than 97%, as determined by Wright-Giemsa-stained cytospin preparations. Neutrophils were cultured in RPMI 1640 medium containing 0.5% or 5% fetal bovine serum (FBS) and treated as indicated in the figure legends. Neutrophil viability under experimental conditions was determined using trypan blue staining and was consistently greater than 95%.

HL-60 Cell Culture and Differentiation

The HL-60 cell line was obtained from American Type Culture Collection and cultured in RPMI 1640 medium supplemented with 10% heat-inactivated FBS, penicillin (100 U/mL), streptomycin (25 µg/mL) and L-glutamine (1 mmol/L). To obtain differentiated cells, HL-60 cells were cultured in medium containing dimethyl sulfoxide (DMSO) (1.3%) for four consecutive days (41). Differentiated cells were then used for small interfering RNA (siRNA) treatment and IL-8 mediated chemotaxis.

siRNA Knockdown of AMPKα1

Differentiated HL-60 cells were incubated with specific siRNA (1 µmol/L) to AMPKα1, as described previously (41). Briefly, cells (3.5 × 106/well) in 12-well plates were incubated in Accell medium (serum free) containing siRNA (1 µmol/L) to AMPKα1 for 72 h. During incubation with siRNA, the cell culture medium was supplemented with 1.3% DMSO to maintain differentiation of the HL-60 cells. The cells were then subjected to Western blot analysis of AMPK or transwell migration assay.

Transwell Migration Assay

Transwell migration assay was performed using 24-well cell plate BD Falcon cell culture inserts (Translucent PET Membrane, BD Biosciences). Briefly, bone marrow neutrophils (106 cells/well) or differentiated HL-60 cells in 300 µL of RPMI 1640 medium (5% FBS) were added to the upper reservoir, whereas W-peptide or IL-8 in culture medium (800 µL) was placed in the lower reservoir of transmigration chamber. In all experiments, chemotaxis was determined after neutrophils or HL-60 cells were allowed to migrate for 60 min at 37°C followed by imaging the cells in the lower reservoir (41). Each condition was tested three or more times.

Measurement of Cell Velocity

Bone marrow neutrophils pretreated as described in figure legends and then loaded into the µ-slide for chemotaxis assay (Ibidi). Cell migration was initiated by inclusion of W-peptide (50 nmol/L) to create a concentration gradient. Migration was recorded by imaging cells with 1 min intervals for a total of 60 min and then distance and movement direction of individual cells were plotted to calculate speed and velocity.

Measurement Neutrophil Chemotaxis In Vivo

Mice were subjected to application of metformin (125 mg/kg of body weight; intraperitoneal [IP]) for 12 h and 2 h before IP injections of W-peptide (0.43 mg/kg). In additional experiments, mice were treated with compound C (3 mg/kg, IP) or vehicle (saline) for 2 h prior to application of W-peptide. After 6 h, mice were euthanized and peritoneal lavages obtained using 10 mL of RPMI 1640 medium (without serum).

Phagocytosis Assay

Phagocytosis of fluorescent labeled E. coli or S. aureus by neutrophils was performed as described previously (39). In brief, phagocytosis of fluorescently labeled bacteria by neutrophils pretreated with or without metformin (500 µmol/L, 2.5 h) was determined by adding tenfold excess of E. coli or S. aureus to the cells. To measure internalization of bacteria, fluorescent E. coli or S. aureus were incubated for 15 min at 37°C, and cells were then washed three times in ice-cold PBS. Next, cells were incubated with or without trypan blue solution (0.2% trypan blue, 20 mmol/L citrate, and 150 mmol/L NaCl, pH 4.5) for 1 min, then centrifuged, and the cell pellet was resuspended in PBS, and the amount of fluorescence was measured using flow cytometry.

In Vitro Killing-Activity Assay

Neutrophils (2 × 106 cells/mL) were incubated with ampicillin-resistant E. coli (2 x 107/mL) in RPMI medium without serum for 90 min at 37°C. Next, 20 µL of cell/bacterial suspension was incubated with 480 µL Triton X-100 (0.1%) for 10 min to lyse neutrophils. Serial dilutions were then plated on agar plates with ampicillin and incubated overnight at 37°C. The number of bacterial colonies on agar plates was determined using colony counter software (Bio-Rad, Hercules, CA, USA).

Peritonitis-Induced Sepsis

The efficiency of bacterial eradication in vivo was performed as described previously (42,43). Mice were subjected to administration of metformin (125 mg/kg of body weight; IP) for 12 h, compound C (3 mg/kg of body weight; IP) or vehicle (PBS) for 2 h before IP injection of ampicillin-resistant E. coli (2 × 108). After 6 h, mice were euthanized and peritoneal lavages obtained using 10 mL RPMI 1640 medium without serum. The number of surviving bacteria was determined by incubation of 95 µL of peritoneal lavages with 5 µL of Triton X-100 (1%) for 10 min to lyse cells, and then serial dilutions were placed on agar plates with ampicillin and incubated overnight at 37°C. Bacterial colonies were counted using colony counter software (Bio-Rad).

Imaging Actin in Neutrophils

Neutrophils were incubated with 4% paraformaldehyde in PBS for 30 min at room temperature then washed with PBS and permeabilized with 0.1% Triton X-100/PBS for 4 min. The cells were then incubated with 3% BSA in PBS for 1 h, followed by the addition of Alexa Fluor 594-conjugated phalloidin (25 µL/mL) for 20 min at room temperature. After the cells were washed with PBS, they were mounted with emulsion oil solution containing DAPI to visualize nuclei. Confocal microscopy was performed as described previously, using a Leica DMIRBE inverted epifluorescence/Nomarski microscope (Leica Microsystems, Wetzlar, Germany) outfitted with Leica TCS NT laser confocal optics (40).

