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Logo of ajrccmIssue Featuring ArticlePublisher's Version of ArticleSubmissionsAmerican Thoracic SocietyAmerican Thoracic SocietyAmerican Journal of Respiratory and Critical Care Medicine
 
Am J Respir Crit Care Med. 2008 July 15; 178(2): 168–179.
Published online 2008 April 24. doi:  10.1164/rccm.200710-1602OC
PMCID: PMC2453511

Mitochondrial Respiratory Complex I Regulates Neutrophil Activation and Severity of Lung Injury

Abstract

Rationale: Mitochondria have important roles in intracellular energy generation, modulation of apoptosis, and redox-dependent intracellular signaling. Although reactive oxygen species (ROS) participate in the regulation of intracellular signaling pathways, including activation of nuclear factor (NF)-κB, there is only limited information concerning the role of mitochondrially derived ROS in modulating cellular activation and tissue injury associated with acute inflammatory processes.

Objectives: To examine involvement of the mitochondrial electron transport chain complex I on LPS-mediated NF-κB activation in neutrophils and neutrophil-dependent acute lung injury.

Methods: Neutrophils incubated with rotenone or metformin were treated with bacterial lipopolysaccharide (LPS) to determine the effects of mitochondrial complex I inhibition on intracellular concentrations of reactive oxygen species, NF-κB activation, and proinflammatory cytokine expression. Acute lung injury was produced by intratracheal injection of LPS into control, metformin, or rotenone-treated mice.

Measurements and Main Results: Inhibition of complex I with either rotenone or the antihyperglycemic agent metformin was associated with increased intracellular levels of both superoxide and hydrogen peroxide, as well as inhibition of LPS-induced IκB-α degradation, NF-κB nuclear accumulation, and proinflammatory cytokine production. Treatment of LPS-exposed mice with rotenone or metformin resulted in inhibition of complex I in the lungs, as well as diminished severity of lung injury.

Conclusions: These results demonstrate that mitochondrial complex I plays an important role in modulating Toll-like receptor 4–mediated neutrophil activation and suggest that metformin, as well as other agents that inhibit mitochondrial complex I, may be useful in the prevention or treatment of acute inflammatory processes in which activated neutrophils play a major role, such as acute lung injury.

Keywords: acute lung injury, neutrophil, mitochondria, reactive oxygen species, nuclear factor-κB

AT A GLANCE COMMENTARY

Scientific Knowledge on the Subject

Little is known about how mitochondria participate in neutrophil activation and neutrophil-driven inflammation.

What This Study Adds to the Field

These results demonstrate that mitochondrial complex I plays an important role in modulating Toll-like receptor 4–mediated neutrophil activation and suggest that metformin, as well as other agents that inhibit mitochondrial complex I, may be useful in the prevention or treatment of acute inflammatory processes in which activated neutrophils play a major role, such as acute lung injury.

Mitochondria have important roles in cellular function, including participation in energy generation and modulation of apoptosis (1). In addition, mitochondria produce large amounts of reactive oxygen species (ROS) and are important participants in redox-dependent intracellular signaling (2). There are four carriers of electron transport, complexes I to IV, embedded in the lipid bilayer of the inner mitochondrial membrane. Complex I (NADH: ubiquinone oxidoreductase) transfers electrons from NADH (nicotinamide adenine dinucleotide reduced) to ubiquinone (coenzyme Q [CoQ]). The energy released by this process results in the transfer of protons across the mitochondrial membrane. Under baseline conditions, approximately 5% of electrons escape from the mitochondrial electron transport chain and, in the presence of oxygen, result in the formation of superoxide anion. Superoxide is rapidly converted into hydrogen peroxide by mitochondrial superoxide dismutase or by spontaneous disproportionation. Complex I is considered to be a major site of electron leak and subsequent superoxide production (3, 4).

Activated neutrophils produce large amounts of ROS, a beneficial function in host defense, where such activity is involved in eradication of bacteria and other pathogens. However, excessive production of ROS by neutrophils can be deleterious, contributing to organ system dysfunction in inflammatory conditions, such as sepsis or acute lung injury (510). In addition to generating ROS, neutrophils also appear to be affected by ROS present in the extracellular and intracellular environments. For example, whereas increased intracellular levels of superoxide in neutrophils lead to activation of nuclear factor (NF)-κB as well as production of proinflammatory cytokines, exposure of neutrophils to hydrogen peroxide inhibits bacterial lipopolysaccharide (LPS)-induced proteasomal degradation of the NF-κB inhibitory subunit IκB-α, nuclear translocation of NF-κB, and expression of NF-κB–dependent cytokines (11).

Recent reports have shown the presence of a mitochondrial network in neutrophils that participates in regulation of cell shape and chemotaxis (12). However, little is known about the role of mitochondrially derived ROS in modulating neutrophil function. To examine this issue, we treated isolated neutrophils and mice with inhibitors of mitochondrial complex I, which are known to increase mitochondrial ROS generation (3, 4). We found that treatment of neutrophils with rotenone, a potent and specific inhibitor of complex I, or metformin, an antihyperglycemic agent that is frequently used in patients with diabetes (13) and which also modulates mitochondrial ROS formation by inhibition of complex I (14), resulted in increased ROS formation, decreased NF-κB activation, and diminished production of proinflammatory cytokines in LPS-stimulated neutrophils. We also demonstrated that rotenone and metformin effectively reduced the severity of LPS-induced acute lung injury in mice.

METHODS

Mice

Male C57BL/6 mice, 8 to 12 weeks of age, were purchased from Jackson Laboratory (Bar Harbor, ME). The mice were kept on a 12:12-hour light–dark cycle with free access to food and water. All experiments were conducted in accordance with institutional review board–approved protocols (Institutional Animal Care and Use Committee, UAB).

Reagents

Escherichia coli 0111:B4 endotoxin (LPS), hydrogen peroxide, dihydroethidium (DHE), rotenone, metformin, catalase, pegylated catalase (PEG-CAT) CoQ1, NADPH, carbonyl cyanide-4-(trifluoromethoxy)-phenylhydrazone (FCCP), and thenoyltrifluoroacetone (TTFA) were obtained from Sigma (St. Louis, MO). 2′,7′-Dichlorodihydrofluorescein diacetate (DCFH-DA) was purchased from Invitrogen (Carlsbad, CA). Cytokine ELISA kits were obtained from R&D Systems (Minneapolis, MN).

Neutrophil Isolation and Culture

Bone marrow neutrophils were isolated as described previously (15, 16). Briefly, bone marrow cell suspensions were isolated from the femur and tibia of a mouse by flushing with RPMI 1640 medium/5% fetal bovine serum (FBS). The cell suspension was passed through a glass wool column and collected by subsequent washing with phosphate-buffered saline (PBS) containing 5% FBS. Negative selection to purify neutrophils was performed by incubation of the cell suspension with biotinylated primary antibodies specific for the cell surface markers F4/80, CD4, CD45R, CD5, and TER119 according to the manufacturer's procedure (www.stemcell.com/technical/13309-PIS.pdf; Stem Cell Technologies, Vancouver, BC, Canada) for 15 minutes at 4°C followed by subsequent incubation with anti-biotin tetrameric antibody (100 μl) (Stem Cell Technologies) for 15 minutes. The complex of antitetrameric antibodies and cells was then incubated with colloidal magnetic dextran iron particles (60 μl) (Stem Cell Technologies) for an additional 15 minutes at 4°C. The T cells, B cells, red blood cells, monocytes, and macrophages were captured in a column surrounded by a magnet, allowing the neutrophils to pass through. Neutrophil purity, as determined by Wright-Giemsa–stained cytospin preparations, was consistently greater than 97%. The purified neutrophils were cultured in RPMI 1640 medium containing FBS (0.5%) and treated as described in the figure legends. Neutrophil viability after experimental treatments was determined using trypan blue staining and was consistently greater than 99%.

Alveolar Macrophage Isolation and Culture

Alveolar macrophages were isolated from the lungs of C57BL/6 mice by cannulating the trachea with a blunt 20-gauge needle and then lavaging the lungs five times with 1 ml of iced PBS/ethylenediaminetetraacetic acid (EDTA) (5 mM). Macrophage purity, as determined by Wright-Giemsa–stained cytospin preparations, was consistently greater than 95%. Cells were washed two times with RPMI 1640/0.5% FBS, cultured in RPMI 1640 medium containing FBS (0.5%) for 2 hours, and then treated as described in the figure legends. Neutrophil viability after experimental treatment was determined using trypan blue staining and was consistently greater than 99%.

Assays of Respiratory Complex I and Citrate Synthase Activities

Respiratory complex I activity in neutrophils and in mitochondria-enriched fractions obtained from mouse lungs or livers was measured spectrophotometrically (UV-2501PC Shimadzu; Shimadzu, Scientific Instruments, Columbia, MD) and corrected by subtraction of the rotenone-insensitive rates (17). Briefly, neutrophils (30 × 106 cells/ml) or mitochondria-enriched fractions from lungs or livers were lysed in potassium/phosphate buffer by 10 repeated freeze–thaw cycles using liquid nitrogen. Complex I activity was then determined in potassium/phosphate buffer containing bovine serum albumin (BSA) (2.5 mg/ml), NADH (100 μM), potassium cyanide (KCN) (1 mM), CoQ1 (50 μM), and 20–100 μg of protein by following the rotenone-sensitive oxidation of NADH (λ = 340 nm) initiated by CoQ1 (50 μM). Data were acquired every 5 seconds for 5 minutes after initiation of the reaction, including 5 minutes after the addition of rotenone (0, 1, or 10 μM) or metformin (0, 30, or 40 mM). Basal complex I activity was approximately 10 or approximately 30 nmol · min−1 · mg−1 in samples obtained from lung or liver, respectively. Citrate synthase was measured by using the coupled reaction among oxaloacetate, acetyl-CoA, and 5,5′-dithiobis(2,4-nitrobenzoic acid) (18).

Imaging of Dichlorofluorescin and Dihydroethidium Fluorescence

Intracellular levels of hydrogen peroxide or superoxide were determined using the redox-sensitive probes DCFH-DA or dihydroethidium (DHE) in conjunction with fluorescent microscopy (19, 20). Briefly, neutrophils (1.5 × 106/well) were incubated in a four-well chambered cover glass (Nalge, Naperville, IL), and treated with rotenone for 60 minutes or metformin for 2.5 hours. The cells were then incubated with DCFH-DA (10 μM) or DHE (10 μM) for 30 minutes and fluorescent microscopic images acquired using double bidirectional scans of live neutrophils with a Leica DMIRBE inverted epifluorescence/Nomarski microscope outfitted with Leica TCS NT laser confocal optics (Leica, Inc., Exton, PA). The pinhole setting was 0.2 Airy units and laser excitation was set for 5% to avoid dye photooxidation. The levels of fluorescence were averaged using SimplePCI software (Compix, Cranberry Township, PA). Images were processed using IPLab Spectrum and Adobe Photoshop (Adobe Systems, San Jose, CA) software.

Isolation of Mitochondria

Liver and lung mitochondria were isolated according to standard procedures with minor modifications (21). Briefly, liver or lung homogenates were incubated in STE buffer containing sucrose (250 mM), Tris pH 7.4 (10 mM), and ethyleneglycol-bis-(β-aminoethyl ether)-N,N′-tetraacetic acid (EGTA) (2 mM), followed by centrifugation (1,000 × g) for 3 minutes at 4°C. Supernatants were then collected and centrifuged (10,000 × g) for 10 minutes at 4°C. The resultant pellets were suspended in STE buffer and centrifuged (10,000 × g) for 10 minutes at 4°C. The pink and light brown pellets surrounding the dark brown center were aspirated and the remaining pellet suspended in STE buffer (1 ml) and centrifuged (10,000 × g) for 15 minutes at 4°C. Finally, the cell pellet was suspended in potassium/phosphate buffer and stored at −80°C.