Western Blot Analysis

Western Blot analysis was performed as described previously (44,45). Briefly, cell lysates of murine bone marrow neutrophils (3.5 × 106/well) were prepared using lysis buffer containing Tris pH 7.4 (50 mmol/L), NaCl (150 mmol/L), NP-40 (0.5%, vol/vol), EDTA (1 mmol/L), EGTA (1 mmol/L), okadaic acid (1 nmol/L) and protease inhibitors. Cell lysates were sonicated and then centrifuged at 10,000g for 15 min at 4°C to remove insoluble material. The protein concentration in the supernatants was determined using the Bradford reagent (BioRad) with BSA as a standard. Samples were mixed with Laemmli sample buffer and boiled for 15 min. Equal amounts of proteins were resolved by 8% to 12% sodium dodecyl sulfate-polyacrylamide gel electrophoresis, and transferred onto polyvinylidene fluoride (PVDF) membranes (Immobilon P; Millipore, Billerica, MA, USA). The membranes were probed with specific antibodies as described in the figure legends followed by detection with HRP-conjugated goat anti-rabbit IgG. Bands were visualized by enhanced chemiluminescence (Super Signal; Pierce Biotechnology, Rockford, IL, USA) and quantified by AlphaEaseFC software (Alpha Innotech, San Leandro, CA, USA). Each experiment was carried out two or more times using cell populations obtained from separate groups of mice.

Statistical Analysis

Statistical significance was determined by the Wilcoxon rank sum test (independent two-group Mann-Whitney U test) as well as Student t test for comparisons between two groups. Multigroup comparisons were performed using one-way analysis of variance (ANOVA) with Tukey post hoc test. A value of P less than 0.05 was considered significant. Analyses were performed on SPSS version 16.0 (IBM, Armonk, NY, USA) for Windows (Microsoft Corporation, Redmond, WA, USA).

Results

Effects of AMPK Inhibition or Activation on Neutrophil Chemotaxis

In initial experiments, mouse neutrophil chemotaxis was determined using W-peptide, a mouse homolog of human IL-8. As shown in Figures 1AC, W-peptide enhanced, in a dose- and time-dependent manner, neutrophil migration in transmigration chambers. To determine if neutrophil chemotaxis affected AMPK activation, neutrophils were incubated with W-peptide for 0, 20, 40 or 60 min and the amounts of total and phosphorylated AMPK were determined using Western blot analysis. As shown in Figure 1D, transient activation of AMPK was detected in neutrophils 20 min after exposure to W-peptide. Similar to the effects of W-peptide, enhanced chemotaxis and activation of AMPK was found in IL-8-treated HL-60 cells, a differentiated human neutrophil-like cell line (Figures 1E, F) (41).
Figure 1

Effects of metformin or AMPK inhibitor compound C on neutrophil Chemotaxis. (A, B, C) Representative images (A) and quantitative data (B, C) show neutrophil migration after dose- and time-dependent stimulation with W-peptide. In (B), transmigration assay was performed by inclusion of W-peptide (0),12.5, 25 or 50 nmol/L) for 60 min, whereas, in (C), migration was determined after inclusion of 50 nmol/L W-peptide for the indicated time period. Means ± SD (n = 3), ***P < 0.001, compared with untreated neutrophils. (D) Representative Western Blots and quantitative data show the amount of phosphorylated and total AMPK in neutrophils treated with W-peptide (50 nmol/L) for 0, 20, 40 or 60 min. Average (mean ± SEM) of optical bend density was obtained from three independent experiments (*P < 0.05, compared with untreated). (E, F) HL-60 cells were treated with IL-8 for 60 min followed by chemotaxis assay (E) and Western Blot analysis (F) for phospho and total AMPK. Means ± SD (n = 3), *P< 0.05, **P< 0.01, ***P< 0.001, compared with untreated cells.

To evaluate the effects of AMPK activation on neutrophil chemotaxis, assays were performed using neutrophils that were left untreated (control) or that were incubated with the AMPK inhibitor compound C. Compound C dose dependently inhibited neutrophil chemotaxis (Figures 2A, B). Additional experiments using the AMPK activators metformin or berberine demonstrated that exposure of neutrophils to such compounds resulted in enhanced chemotaxis (Figure 2C). The confirmatory experiments also were performed using control (scrambled) and specific siRNA to diminish expression of AMPKα1. As shown in Figures 2D and 2E, siRNA mediated knockdown of AMPKα1 resulted in significant decrease in HL-60 chemotaxis. Although metformin and berberine stimulated AMPK activation and neutrophil motility, AICAR did not increase chemotaxis (data not shown) likely due to effects mediated by enzymatically produced ZMP in the AICAR-treated cells (46, 47, 48).
Figure 2

Effects of AMPK activation or inhibition on neutrophil chemotaxis. Neutrophils were pretreated with compound C (0), 1,2,3 or 10 µmol/L) for 60 min, metformin (500 µmol/L) or berberine (10 µmol/L) for 2.5 h and then chemotaxis was measured after inclusion of cells in transmigration chambers and exposure to W-peptide for 60 min. (A) Representative images show amount of control (untreated) or compound C-treated (30 µmol/L) neutrophils that migrated into the lower reservoir. Panel (B) shows dose-dependent inhibition by compound C, whereas (C) metformin exposure or berberine exposure enhanced neutrophil chemotaxis. Means ± SD (n = 3), *P < 0.05, compared with control. Lower panels B or C show Western blots of phospho AMPK, total AMPK and actin obtained from neutrophils treated with compound C (10 µmol/L) for 60 min, metformin (500 µmol/L) for 2.5 h, or berberine (10 µmol/L) for 2.5 h. (D) Chemotaxis assays were performed in control (untreated) cells and cells treated with control (scrambled siRNA) or specific siRNA to AMPKα1 subunit. (E) Representative Western blots show amounts of AMPKα1 and actin before and after treatment with scrambled or siRNA to AMPKα1. ctr, Control; met, metformin; ber, berberine; scr., scrambled.