Purification of Nuclear Proteins

Nuclear proteins were purified from 7 × 106 neutrophils lysed in 100 μl of buffer containing Tris pH 7.5 (10 mM), NaCl (10 mM), MgCl2 (3 mM), Nonidet P40 (NP 40) (0.02%), EGTA (1 mM), sodium orthovanadate (1 mM), sodium fluoride (50 mM), and the protease inhibitors phenylmethylsulphonyl fluoride (100 μM), leupeptin (10 μg/ml), aprotinin (10 μg/ml), pepstatin A (5 μg/ml), and okadaic acid (1 nM). The lysed cells were centrifuged (2,700 g) for 10 minutes at 4°C. The supernatant containing the cytosol was collected and then centrifuged (20,800 g) for 15 minutes at 4°C to obtain the cytosolic fraction. The pellet containing nuclei was washed three times by gentle resuspension in 150 μl wash buffer ([1,4-piperazinebis (ethane sulfonic acid)] pH 6.8 [10 mM], sucrose [300 mM], MgCl2 [3 mM], EGTA [1 mM], NaCl [25 mM], sodium orthovanadate [1 mM], sodium fluoride [50 mM], and protease inhibitors), and centrifuged (2,700 g) for 5 minutes at 4°C. Nuclear proteins were obtained using nuclear extraction buffer (Tris pH 7.4 [50 mM], NaCl [150 mM], NP 40 [0.5%, vol/vol], EDTA [1 mM], EGTA [1 mM], okadaic acid [1 nM], and protease inhibitors). The nuclear lysates were then sonicated and centrifuged (10,000 × g) for 15 minutes at 4°C. The protein concentration of the supernatant was determined using Bradford reagent (BioRad, Hercules, CA) with BSA as a standard.

Western Blot Analysis

Briefly, neutrophils (3.5 × 106/well), macrophages (2 × 105/well), or isolated nuclei were lysed using buffer containing Tris pH 7.4 (50 mM), NaCl (150 mM), NP-40 (0.5%, vol/vol), EDTA (1 mM), EGTA (1 mM), okadaic acid (1 nM), and protease inhibitors. The cell lysates were sonicated and centrifuged at 10,000 × g for 15 minutes at 4°C. 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 5 minutes. Equal amounts of proteins were resolved by 10% sodium dodecyl sulfate–polyacrylamide gel electrophoresis, and transferred onto polyvinylidene fluoride (PVDF) membranes (Immobilon P; Millipore, Billerica, MA). The membranes were probed with specific antibodies to IκB-α (Cell Signaling, Beverly, MA), p65 (Santa Cruz Biotechnology, Santa Cruz, CA), or actin (Sigma), followed by detection with horseradish peroxidase–conjugated goat anti-rabbit IgG. Bands were visualized by enhanced chemiluminescence (Super Signal; Pierce Biotechnology, Rockford, IL) and quantified by AlphaEaseFC software (Alpha Innotech, San Leandro, CA). Each experiment was carried out two or more times using cell populations obtained from separate groups of mice.

In Vivo Acute Lung Injury Model

To induce acute lung injury, Escherichia coli 0111:B4 LPS (1 mg/kg) in PBS was administered into the oropharynx (22). Briefly, mice were anesthetized with isoflurane, the tongue was gently extended, and LPS in PBS (50 μl) was instilled into the distal part of the oropharynx.

In pretreatment experiments, mice were given rotenone (8 mg/kg) in saline/dimethyl sulfoxide (1:1) or saline/dimethyl sulfoxide injection intraperitoneally 4 hours before intratracheal LPS administration. Previously, a similar dosage of rotenone was reported in C57BL/6 mice (23). Metformin (250 mg/kg) in saline or saline alone (200 μl) was injected (intraperitoneally) starting 4 hours before LPS administration. In additional experiments, metformin (125 mg/kg) in saline or saline alone was given (intraperitoneally) 30 minutes and 8 hours after oropharyngeal administration of LPS. These doses of metformin were previously used in murine models examining efficacy or toxicity of metformin (2426). There were no deaths associated with rotenone, metformin, or LPS administration.

Harvest of Lungs and BAL

Lungs were harvested 24 hours after LPS administration. BAL fluid was obtained by cannulating the trachea with a blunt 20-gauge needle and then lavaging the lungs three times with 1 ml of iced PBS.

Wet-to-Dry Lung Weight Ratios

The wet-to-dry ratio was determined as reported previously (27). Separate groups of mice were used to measure wet-to-dry ratios and for BAL fluid acquisition. All mice used for lung wet-to-dry weight ratios were of identical ages. Lungs were excised, rinsed briefly in PBS, blotted, and then weighed to obtain the “wet” weight. Lungs were then dried in an oven at 80°C for 7 days to obtain the “dry” weight.

Myeloperoxidase Assay

Myeloperoxidase activity was assayed as reported previously with minor modifications (28). In brief, lung tissue was homogenized in 1 ml of potassium phosphate buffer, pH 6.0 (50 mM), containing a reducing agent, N-ethylmaleimide (10 mM), for 30 seconds on ice. The homogenate was centrifuged (12,000 g) for 30 minutes at 4°C and washed twice in ice-cold buffer. The pellet was then resuspended and sonicated on ice for 90 seconds in ×10 volume of hexadecyltrimethylammonium bromide (HTAB) buffer (HTAB [0.5%], potassium phosphate pH 6.0 [50 mM]). Samples were incubated in a water bath for 2 hours at 56°C and then centrifuged (12,000 g) for 10 minutes. The supernatant was collected for assay of myeloperoxidase activity as determined by measuring the H2O2-dependent oxidation of 3,3′-dimethoxybenzidine dihydrochloride (λ = 460 nm).

Cytokine ELISA

ELISAs were used to measure cytokines in BAL fluid or in culture media from LPS-stimulated neutrophils. Levels of tumor necrosis factor (TNF)-α, macrophage inflammatory protein (MIP)-2, IL-6, or keratinocyte-derived chemokine (KC) were determined using commercially available ELISA kits (R&D Systems), according to the manufacturer's instructions and as previously described (15, 16).

Measurement of Glucose in Plasma

Glucose content in blood plasma was determined using an Accu-Chek Advantage glucometer (model 768; Boehringer Mannheim, Nutley, NJ).

Histochemistry

Mice were killed and 1 ml of paraformaldehyde (10%) was injected into the lungs by cannulating the trachea with a blunt 20-gauge needle. The lungs were excised, rinsed briefly in PBS, blotted, and incubated in 10% paraformaldehyde for 24 hours followed by paraffin embedding and processing for hematoxylin–eosin staining.

Statistical Analyses

For each experiment, neutrophils were isolated and pooled from groups of mice (n = 3–6) and all conditions were studied at the same time. One-way analysis of variance, the Tukey-Kramer multiple comparisons test (for multiple groups), or Student's t test (for comparisons between two groups) was used. P < 0.05 was considered to be statistically significant.

RESULTS

Rotenone Inhibits Mitochondrial Complex I and Increases ROS Generation by Neutrophils

Rotenone is a potent inhibitor of mitochondrial respiratory complex I and increases superoxide production by this organelle in many types of cells (29, 30). However, whether rotenone can inhibit complex I and alter mitochondrially generated ROS production in neutrophils has not previously been investigated. Therefore, the effect of rotenone on complex I activity was measured in neutrophil extracts by following rotenone-sensitive oxidation of NADH initiated by CoQ1. Figure 1A shows that neutrophils possess active complex I that is dose-dependently inhibited by rotenone.

Figure 1.
Rotenone inhibits mitochondrial respiratory complex I and induces dihydroethidium (DHE) and 2′,7′-dichlorodihydrofluorescein (DCFH) oxidation in neutrophils. (A) Enzymatic activity of respiratory complex I in cell extracts (100 μg ...

Because rotenone potently inhibited mitochondrial complex I activity in neutrophils, we next examined the role of complex I on ROS production. To detect superoxide generation, neutrophils were treated with rotenone and then loaded with the cell-permeable probe DHE (10 μM). As shown in Figures 1B and 1C, treatment of neutrophils with rotenone resulted in a robust increase in DHE fluorescence. Consistent with the rotenone-induced increase in superoxide production, there were also elevated levels of intracellular hydrogen peroxide, as determined by the probe DCFH-DA, in rotenone-treated neutrophils (Figures 1B and 1D).

Prolonged inhibition of mitochondrial complex I by rotenone has been shown to induce apoptosis in nonmyelocytic cell populations (3033). In contrast, rotenone did not induce apoptosis of human neutrophils (34). Cell death after exposure of mouse neutrophils to rotenone (10 μM) for 6 hours was consistently less than 2%, as determined by trypan blue exclusion assay (data not shown).

Rotenone-dependent Inhibition of Complex I Alters LPS-induced Nuclear Translocation of NF-κB and Cytokine Production by Neutrophils

Mitochondrially generated ROS participate in the regulation of multiple signal transduction pathways (19, 24, 35, 36), including NF-κB activation (37). Because rotenone treatment caused an increase in intracellular levels of both superoxide and hydrogen peroxide (Figures 1B, 1C, and 1D), we determined if LPS-mediated phosphorylation of the NF-κB p65 subunit, p65 nuclear accumulation, and proinflammatory cytokine production were altered in neutrophils exposed to rotenone. As shown in Figures 2A and 2B, culture of neutrophils with LPS resulted in increased levels of Ser-536 phosphorylation and nuclear accumulation of the NF-κB p65 subunit, whereas rotenone pretreatment inhibited these effects. Moreover, exposure of neutrophils to rotenone was associated with a dose-dependent decrease in LPS-induced secretion of the NF-κB–dependent cytokine TNF-α as well as release of MIP-2, a CXC chemokine whose transcription is also regulated by NF-κB (38) (Figures 2C and 2D). Rotenone alone had no effect on NF-κB nuclear accumulation and cytokine production by neutrophils.

Figure 2.
Effects of rotenone on LPS-induced p65 (Ser-536) phosphorylation, p65 nuclear accumulation, and cytokine production by neutrophils. (A) Representative Western blots show rotenone-dependent inhibition of LPS-induced p65 phosphorylation and p65 nuclear ...

Because IκB-α has a central role in maintaining cytoplasmic sequestration of NF-κB (39, 40), we examined the effect of rotenone on IκB-α levels in neutrophils. As shown in Figures 3A–3D, rotenone inhibited LPS-mediated IκB-α degradation. In contrast, treatment of neutrophils with thenoyltrifluoroacetone (TTFA), a specific inhibitor of complex II (41, 42), had no effect.

Figure 3.
Rotenone inhibits LPS-mediated NF-κB inhibitory subunit (IκB)-α degradation in neutrophils. (A) A representative Western blot shows dose-dependent inhibition of LPS- induced IκB-α degradation by rotenone. Neutrophils ...

Inhibition of the mitochondrial electron chain can affect ATP generation and result in inefficient IκB-α phosphorylation and degradation (43). To examine this possibility, cells were treated with carbonyl cyanide-4-(trifluoromethoxy)-phenylhydrazone (FCCP), an uncoupler of mitochondrial respiration that results in inhibition of mitochondrial ATP synthesis (44). As shown in Figure 3D, pretreatment of neutrophils with FCCP (5 μM) for 60 minutes had no effect on LPS-induced IκB-α degradation. This result indicates that the decrease in mitochondrially generated ATP associated with complex I inhibition is not responsible for effects on IκB-α degradation.

To further explore whether the ROS generated by complex I inhibition are responsible for modulation of IκB-α degradation, neutrophils were pretreated with catalase or PEG-CAT and then cultured with rotenone and LPS. Of note, PEG-CAT, unlike unmodified catalase, has been demonstrated to transit rapidly to the intracellular space and participate in the dismutation of mitochondrially derived H2O2 (45, 46). As shown in Figures 3E and 3F, treatment of neutrophils with PEG-CAT, but not catalase, abolished the inhibitory effects of rotenone on LPS-induced IκB-α degradation. These results suggest that the mechanism through which mitochondrially derived ROS, and specifically H2O2, inhibit the nuclear translocation of NF-κB and expression of NF-κB–dependent cytokines is by preventing IκB-α degradation with resultant cytosolic retention of NF-κB.

Metformin Inhibits Complex I Activity and LPS-induced Neutrophil Activation

Metformin, a biguanide frequently used in the treatment of diabetes, has been shown to block complex I, increase ROS production by mitochondria, and alter intracellular signaling pathways (24), but its activity on Toll-like receptor/IL-1 receptor (TLR/IL-1R)–induced cellular activation has not been explored in neutrophils. As shown in Figure 4A, addition of metformin to neutrophil cell extracts significantly inhibits complex I activity.

Figure 4.
Effects of metformin on complex I activity and dihydroethidium (DHE) or 2′,7′-dichlorodihydrofluorescein (DCFH) oxidation in neutrophils. (A) Mitochondrial complex I activity was determined in control cell extracts (100 μg/ml) ...

Metformin increased DCF and DHE fluorescence in neutrophils (Figures 4B and 4C), indicating that metformin increases intracellular levels of ROS. In a similar manner to rotenone, metformin decreased LPS-induced Ser-536 phosphorylation of the NF-κB p65 subunit, nuclear accumulation of NF-κB, and cytokine production (Figure 5). In addition, metformin dose-dependently prevented degradation of IκB-α in LPS-stimulated neutrophils (Figures 6A–6C). This effect of metformin was reversed by preincubation of neutrophils with PEG-CAT, demonstrating that it was specific for hydrogen peroxide (Figure 6D).