AMPK Activation Prevents LPS-Induced Inhibition of Chemotaxis

Previous studies have shown that engagement of TLR4 diminished IL-8-dependent chemotaxis of human neutrophils (49). Similar to the previously reported results, we found that exposure of mouse bone marrow neutrophils to LPS also resulted in inhibition of neutrophil chemotaxis (Figures 3A, B). Western blot analysis showed that inhibition of neutrophil chemotaxis was associated with dose- and time-dependent decrease in LPS-induced AMPK phosphorylation (Figures 3C, D). To further determine the relationship between LPS and AMPK, neutrophils were treated with AICAR before or after exposure to LPS. As shown in Figures 3E and 4F, the addition of AICAR to the cell cultures, at either pre- or postexposure to LPS, was able to increase activity of AMPK.
Figure 3

Exposure to LPS diminished neutrophil chemotaxis and AMPK phosphorylation. (A) Representative images show neutrophil transmigration before and after treatment with LPS. Neutrophils were treated with LPS (0 or 1 µg/mL) for 90 min. The cells were then washed and chemotaxis examined over a 60 min period. In (B), neutrophils were incubated with LPS for 90 min followed by measurement of neutrophil chemotaxis. (C, D) Representative Western blots and quantitative data show the amounts of phosphorylated and total AMPK obtained from neutrophils treated with LPS (0-1,000 ng/mL) for 90 min (C) or after exposure to LPS (300 ng/mL) for the indicated time periods (D). Means ± SEM (n = 3), *P< 0.05. (E, F) LPS suppresses activation of AMPK. Representative Western Blots and quantitative data show amounts of phospho and total AMPK, and actin. Neutrophils were treated with AICAR (0 or 250 µmol/L) for 60 min and then cultured with LPS (0 or 300 ng/mL) for an additional 60 min. Cells also were treated with LPS (300 ng/mL) for 60 min followed by inclusion of AICAR (250 µmol/L) in the cultures for an additional 60 min. Means ± SD, n = 3, *P< 0.05, compared with neutrophils treated with LPS alone. ctr, Control; AIC, AICAR.

Because metformin-induced activation of AMPK was shown to diminish LPS-mediated neutrophil proinflammatory activation (31), we hypothesized that there might be similar effects of AMPK activation in preventing the inhibitory effects of LPS on chemotaxis. As shown in Figure 4A, incubation of neutrophils with metformin and LPS significantly improved chemotaxis as compared with that found when neutrophils were treated with LPS alone. Metformin increased neutrophil chemotaxis when included in the cell cultures before or after exposure of the cells to LPS. In additional experiments, the effects of metformin on LPS-associated diminishment of neutrophil velocity were determined using µ-slide for chemotaxis assay. As shown in Figures 4B and 4C, metformin increased neutrophil velocity and also prevented neutrophil immobilization after exposure to LPS. In contrast, treatment of LPS-exposed neutrophils with the AMPK inhibitor compound C resulted in significant inhibition of neutrophil chemokinesis.
Figure 4

Metformin diminished LPS-induced inhibition of neutrophil chemotaxis. (A) Neutrophils were treated with metformin (met; 0 or 500 µmol/L) for 90 min and then LPS (0 or 300 ng/mL) for 60 min, or cells were first treated with LPS (300 ng/mL) for 60 min followed by inclusion of metformin (500 µmol/L) in the cultures for an additional 90 min. Neutrophil chemotaxis was then examined. Means ± SD, n = 3, *P < 0.05, **P < 0.01 compared with neutrophils treated with LPS alone. (B) Representative images show direction and distance (length of arrows) passed by the neutrophils a pretreated with metformin, LPS, compound C or combination of metformin and LPS. Panel (C) shows neutrophil velocity. Mean ± SEM, n ≥ 20, *P < 0.05, **P < 0.01 compared with control, *P < 0.001 compared with metformin and §P < 0.001 compared with LPS alone. Large arrow indicates direction to W-peptide. (D, E). Metformin stimulates, whereas compound C diminishes neutrophil chemotaxis in vivo. Panel (D) shows time line administration of metformin (125 mg/kg; IP), compound C (3 mg/kg; IP), PBS (200 µL; IP) or W-peptide (0.43 mg/kg; IP) followed by acquisition of peritoneal neutrophils. Panel (E) shows amount of peritoneal neutrophils obtained from mice treated as indicated in (D). Mean ± SEM (n ≥ 3). *P< 0.05, compared control or mice treated with compound C. ctr, Control; met or Met., metformin; W-pep, W-peptide; com. C, compound C.

Given our in vitro results showing that AMPK activation modulated neutrophil chemotaxis, we determined if activation or inhibition of AMPK can affect neutrophil chemotaxis in vivo. To examine this possibility, control mice or mice treated with metformin or compound C were then given an IP injection of W-peptide and the number of neutrophils migrating into the peritoneum was measured 5 h later (Figure 4D). As shown in Figure 4E, treatment with metformin before application of W-peptide was associated with an increased number of peritoneal neutrophils as compared with treatment with W-peptide alone. In contrast to metformin, administration of compound C diminished W-peptide-induced peritoneal accumulation of neutrophils.

AMPK Activation Facilitates Neutrophil-Dependent Bacterial Uptake and Killing

Although our experiments found that treatment with the AMPK activator metformin or the AMPK inhibitor compound C significantly affect neutrophil chemotaxis, the effects of AMPK activation on bacterial killing were not determined. In addition to the generation of ROS, phagocytosis is central in bacterial eradication. To measure phagocytosis, control (untreated) neutrophils or neutrophils treated with metformin or compound C were incubated with fluorescein isothiocyanate (FITC)-tagged E. coli or S. aureus and then subjected to flow cytometry. As shown in Figures 5A and 5B, pretreatment with metformin increased the ability of neutrophils to phagocyte bacteria. Next, we determined if activation or inhibition of AMPK can affect bacterial killing. To examine this possibility, neutrophils were left untreated or were incubated with metformin, AICAR or compound C. As shown in Figures 5C and 5D, both metformin and AICAR increased, whereas compound C diminished, bacterial killing. Results obtained from bacterial killing assays showed that a modest increase in the amount of bacteria was recovered after incubation of neutrophils with LPS (Figures 5C, D).
Figure 5