Figure 5.
Metformin inhibits LPS-mediated p65 (Ser-536) phosphorylation, nuclear factor (NF)-κB nuclear translocation, and cytokine production by neutrophils. Neutrophils were incubated with metformin (0 or 250 μM) for 2.5 hours followed by treatment ...
Figure 6.
Effects of metformin on LPS-induced IκB-α degradation. (A, B) A representative Western blot and optical densitometry (mean ± SD) of IκB-α and actin from neutrophils incubated with metformin (0–500 μM) ...

The inhibitory effects of complex I inhibition by rotenone (Figure 3) or metformin (Figures 6A–6D) on IκB-α degradation were not limited to neutrophils, as similar findings were present in LPS-stimulated alveolar macrophages (Figure 6E).

Rotenone Pretreatment Attenuates LPS-induced Acute Lung Injury

To examine the effects of mitochondrial complex I inhibition on LPS-induced acute lung injury, mice were pretreated with rotenone 4 hours before LPS administration. Rotenone administration resulted in significant inhibition (~30%) of complex I activity in enriched mitochondrial fractions from lung homogenates (Figure 7A). To ensure that the reduction in complex I activity was due to rotenone specific effects and was not an artifact of rotenone affecting the mitochondrial purification process, mitochondrial citrate synthase activity was measured. In previous studies (47, 48), mitochondrial citrate synthase activity has been shown to be resistant to oxidant-induced inactivation and therefore has been used as an indicator of mitochondrial content in enriched fractions. As shown in Figure 7, no alterations of citrate synthase activity were found in mitochondrial fractions from rotenone-treated as compared with vehicle-treated mice.

Figure 7.
Effects of rotenone on LPS-induced acute lung injury. (A) Complex I and citrate synthase activity were measured in mitochondria-enriched fractions obtained from lungs of C57BL/6 mice treated with rotenone (0 or 8 mg/kg intraperitoneally) 24 hours previously ...

Rotenone-treated mice had less severe lung injury than those given vehicle alone before LPS. In particular, wet-to-dry ratios, pulmonary myeloperoxidase concentrations, and neutrophil numbers in BAL fluid were significantly reduced in mice that received rotenone before LPS administration (Figure 7B). There were no significant differences in wet-to-dry ratios between control mice given vehicle or rotenone alone, without LPS administration (data not shown). Pulmonary and BAL concentrations of MIP-2, TNF-α, IL-6, and KC were also significantly decreased in mice pretreated with rotenone before LPS instillation (Figure 7C).

Metformin Prevents LPS-induced Acute Lung Injury

Because a presumed mechanism of metformin's metabolic actions in vivo is inhibition of respiratory complex I (14), complex I activity was measured in mitochondria-enriched fractions obtained from murine liver and lungs. In hepatic extracts, basal complex I activity was approximately 30 nmol · min−1 · mg−1, and there was nearly complete inhibition in the presence of rotenone (Figure E1A of the online supplement). Metformin, when given to unmanipulated mice or when administered to LPS-treated mice either before or after LPS administration, decreased complex I activity in the liver and lungs (Figure 8A and Figure E1B), demonstrating in vivo inhibitory effects on complex I.

Figure 8.
Metformin treatment diminishes the severity of LPS-induced acute lung injury. C57BL/6 mice were given LPS (1 mg/kg) intratracheally followed by vehicle intraperitoneally 0.5 and 8 hours post-LPS, or two doses of metformin (125 mg/kg intraperitoneally) ...

The severity of lung injury, as determined by lung edema and neutrophil accumulation into the pulmonary interstitium and airspaces, was significantly reduced in mice that received metformin starting either before (Figure E2) or after administration of LPS (Figures 8A and 8B). Levels of cytokines and chemokines, specifically MIP-2 and IL-6, were also significantly decreased in the lungs of mice that had received metformin after LPS administration (Figure 8C). Similar results were obtained from mice given metformin before LPS injection (Figure E3). There were no significant differences in the wet-to-dry ratios between control mice given saline or metformin alone, without LPS administration (data not shown). As shown in Figure 9, there was decreased LPS-induced neutrophil accumulation and interstitial edema in metformin-treated mice as compared with those given saline.

Figure 9.
Effects of metformin on LPS-induced neutrophil accumulation in the lungs. Representative histologic sections show decrease in the accumulation of interstitial and intraalveolar neutrophils in LPS/metformin-treated mice compared with mice given LPS and ...

Recent studies in critically ill patients have shown that strict control of circulating glucose levels results in better clinical outcomes and fewer complications (49, 50). Because metformin is used to reduce elevated serum glucose levels in patients with type 2 diabetes, it is possible that its beneficial effects on acute lung injury were due to actions in controlling glucose levels rather than on complex I. However,LPS-exposed mice treated with metformin had higher circulating glucose concentrations than did those in the control group, where there was a significant decrease (~40%) in plasma glucose 24 hours after LPS administration (control, 385 ± 26 mg/dl; LPS, 216 ± 32 mg/dl; metformin/LPS, 345 ± 34 mg/dl). Moreover, in mice not given LPS, metformin had no effects on plasma glucose levels (metformin, 374 ± 11 mg/dl).

DISCUSSION

Complex I, also known as NADH–ubiquinone oxidoreductase, is the first of four electron carriers in the mitochondrial transport chain and, with complex III, is a major site of mitochondrial superoxide production (3). Under normal metabolic conditions, approximately 5% of electrons can escape from the mitochondrial electron chain and generate superoxide in the presence of oxygen. Although increased production of superoxide from complex I has been postulated to occur as a result of reverse electron flux (4), the precise mechanism of complex I–mediated superoxide formation has not been fully elucidated.

The present studies show that inhibition of mitochondrial respiratory complex I in neutrophils is associated with profound effects on TLR4-induced neutrophil function, including increases in intracellular ROS levels as well as diminished NF-κB activation and proinflammatory cytokine production. Although inhibition of respiratory complex I, with associated increase in ROS production, has been demonstrated using isolated mitochondria, in cell culture models and in vivo (3, 4, 24, 51), mitochondrial complex I has not previously been shown to be involved in the regulation of intracellular levels of ROS in neutrophils. In these experiments, both rotenone and metformin inhibited complex I activity and exposure to either of these agents produced rapid increases in superoxide and H2O2 concentrations in neutrophils. Inhibition of complex I was also found in the lungs of mice treated with metformin or rotenone.

A possible mechanism for the antiinflammatory effects of complex I blockade may be through increasing intracellular concentrations of H2O2. Superoxide produced by complex I is predominantly generated in the mitochondrial matrix and, as a charged species, superoxide is not readily diffusible across mitochondrial membranes. However, superoxide rapidly undergoes dismutation to H2O2 within the mitochondria and, in contrast to superoxide, H2O2 is capable of diffusing across membranes and can transit from the mitochondria into the cytoplasm where it participates as a second messenger in the regulation of NF-κB and other intracellular signaling pathways. Previous studies, including those from our laboratory, have demonstrated that exposure of neutrophils to extracellular H2O2, which is associated with rapid increases in its intracellular concentrations, resulted in inhibition of LPS-induced IκB-α degradation, NF-κB activation, and expression of NF-κB–dependent cytokines, such as TNF-α, MIP-2, and IL-8 (11, 15, 52). In the present experiments, treatment of LPS-stimulated neutrophils with PEG-CAT abrogated the inhibitory effects of rotenone or metformin on IκB-α degradation. These results are consistent with recent reports showing that PEG-CAT decreases intracellular levels of H2O2, including mitochondrially derived H2O2 (45, 46).

Inhibition of complex I activity, in addition to enhancing mitochondrial ROS generation, also results in decreased ATP production by mitochondria and subsequent effects on ATP-dependent intracellular processes. Although such inhibition of mitochondrial ATP generation could affect IκB-α degradation, our experiments found that rotenone or metformin, but not FCCP, a known uncoupler of mitochondrial respiration, inhibited LPS-induced IκB-α degradation. These results indicate that enhanced mitochondrial ROS, and not suppression of ATP generation, are responsible for the inhibitory effects of complex I blockade on LPS-induced IκB-α degradation, nuclear translocation of NF-κB, and expression of NF-κB–dependent proinflammatory cytokines. In addition, we examined whether other components of the mitochondrial respiratory sequence could also affect IκB-α degradation in a manner similar to that observed with complex I inhibition. However, inhibition of complex II with TTFA had no effects on LPS-induced IκB-α degradation, indicating that inhibition of complex I has specific effects not generalizable to other ROS-generating mitochondrial components.

Several steps in the NF-κB signaling cascade have been shown to be regulated by H2O2. H2O2-dependent increases in S-glutathionylation of IKKβ (53), oxidation of IκB-α at methionine 45 (54), cysteine thiol oxidation of the p50 subunit of NF-κB (55), as well as inhibition of proteasome-dependent degradation of IκB-α result in diminished NF-κB signaling. However, not all of these inhibitory effects of H2O2 have been found in all cell types (5658). For example, the ability of H2O2 to reduce LPS-induced proteasomal activity, which was recently described in neutrophils, was not present in macrophages (11). Nevertheless, in the present studies, blockade of complex I with rotenone or metformin had similar inhibitory effects on IκB-α degradation in LPS-stimulated alveolar macrophages and neutrophils, suggesting that this is a general antiinflammatory mechanism. These results also suggest that effects of rotenone and metformin on pulmonary cell populations other than infiltrating neutrophils, such as alveolar macrophages, may contribute to the benefit of complex I inhibition in acute lung injury.

In the present studies, rotenone and metformin reduced the severity of LPS-induced acute lung injury, an inflammatory process in which activated neutrophils that infiltrate the pulmonary interstitium and migrate into the airways play an important role (27, 59). Although rotenone has been shown to effectively block respiratory complex I, its in vivo use is limited by dopaminergic neuron injury followed by the appearance of Parkinson-like symptoms in rodent models as well as in humans. In these experiments, metformin had beneficial effects even when administered after exposure of the lungs to LPS, suggesting that the role of mitochondrially derived ROS in contributing to pulmonary injury is not limited to the immediate period after TLR4 engagement. Metformin is commonly used in patients with diabetes (13) and complex I inhibition has been suggested as a central mechanism for its beneficial effect in this clinical setting (14). Metformin has a broad spectrum of effects that include improving insulin-mediated glucose metabolism, inhibition of adipose tissue lipolysis, reduction in circulating free fatty acids, and diminished very low density lipoprotein production. However, little is known concerning the effects of metformin on acute inflammatory processes. Recently, metformin has been shown to prevent LPS-induced liver dysfunction after partial hepatectomy, including the accumulation of neutrophils into the liver as well as elevations in hepatic levels of IL-6 and IFN-γ (25). Similarly, metformin reduced hepatic inflammation in animal models of nonalcoholic steatohepatitis as well as in humans with this condition (60, 61). Metformin has also been shown to decrease the proinflammatory response of human umbilical vein endothelial cells when exposed to cytokines in vitro (62). Of note, despite its known effects on glucose metabolism, mice treated with metformin in these experiments had higher plasma glucose levels than did those receiving placebo, indicating that the antiinflammatory effects of metformin were not due to improved glucose control in the treated animals.

The inhibitory effects of metformin on complex I activity appear to be related to its time-dependent accumulation in mitochondria, where millimolar ranges of concentration may be achieved (14). Although metformin has been shown to have both direct and indirect effects on complex I activity, the primary mechanisms responsible are not fully characterized (14, 63). Nevertheless, the present studies demonstrate that mitochondrial complex I activation plays an important role in modulating LPS-mediated neutrophil activation, degradation of IκB-α, nuclear translocation of NF-κB, and neutrophil-dependent cytokine production, as well as inflammatory processes, such as acute lung injury, in which activated neutrophils play a major role. Metformin is a safe and widely used agent for the therapy of non–insulin-requiring diabetes. The present results suggest that metformin, as well as other agents that inhibit mitochondrial complex I activity, may be useful in the prevention or treatment of acute inflammatory processes, such as acute lung injury.

Supplementary Material

[Online Supplement]

Acknowledgments

The authors thank Youhong Zhang for technical assistance.

Notes

Supported in part by National Institutes of Health grants HL62221, HL76206, and HL068743 to E.A. and by the Société Française d'Anesthésie et de Réanimation and the University Hospital of Amiens (France) to E.L.

This article has an online supplement, which is accessible from this issue's table of contents at www.atsjournals.org

Originally Published in Press as DOI: 10.1164/rccm.200710-1602OC on April 24, 2008

Conflict of Interest Statement: None of the authors has a financial relationship with a commercial entity that has an interest in the subject of this manuscript.