Metformin increases bacteria uptake and killing in vitro and in vivo. (A, B). Neutrophils (106 cells/mL) were pretreated with or without metformin (500 µmol/L) for 2.5 h and then incubated with fluorescently tagged E. coli(107/mL) (A) or S. aureus (107/mL) (B) for additional 20 min. Neutrophil-dependent uptake of bacteria was determined using flow cytometry. Means ± SEM (n = 3), *P < 0.05 or **P < 0.01. (C, D) Neutrophils (2 × 106 cells/mL) were pretreated with metformin (0 or 500 µmol/L) for 2.5 h, AICAR (0 or 250 µmol/L) for 2 h, LPS (1 µg/mL), compound C (10 µmol/L) or rapamycin (10 nmol/L) for 60 min. Next, neutrophils were incubated with E. coli (2 × 107/mL) for 90 min. Images (C) show agar plates with colonies formed by viable E. coli that were obtained after incubating bacteria with neutrophils. Panel (D) shows the number of viable bacteria recovered from killing assay. Means ± SEM (n = 4), *P < 0.05 compared with control. (E, F, G) Mice were subjected to the administration of metformin (125 mg/kg; IP) for 12 h, compound C (3 mg/kg; IP), or vehicle (0.9% saline) for 2 h followed by IP injection of E. coli (2 × 108) for an additional 6 h. (E) Representative images showed the number of E. coli colonies formed from viable bacteria that were recovered from peritoneal lavages. (F, G) Average of viable bacteria (F) and neutrophils (G) obtained from peritoneal lavages (mean ± SEM, n ≥ 5). *P < 0.05, **P < 0.01. RFU, relative fluorescence unit; ctr, control; met, metformin; CFU, colony-forming unit; com. C, compound C.

Previous studies have shown that signaling cascades downstream of AMPK activates regulation of mTORC1. Therefore, in additional experiments, neutrophils were treated with the specific mTOR inhibitor rapamycin. However, rapamycin exposure did not affect the ability of neutrophils to eradicate bacteria (see Figures 5C, D).

AMPK Activation Enhances Bacterial Killing in Peritonitis-Induced Sepsis

Considering our in vitro results that AMPK activation with metformin increased neutrophil chemotaxis, as well as enhanced uptake and killing bacteria in vitro, we determined if metformin treatment can improve bacterial clearance in vivo. This possibility was examined using a murine model for peritonitis-induced sepsis (42,43). As shown in Figures 5E and 5F, there were significant decreases in the numbers of viable bacteria recovered from mice that received metformin as compared with controls. Of note, the number of peritoneal neutrophils was found to be increased, compared with the control group (Figure 5G).

AMPK Activation Stimulates Actin Rearrangement, Neutrophil Leading Edge Formation, and Diminishes LPS/TLR4-Mediated Inhibition of Neutrophil Chemotaxis

Although our experiments demonstrated that AMPK activation enhanced neutrophil chemotaxis and bacterial killing, the mechanism responsible for such effects was not delineated. AMPK activation induced by cellular exposure to metformin or AICAR results in cytoskeletal rearrangement (17). As shown in Figure 6, whereas significant decrease in the level of actin polymerization was found in LPS-treated neutrophils, such inhibitory effects of LPS were prevented by exposure of the neutrophils to metformin or AICAR. As shown in Figures 7A and 7B, inclusion of metformin or AICAR effectively diminished LPS-induced IκBα degradation. Of note, pretreatment with the specific IKK inhibitor PS-1145 also resulted in inhibition of IκBα degradation as well as prevented neutrophil immobilization by LPS (Figures 7CE). Although mTORC1 activation is essential for the enhancement of the proinflammatory properties of LPS-treated neutrophils, metformin did not affect LPS-mediated phosphorylation of rpS6 (Figure 7F). Of note, inclusion of rapamycin diminished mTORC1 activation (Figures 7G, H).
Figure 6

AMPK activation induces neutrophil cytoskeletal rearrangement and leading edge formation. Neutrophils were pretreated with AICAR (0 or 250 µmol/L) for 90 min or metformin (0 or 500 µmol/L) for 2.5 h followed by inclusion of LPS (0 or 1 µg/mL) for additional 90 min. (A,B) Representative images show actin (green) and nuclei (blue) staining (A), whereas (B) shows magnified region of interest. (C) Average of actin fluorescence is shown. Mean ± SD actin fluorescence intensity (n < 3 ∼ 5), *P < 0.05.

Figure 7

Effects of metformin, AICAR and IKK inhibitor on LPS-dependent activation of TLR4 or mTOR signaling pathways. Neutrophils were cultured with AICAR (0 or 500 µmol/L) for 2.5 h, metformin (0 or 500 µmol/L) for 2.5 h, IKK inhibitor PS-1145 (0 or 10 µmol/L) for 60 min or rapamycin (0 or 30 nmol/L) for 30 min. Next, neutrophils were cultured with LPS (0 or 300 ng/mL) for an additional 60 min. (A, C, F, G) Representative Western blots show amount of IκBα, total and phosphorylated ribosomal protein S6 (rpS6) (Ser240/244), 4E-binding protein 1 (4E-BP1), and actin. Panels (B, D, F and H) show average of Western blots optical bend densitometry. Means ± SEM (n = 3); (B, D) *P < 0.05, **P < 0.01 compared with LPS only; (F) **P< 0.01 compared with control (untreated); (H) **P< 0.01 compared with control (untreated), LPS or rapamycin- and LPS-treated cells. Panel (E) shows the ability of IKK inhibitor PS-1145 to prevent LPS-mediated inhibition of neutrophil chemotaxis.

Discussion

In the present studies, we found that activation of AMPK enhanced neutrophil chemotaxis and bacterial uptake, both essential components of bacterial killing. Recent studies, including results obtained from our laboratory (39), have shown that metformin or other AMPK activators enhance cell mobility and also phagocytosis. For example, AMPK activation was associated with enhanced T cell chemotaxis or migration of epithelial cells (38,50). AMPK activation has also been shown to enhance the phagocytic ability of macrophages, including uptake of bacteria, synthetic beads or apoptotic cells (39). These results are consistent with an ability of activated AMPK to facilitate microbial eradication through mechanisms that involve enhancement of neutrophil chemotaxis and/or bacterial uptake. Consistent with these previously reported findings, our present in vivo results showed that metformin effectively improved bacterial killing in vivo.