References

1. Green DR, Reed JC. Mitochondria and apoptosis. Science 1998;281:1309–1312. [PubMed]
2. Droge W. Free radicals in the physiological control of cell function. Physiol Rev 2002;82:47–95. [PubMed]
3. Lenaz G, Fato R, Genova ML, Bergamini C, Bianchi C, Biondi A. Mitochondrial complex I: structural and functional aspects. Biochim Biophys Acta 2006;1757:1406–1420. [PubMed]
4. Lambert AJ, Brand MD. Inhibitors of the quinone-binding site allow rapid superoxide production from mitochondrial NADH: ubiquinone oxidoreductase (complex I). J Biol Chem 2004;279:39414–39420. [PubMed]
5. Brown KA, Brain SD, Pearson JD, Edgeworth JD, Lewis SM, Treacher DF. Neutrophils in development of multiple organ failure in sepsis. Lancet 2006;368:157–169. [PubMed]
6. Crimi E, Sica V, Slutsky AS, Zhang H, Williams-Ignarro S, Ignarro LJ, Napoli C. Role of oxidative stress in experimental sepsis and multisystem organ dysfunction. Free Radic Res 2006;40:665–672. [PubMed]
7. Kolls JK. Oxidative stress in sepsis: a redox redux. J Clin Invest 2006;116:860–863. [PMC free article] [PubMed]
8. Fink MP. Reactive oxygen species as mediators of organ dysfunction caused by sepsis, acute respiratory distress syndrome, or hemorrhagic shock: potential benefits of resuscitation with Ringer's ethyl pyruvate solution. Curr Opin Clin Nutr Metab Care 2002;5:167–174. [PubMed]
9. Strassheim D, Park JS, Abraham E. Sepsis: current concepts in intracellular signaling. Int J Biochem Cell Biol 2002;34:1527–1533. [PubMed]
10. Chabot F, Mitchell JA, Gutteridge JM, Evans TW. Reactive oxygen species in acute lung injury. Eur Respir J 1998;11:745–757. [PubMed]
11. Zmijewski JW, Zhao X, Xu Z, Abraham E. Exposure to hydrogen peroxide diminishes NF-kappaB activation, IkappaB-alpha degradation, and proteasome activity in neutrophils. Am J Physiol Cell Physiol 2007;293:C255–C266. [PubMed]
12. Fossati G, Moulding DA, Spiller DG, Moots RJ, White MR, Edwards SW. The mitochondrial network of human neutrophils: role in chemotaxis, phagocytosis, respiratory burst activation, and commitment to apoptosis. J Immunol 2003;170:1964–1972. [PubMed]
13. Witters LA. The blooming of the French lilac. J Clin Invest 2001;108:1105–1107. [PMC free article] [PubMed]
14. Owen MR, Doran E, Halestrap AP. Evidence that metformin exerts its anti-diabetic effects through inhibition of complex 1 of the mitochondrial respiratory chain. Biochem J 2000;348:607–614. [PubMed]
15. Strassheim D, Asehnoune K, Park JS, Kim JY, He Q, Richter D, Mitra S, Arcaroli J, Kuhn K, Abraham E. Modulation of bone marrow-derived neutrophil signaling by H2O2: disparate effects on kinases, NF-kappaB, and cytokine expression. Am J Physiol Cell Physiol 2004;286:C683–C692. [PubMed]
16. Yum HK, Arcaroli J, Kupfner J, Shenkar R, Penninger JM, Sasaki T, Yang KY, Park JS, Abraham E. Involvement of phosphoinositide 3-kinases in neutrophil activation and the development of acute lung injury. J Immunol 2001;167:6601–6608. [PubMed]
17. Birch-Machin MA, Turnbull DM. Assaying mitochondrial respiratory complex activity in mitochondria isolated from human cells and tissues. Methods Cell Biol 2001;65:97–117. [PubMed]
18. Shepherd D, Garland PB. The kinetic properties of citrate synthase from rat liver mitochondria. Biochem J 1969;114:597–610. [PubMed]
19. Watanabe N, Zmijewski JW, Takabe W, Umezu-Goto M, Le Goffe C, Sekine A, Landar A, Watanabe A, Aoki J, Arai H, et al. Activation of mitogen-activated protein kinases by lysophosphatidylcholine-induced mitochondrial reactive oxygen species generation in endothelial cells. Am J Pathol 2006;168:1737–1748. [PubMed]
20. Zmijewski JW, Moellering DR, Le Goffe C, Landar A, Ramachandran A, Darley-Usmar VM. Oxidized LDL induces mitochondrially associated reactive oxygen/nitrogen species formation in endothelial cells. Am J Physiol Heart Circ Physiol 2005;289:H852–H861. [PubMed]
21. Frezza C, Cipolat S, Scorrano L. Organelle isolation: functional mitochondria from mouse liver, muscle and cultured fibroblasts. Nat Protocols 2007;2:287–295.
22. Foster WM, Walters DM, Longphre M, Macri K, Miller LM. Methodology for the measurement of mucociliary function in the mouse by scintigraphy. J Appl Physiol 2001;90:1111–1117. [PubMed]
23. Thiffault C, Langston JW, Di Monte DA. Increased striatal dopamine turnover following acute administration of rotenone to mice. Brain Res 2000;885:283–288. [PubMed]
24. Zou MH, Kirkpatrick SS, Davis BJ, Nelson JS, Wiles WG 4th, Schlattner U, Neumann D, Brownlee M, Freeman MB, Goldman MH. Activation of the AMP-activated protein kinase by the anti-diabetic drug metformin in vivo: role of mitochondrial reactive nitrogen species. J Biol Chem 2004;279:43940–43951. [PubMed]
25. Bergheim I, Luyendyk JP, Steele C, Russell GK, Guo L, Roth RA, Arteel GE. Metformin prevents endotoxin-induced liver injury after partial hepatectomy. J Pharmacol Exp Ther 2006;316:1053–1061. [PubMed]
26. Davis BJ, Xie Z, Viollet B, Zou MH. Activation of the AMP-activated kinase by antidiabetes drug metformin stimulates nitric oxide synthesis in vivo by promoting the association of heat shock protein 90 and endothelial nitric oxide synthase. Diabetes 2006;55:496–505. [PubMed]
27. Abraham E, Carmody A, Shenkar R, Arcaroli J. Neutrophils as early immunologic effectors in hemorrhage- or endotoxemia-induced acute lung injury. Am J Physiol Lung Cell Mol Physiol 2000;279:L1137–L1145. [PubMed]