Severe sepsis is characterized by alterations in immunologic and host defense functions that include downregulation of neutrophil chemotaxis and phagocytosis (2,16,17,51,52). Because AMPK activation in metformin-treated neutrophils prevented LPS-mediated inhibition of chemotaxis, it is possible that metformin treatment may preserve neutrophil chemotaxis in the setting of sepsis and facilitate the ability of the host to clear invading pathogens. Our results showed that metformin can reverse the inhibitory actions of LPS on chemotaxis, and also prevent LPS-induced degradation of IκBα. Of note, exposure of neutrophils to the IKK inhibitor PS-1145 (53,54) also diminished IκBα degradation and prevented inhibition of neutrophil chemotaxis by LPS, suggesting that the effects of AMPK activation in this setting may also be due to its ability to inhibit IκBα degradation. Although previous studies have shown that metformin and other AMPK activators are capable of inhibiting mTORC1 function (55,56), in the present experiments, exposure of neutrophils to metformin did not prevent LPS-dependent activation of mTOR. These results suggest that AMPK activation enhances neutrophil chemotaxis through mechanisms that involve suppression of TLR4-associated signaling pathways other than those involving mTOR. Although our results suggest that AMPK activation has beneficial effects on neutrophil function related to microbial clearance, it will be important to determine how AMPK activation affects such functions in additional cell populations, and also if AMPK activation can restore the diminished monocyte and T cell responses frequently found in sepsis (57).

Previous studies and results obtained from our laboratory have described antiinflammatory effects mediated by activated AMPK. Metformin, AICAR or berberine all were shown to diminish neutrophil and macrophage proinflammatory activation, as well as to decrease the severity of endotoxin- or ventilator-induced acute lung injury (29,31,58). Exposure of macrophages to antiinflammatory mediators, such as IL-10 or TGF-β, resulted in activation of AMPK followed by transition of the cells from the M1 to M2 phenotype (33). Recent studies have shown that activated AMPK can also modulate the resolution of inflammatory conditions due to enhancement of the phagocytic ability of macrophages and neutrophils. In particular, AMPK activation increased the uptake of bacteria and enhanced efferocytosis, an essential process in the resolution of inflammation in which apoptotic cells are ingested and cleared by phagocytic cells (39,59,60). Beneficial effects of AMPK activation also were related to improvement of vascular integrity in mice models for endotoxemia-induced ALI and to airway remodeling in asthma (34,61). In experimental models of diabetes, endothelial barrier function was preserved through mechanisms involving activation of AMPK (62).

Recent studies have shown that AMPK phosphorylation was diminished upon exposure of cells to LPS. In particular, culture with LPS significantly decreased AMPK activity in neutrophils, peritoneal macrophages, Raw 264.7 cells, and endothelial cells (33,34,45,63,64). The combination of LPS and saturated fatty acid palmitate also was shown to induce prolonged inactivation of AMPK in bone marrow macrophages (65). Our present results indicate that in spite of inhibitory action of LPS, inclusion of AICAR or metformin was able to partially increase AMPK phosphorylation, even when included in cultures after cellular exposure to LPS (Figure 3) (45).

Bacterial dissemination leading to multiorgan injury contributes to the high mortality rate associated with sepsis (10,11,19). Whereas many patients survive the initial stages of sepsis, many will develop later clinical complications including nosocomial infections that lead to prolonged hospitalization. In spite of improved understanding of the mechanisms responsible for complications in sepsis, pharmacological approaches to prevent secondary infection and decrease morbidity and mortality associated with late infection have not been well characterized (57). Metformin is approved for use in patients with diabetes with a well-established safety profile and known side effects and, for these reasons, may be considered for examination as a therapeutic approach in clinical trials of patients with sepsis. Although the early use of antibiotics is beneficial during sepsis, microbial products, as well as hostderived danger associated molecular pattern molecules (DAMPs) are still frequently present in the circulation and are likely to contribute to organ system dysfunction (66,67). For example, release of HMGB1, histones and mitochondrial proteins are known to increase the severity of acute inflammatory conditions and intensify the immunosuppressed state characteristic of late sepsis (66, 67, 68, 69, 70, 71). Of note, AMPK activators, including metformin, were shown to diminish acute inflammatory injury of lung or liver as well as decrease the release of DAMPs and improve mortality in experimental models of LPS-induced sepsis (5,29,36). Although antibiotics are sufficient to kill bacteria, the combination of metformin and antibiotics may have additional benefit in sepsis, particularly as metforminstimulated neutrophils have increased chemotaxis and bacterial uptake.

Disclosure

The authors declare that they have no competing interests as defined by Molecular Medicine, or other interests that might be perceived to influence the results and discussion reported in this paper.

Notes

Acknowledgments

This work was supported in part by National Institutes of Health Grants GM87748 and HL107585 to JW Zmijewski and NIH P30 AR 48311 to The Flow Cy-tometry Core, Arthritis and Muscu-loskeletal Center UAB. We thank Anna A Zmijewska and Enid Keyser for technical support.

References

  1. 1.
    Stuart LM, Ezekowitz RA. (2008) Phagocytosis and comparative innate immunity: learning on the fly. Nat. Rev. Immunol. 8:131–41.CrossRefGoogle Scholar
  2. 2.
    Phillipson M, Kubes P. (2011) The neutrophil in vascular inflammation. Nat. Med. 17:1381–90.CrossRefPubMedGoogle Scholar
  3. 3.
    Foxman EF, Campbell JJ, Butcher EC. (1997) Multistep navigation and the combinatorial control of leukocyte chemotaxis. J. Cell Biol. 139:1349–60.CrossRefGoogle Scholar
  4. 4.
    Williams MR, Azcutia V, Newton G, Alcaide P, Luscinskas FW. (2011) Emerging mechanisms of neutrophil recruitment across endothelium. Trends Immunol. 32:461–9.CrossRefPubMedPubMedCentralGoogle Scholar
  5. 5.
    Lambeth JD. (2004) NOX enzymes and the biology of reactive oxygen. Nat. Rev. Immunol. 4:181–9.Google Scholar
  6. 6.
    Hampton MB, Kettle AJ, Winterbourn CC. (1998) Inside the neutrophil phagosome: oxidants, myeloperoxidase, and bacterial killing. Blood. 92:3007–17.PubMedGoogle Scholar
  7. 7.
    Brinkmann V, et al. (2004) Neutrophil extracellular traps kill bacteria. Science. 303:1532–5.CrossRefGoogle Scholar
  8. 8.
    Papayannopoulos V, Zychlinsky A. (2009) NETs: a new strategy for using old weapons. Trends Immunol. 30:513–21.CrossRefPubMedGoogle Scholar
  9. 9.
    Brown KA, et al. (2006) Neutrophils in development of multiple organ failure in sepsis. Lancet. 368:157–69.CrossRefPubMedGoogle Scholar
  10. 10.
    Vincent JL, Abraham E. (2006) The last 100 years of sepsis. Am. J. Respir. Crit. Care Med. 173:256–63.CrossRefPubMedGoogle Scholar
  11. 11.
    van der Poll T, Opal SM. (2008) Host-pathogen interactions in sepsis. Lancet Infect. Dis. 8:32–43.CrossRefPubMedGoogle Scholar
  12. 12.
    Muller LM, et al. (2005) Increased risk of common infections in patients with type 1 and type 2 diabetes mellitus. Clin. Infect. Dis. 41:281–8.CrossRefPubMedGoogle Scholar
  13. 13.
    Abraham E. (2003) Neutrophils and acute lung injury. Crit. Care Med. 31: S195–9.CrossRefPubMedGoogle Scholar
  14. 14.
    Chaudry IH, Ayala A. (1993) Mechanism of increased susceptibility to infection following hemorrhage. Am. J. Surg. 165:59S–67S.CrossRefPubMedGoogle Scholar
  15. 15.
    Stephan RN, Kupper TS, Geha AS, Baue AE, Chaudry IH. (1987) Hemorrhage without tissue trauma produces immunosuppression and enhances susceptibility to sepsis. Arch. Surg. 122:62–8.CrossRefPubMedGoogle Scholar
  16. 16.
    Alves-Filho JC, de Freitas A, Russo M, Cunha FQ. (2006) Toll-like receptor 4 signaling leads to neutrophil migration impairment in polymicrobial sepsis. Crit. Care Med. 34:461–70.CrossRefPubMedGoogle Scholar
  17. 17.
    Arraes SM, et al. (2006) Impaired neutrophil chemotaxis in sepsis associates with GRK expression and inhibition of actin assembly and tyrosine phosphorylation. Blood. 108:2906–13.CrossRefPubMedGoogle Scholar
  18. 18.
    Tavares-Murta BM, et al. (2002) Failure of neutrophil chemotactic function in septic patients. Crit. Care Med. 30:1056–61.CrossRefPubMedGoogle Scholar
  19. 19.
    Alves-Filho JC, de Freitas A, Spiller F, Souto FO, Cunha FQ. (2008) The role of neutrophils in severe sepsis. Shock. 30 Suppl 1:3–9.CrossRefPubMedGoogle Scholar
  20. 20.
    Rios-Santos F, et al. (2007) Down-regulation of CXCR2 on neutrophils in severe sepsis is mediated by inducible nitric oxide synthase-derived nitric oxide. Am. J. Respir. Crit. Care Med. 175:490–7.CrossRefPubMedGoogle Scholar
  21. 21.
    Benjamim CF, et al. (2002) Inhibition of leukocyte rolling by nitric oxide during sepsis leads to reduced migration of active microbicidal neutrophils. Infect. Immun. 70:3602–10.CrossRefPubMedPubMedCentralGoogle Scholar
  22. 22.
    Bailey CJ, Turner RC. (1996) Metformin. N. Engl. J. Med. 334:574–9.CrossRefPubMedGoogle Scholar
  23. 23.
    Saenz A, et al. (2005) Metformin monotherapy for type 2 diabetes mellitus. Cochrane Database Syst. Rev. 3:CD002966.Google Scholar
  24. 24.
    Wulffele MG, Kooy A, de Zeeuw D, Stehouwer CD, Gansevoort RT. (2004) The effect of metformin on blood pressure, plasma cholesterol and triglycerides in type 2 diabetes mellitus: a systematic review. J. Intern. Med. 256:1–14.CrossRefPubMedGoogle Scholar
  25. 25.
    El-Mir MY, et al. (2000) Dimethylbiguanide inhibits cell respiration via an indirect effect targeted on the respiratory chain complex I. J. Biol. Chem. 275:223–8.CrossRefPubMedGoogle Scholar
  26. 26.
    Hawley SA, Gadalla AE, Olsen GS, Hardie DG. (2002) The antidiabetic drug metformin activates the AMP-activated protein kinase cascade via an adenine nucleotide-independent mechanism. Diabetes. 51:2420–5.CrossRefPubMedGoogle Scholar
  27. 27.
    Hardie DG, Ross FA, Hawley SA. (2012) AMPK: a nutrient and energy sensor that maintains energy homeostasis. Nat. Rev. Mol. Cell Biol. 13:251–62.CrossRefPubMedPubMedCentralGoogle Scholar
  28. 28.
    O’Neill LA, Hardie DG. (2013) Metabolism of inflammation limited by AMPK and pseudostarvation. Nature. 493:346–55.CrossRefPubMedGoogle Scholar
  29. 29.
    Zhao X, et al. (2008) Activation of AMPK attenuates neutrophil proinflammatory activity and decreases the severity of acute lung injury. Am. J. Physiol. Lung Cell Mol. Physiol. 295:L497–504.CrossRefPubMedPubMedCentralGoogle Scholar
  30. 30.
    Bergheim I, et al. (2006) Metformin prevents endotoxin-induced liver injury after partial hepatectomy. J. Pharmacol. Exp. Ther. 316:1053–61.CrossRefPubMedGoogle Scholar
  31. 31.
    Zmijewski JW, et al. (2008) Mitochondrial respiratory complex I regulates neutrophil activation and severity of lung injury. Am. J. Respir. Crit. Care Med. 178:166–79.CrossRefGoogle Scholar
  32. 32.
    Hattori Y, Suzuki K, Hattori S, Kasai K. (2006) Metformin inhibits cytokine-induced nuclear factor kappaB activation via AMP-activated protein kinase activation in vascular endothelial cells. Hypertension. 47:1183–8.CrossRefPubMedGoogle Scholar
  33. 33.
    Sag D, Carling D, Stout RD, Suttles J. (2008) Adenosine 5′-monophosphate-activated protein kinase promotes macrophage polarization to an anti-inflammatory functional phenotype. J. Immunol. 181:8633–41.CrossRefPubMedPubMedCentralGoogle Scholar
  34. 34.
    Xing J, et al. (2013) Inhibition of AMP-activated protein kinase accentuates lipopolysaccharide-in-duced lung endothelial barrier dysfunction and lung injury in vivo. Am. J. Pathol. 182:1021–30.CrossRefPubMedPubMedCentralGoogle Scholar
  35. 35.
    Jeong HW, et al. (2009) Berberine suppresses proinflammatory responses through AMPK activation in macrophages. Am. J. Physiol. Endocrinol. Metab. 296:E955–64.CrossRefPubMedGoogle Scholar
  36. 36.
    Tsoyi K, et al. (2011) Metformin inhibits HMGB1 release in LPS-treated RAW 264.7 cells and increases survival rate of endotoxaemic mice. Br. J. Pharmacol. 162:1496–508.CrossRefGoogle Scholar
  37. 37.
    Pearce EL, et al. (2009) Enhancing CD8 T-cell memory by modulating fatty acid metabolism. Nature. 460:103–7.CrossRefPubMedPubMedCentralGoogle Scholar
  38. 38.
    Chan O, Burke JD, Gao DF, Fish EN. (2012) The chemokine CCL5 regulates glucose uptake and AMP kinase signaling in activated T cells to facilitate chemotaxis. J. Biol. Chem. 287:29406–16.CrossRefPubMedPubMedCentralGoogle Scholar
  39. 39.
    Bae HB, et al. (2011) AMP-activated protein kinase enhances the phagocytic ability of macrophages and neutrophils. Faseb. J. 25:4356–68.CrossRefGoogle Scholar
  40. 40.
    Zmijewski JW, et al. (2009) Antiinflammatory effects of hydrogen peroxide in neutrophil activation and acute lung injury. Am. J. Respir. Crit. Care Med. 179:694–704.CrossRefPubMedPubMedCentralGoogle Scholar
  41. 41.
    Millius A, Weiner OD. (2009) Chemotaxis in neutrophil-like HL-60 cells. Methods Mol. Biol. 571:167–77.CrossRefPubMedPubMedCentralGoogle Scholar
  42. 42.
    Renckens R, et al. (2006) Endogenous tissue-type plasminogen activator is protective during Escherichia coli-induced abdominal sepsis in mice. J. Immunol. 177:1189–96.CrossRefPubMedGoogle Scholar
  43. 43.
    Tadie JM, Bae HB, Banerjee S, Zmijewski JW, Abraham E. (2012) Differential activation of RAGE by HMGB1 modulates neutrophil-associated NADPH oxidase activity and bacterial killing. Am. J. Physiol. Cell Physiol. 302:C249–56.CrossRefPubMedGoogle Scholar
  44. 44.
    Zmijewski JW, et al. (2010) Exposure to hydrogen peroxide induces oxidation and activation of AMP-activated protein kinase. J Biol. Chem. 285:33154–64.CrossRefPubMedPubMedCentralGoogle Scholar
  45. 45.
    Tadie JM, et al. (2012) Toll-like receptor 4 engagement inhibits adenosine 5′-monophosphate-activated protein kinase activation through a high mobility group box 1 protein-dependent mechanism. Mol. Med. 18:659–68.CrossRefPubMedPubMedCentralGoogle Scholar
  46. 46.
    Sullivan JE, et al. (1994) Inhibition of lipolysis and lipogenesis in isolated rat adipocytes with AICAR, a cell-permeable activator of AMP-activated protein kinase. FEBS Lett. 353:33–36.CrossRefPubMedGoogle Scholar
  47. 47.
    Elferink JG, de Koster BM. (2000) Inhibition of in-terleukin-8-activated human neutrophil chemotaxis by thapsigargin in a calcium- and cyclic AMP-dependent way. Biochem. Pharmacol. 59:36975.CrossRefGoogle Scholar
  48. 48.
    Elferink JG, de Koster BM, Boonen GJ, de Priester W. (1992) Inhibition of neutrophil chemotaxis by purinoceptor agonists. Arch. Int. Pharmacodyn. Ther. 317:93–106.PubMedGoogle Scholar
  49. 49.
    Hayashi F, Means TK, Luster AD. (2003) Toll-like receptors stimulate human neutrophil function. Blood. 102:2660–9.CrossRefPubMedGoogle Scholar
  50. 50.
    Nakano A, et al. (2010) AMPK controls the speed of microtubule polymerization and directional cell migration through CLIP-170 phosphorylation. Nat. Cell Biol. 12:583–90.CrossRefPubMedGoogle Scholar
  51. 51.
    Taneja R, Sharma AP, Hallett MB, Findlay GP, Morris MR. (2008) Immature circulating neutrophils in sepsis have impaired phagocytosis and calcium signaling. Shock. 30:616–22.CrossRefGoogle Scholar
  52. 52.
    Duignan JP, Collins PB, Johnson AH, Bouchier-Hayes D. (1986) The association of impaired neutrophil chemotaxis with postoperative surgical sepsis. Br. J. Surg. 73:236–40.CrossRefGoogle Scholar
  53. 53.
    Yemelyanov A, et al. (2006) Effects of IKK inhibitor PS1145 on NF-kappaB function, proliferation, apoptosis and invasion activity in prostate carcinoma cells. Oncogene. 25:387–98.CrossRefPubMedGoogle Scholar
  54. 54.
    Cilloni D, et al. (2006) The NF-kappaB pathway blockade by the IKK inhibitor PS1145 can overcome imatinib resistance. Leukemia. 20:61–7.CrossRefPubMedGoogle Scholar
  55. 55.
    Bolster DR, Crozier SJ, Kimball SR, Jefferson LS. (2002) AMP-activated protein kinase suppresses protein synthesis in rat skeletal muscle through down-regulated mammalian target of rapamycin (mTOR) signaling. JBiol. Chem. 277:23977–80.CrossRefGoogle Scholar
  56. 56.
    Inoki K, Kim J, Guan KL. (2012) AMPK and mTOR in cellular energy homeostasis and drug targets. Annu. Rev. Pharmacol. Toxicol. 52:381–400.CrossRefPubMedGoogle Scholar
  57. 57.
    Gentile LF, et al. (2012) Persistent inflammation and immunosuppression: a common syndrome and new horizon for surgical intensive care. J. Trauma Acute Care Surg. 72:1491–501.CrossRefPubMedPubMedCentralGoogle Scholar
  58. 58.
    Tsaknis G, et al. (2012) Metformin attenuates ventilator-induced lung injury. Crit. Care. 16:R134.CrossRefPubMedPubMedCentralGoogle Scholar
  59. 59.
    Labuzek K, Liber S, Gabryel B, Adamczyk J, Okopien B. (2010) Metformin increases phagocytosis and acidifies lysosomal/endosomal compartments in AMPK-dependent manner in rat primary microglia. Naunyn Schmiedebergs Arch. Pharmacol. 381:171–86.CrossRefPubMedGoogle Scholar
  60. 60.
    Jiang S, et al. (2013) Mitochondria and AMP-activated protein kinase-dependent mechanism of efferocytosis. J Biol. Chem. 288:26013–26.CrossRefPubMedPubMedCentralGoogle Scholar
  61. 61.
    Park CS, et al. (2012) Metformin reduces airway inflammation and remodeling via activation of AMP-activated protein kinase. Biochem. Pharmacol. 84:1660–70.CrossRefPubMedGoogle Scholar
  62. 62.
    Li FY, et al. (2012) Endothelium-selective activation of AMP-activated protein kinase prevents diabetes mellitus-induced impairment in vascular function and reendothelialization via induction of heme oxygenase-1 in mice. Circulation. 126:1267–77.CrossRefPubMedGoogle Scholar
  63. 63.
    Yang Z, Kahn BB, Shi H, Xue BZ. Macrophage alpha1 AMP-activated protein kinase (alpha1AMPK) antagonizes fatty acid-induced inflammation through SIRT1. J. Biol. Chem. 285:19051–9.Google Scholar
  64. 64.
    Ji G, et al. (2012) Genistein suppresses LPS-induced inflammatory response through inhibiting NF-kappaB following AMP kinase activation in RAW 264.7 macrophages. PLoS ONE. 7:e53101.CrossRefPubMedPubMedCentralGoogle Scholar
  65. 65.
    Wen H, etal. (2011) Fatty acid-induced NLRP3—ASC inflammasome activation interferes with insulin signaling. Nat. Immunol. 12:406–15.CrossRefGoogle Scholar
  66. 66.
    Zhang Q, et al. (2010) Circulating mitochondrial DAMPs cause inflammatory responses to injury. Nature. 464:104–7.CrossRefPubMedPubMedCentralGoogle Scholar
  67. 67.
    Pugin J. (2008) Dear SIRS, the concept of “alarmins” makes a lot of sense! Intensive Care Med. 34:216–21.Google Scholar
  68. 68.
    Wang H, et al. (1999) HMG-1 as a late mediator of endotoxin lethality in mice. Science. 285:246–51.CrossRefGoogle Scholar
  69. 69.
    Scaffidi P, Misteli T, Bianchi ME. (2002) Release of chromatin protein HMGB1 by necrotic cells triggers inflammation. Nature. 418:191–5.CrossRefGoogle Scholar
  70. 70.
    Qin S, et al. (2006) Role of HMGB1 in apoptosismediated sepsis lethality. J. Exp. Med. 203:1637–42.CrossRefPubMedPubMedCentralGoogle Scholar
  71. 71.
    Xu J, et al. (2009) Extracellular histones are major mediators of death in sepsis. Nat. Med. 15:1318–21.CrossRefPubMedPubMedCentralGoogle Scholar

Copyright information

© The Author(s) 2013

Open Access This article is licensed under a Creative Commons Attribution-NonCommercial-NoDerivatives 4.0 International License, which permits any non-commercial use, sharing, distribution and reproduction in any medium or format, as long as you give appropriate credit to the original author(s) and the source, and provide a link to the Creative Commons license. You do not have permission under this license to share adapted material derived from this article or parts of it.

The images or other third party material in this article are included in the article’s Creative Commons license, unless indicated otherwise in a credit line to the material. If material is not included in the article’s Creative Commons license and your intended use is not permitted by statutory regulation or exceeds the permitted use, you will need to obtain permission directly from the copyright holder.

To view a copy of this license, visit (https://doi.org/creativecommons.org/licenses/by-nc-nd/4.0/)

Authors and Affiliations

  • Dae Won Park
    • 1
    • 2
  • Shaoning Jiang
    • 1
  • Jean-Marc Tadie
    • 1
    • 3
  • William S. Stigler
    • 1
  • Yong Gao
    • 1
  • Jessy Deshane
    • 1
  • Edward Abraham
    • 4
  • Jaroslaw W. Zmijewski
    • 1
  1. 1.Division of Pulmonary, Allergy and Critical Care Medicine, Department of MedicineUniversity of Alabama at Birmingham School of MedicineBirminghamUSA
  2. 2.Division of Infectious DiseasesKorea University Ansan HospitalAnsanRepublic of Korea
  3. 3.Service des Maladies Infectieuses et Réanimation MédicaleCentre Hospitalier UniversitaireRennesFrance
  4. 4.Office of the DeanWake Forest University School of MedicineWinston-SalemUSA

Personalised recommendations