28. Wang XQ, Bdeir K, Yarovoi S, Cines DB, Fang W, Abraham E. Involvement of the urokinase kringle domain in lipopolysaccharide-induced acute lung injury. J Immunol 2006;177:5550–5557. [PubMed]
29. Kushnareva Y, Murphy AN, Andreyev A. Complex I-mediated reactive oxygen species generation: modulation by cytochrome c and NAD(p)+ oxidation-reduction state. Biochem J 2002;368:545–553. [PubMed]
30. Li N, Ragheb K, Lawler G, Sturgis J, Rajwa B, Melendez JA, Robinson JP. Mitochondrial complex I inhibitor rotenone induces apoptosis through enhancing mitochondrial reactive oxygen species production. J Biol Chem 2003;278:8516–8525. [PubMed]
31. Fiskum G, Starkov A, Polster BM, Chinopoulos C. Mitochondrial mechanisms of neural cell death and neuroprotective interventions in Parkinson's disease. Ann N Y Acad Sci 2003;991:111–119. [PubMed]
32. Barrientos A, Moraes CT. Titrating the effects of mitochondrial complex I impairment in the cell physiology. J Biol Chem 1999;274:16188–16197. [PubMed]
33. Isenberg JS, Klaunig JE. Role of the mitochondrial membrane permeability transition (MPT) in rotenone-induced apoptosis in liver cells. Toxicol Sci 2000;53:340–351. [PubMed]
34. Sim S, Yong TS, Park SJ, Im KI, Kong Y, Ryu JS, Min DY, Shin MH. NADPH oxidase-derived reactive oxygen species-mediated activation of ERK1/2 is required for apoptosis of human neutrophils induced by Entamoeba histolytica. J Immunol 2005;174:4279–4288. [PubMed]
35. Chen K, Thomas SR, Albano A, Murphy MP, Keaney JF Jr. Mitochondrial function is required for hydrogen peroxide-induced growth factor receptor transactivation and downstream signaling. J Biol Chem 2004;279:35079–35086. [PubMed]
36. Zhang DX, Gutterman DD. Mitochondrial reactive oxygen species-mediated signaling in endothelial cells. Am J Physiol Heart Circ Physiol 2007;292:H2023–H2031. [PubMed]
37. Chandel NS, Trzyna WC, McClintock DS, Schumacker PT. Role of oxidants in NF-kappa B activation and TNF-alpha gene transcription induced by hypoxia and endotoxin. J Immunol 2000;165:1013–1021. [PubMed]
38. Ghosh S, Karin M. Missing pieces in the NF-kappaB puzzle. Cell 2002;109:S81–S96. [PubMed]
39. Ben-Neriah Y. Regulatory functions of ubiquitination in the immune system. Nat Immunol 2002;3:20–26. [PubMed]
40. Alkalay I, Yaron A, Hatzubai A, Jung S, Avraham A, Gerlitz O, Pashut-Lavon I, Ben-Neriah Y. In vivo stimulation of I kappa B phosphorylation is not sufficient to activate NF-kappa B. Mol Cell Biol 1995;15:1294–1301. [PMC free article] [PubMed]
41. Quillet-Mary A, Jaffrezou JP, Mansat V, Bordier C, Naval J, Laurent G. Implication of mitochondrial hydrogen peroxide generation in ceramide-induced apoptosis. J Biol Chem 1997;272:21388–21395. [PubMed]
42. Ulvik R, Romslo I. Effect of thenoyltrifluoroacetone on oxygen consumption and energy conservation in isolated rat liver mitochondria. FEBS Lett 1975;59:180–183. [PubMed]
43. Josse C, Legrand-Poels S, Piret B, Sluse F, Piette J. Impairment of the mitochondrial electron chain transport prevents NF-kappa B activation by hydrogen peroxide. Free Radic Biol Med 1998;25:104–112. [PubMed]
44. McCracken RO, Carr AW, Stillwell WH, Lipkowitz KB, Boisvenue R, O'Doherty GO, Wickiser DI. Trifluoromethanesulfonamide anthelmintics: protonophoric uncouplers of oxidative phosphorylation. Biochem Pharmacol 1993;45:1873–1880. [PubMed]
45. Beckman JS, Minor RL Jr, White CW, Repine JE, Rosen GM, Freeman BA. Superoxide dismutase and catalase conjugated to polyethylene glycol increases endothelial enzyme activity and oxidant resistance. J Biol Chem 1988;263:6884–6892. [PubMed]
46. Teoh ML, Sun W, Smith BJ, Oberley LW, Cullen JJ. Modulation of reactive oxygen species in pancreatic cancer. Clin Cancer Res 2007;13:7441–7450. [PubMed]
47. Ramachandran A, Ceaser E, Darley-Usmar VM. Chronic exposure to nitric oxide alters the free iron pool in endothelial cells: role of mitochondrial respiratory complexes and heat shock proteins. Proc Natl Acad Sci USA 2004;101:384–389. [PubMed]
48. Ceaser EK, Ramachandran A, Levonen AL, Darley-Usmar VM. Oxidized low-density lipoprotein and 15-deoxy-delta 12,14-PGJ2 increase mitochondrial complex I activity in endothelial cells. Am J Physiol Heart Circ Physiol 2003;285:H2298–H2308. [PubMed]
49. Van den Berghe G, Wilmer A, Hermans G, Meersseman W, Wouters PJ, Milants I, Van Wijngaerden E, Bobbaers H, Bouillon R. Intensive insulin therapy in the medical ICU. N Engl J Med 2006;354:449–461. [PubMed]
50. Van den Berghe G, Wouters P, Weekers F, Verwaest C, Bruyninckx F, Schetz M, Vlasselaers D, Ferdinande P, Lauwers P, Bouillon R. Intensive insulin therapy in the critically ill patients. N Engl J Med 2001;345:1359–1367. [PubMed]
51. Brunmair B, Staniek K, Gras F, Scharf N, Althaym A, Clara R, Roden M, Gnaiger E, Nohl H, Waldhausl W, et al. Thiazolidinediones, like metformin, inhibit respiratory complex I: a common mechanism contributing to their antidiabetic actions? Diabetes 2004;53:1052–1059. [PubMed]
52. Lekstrom-Himes JA, Kuhns DB, Alvord WG, Gallin JI. Inhibition of human neutrophil IL-8 production by hydrogen peroxide and dysregulation in chronic granulomatous disease. J Immunol 2005;174:411–417. [PubMed]
53. Reynaert NL, van der Vliet A, Guala AS, McGovern T, Hristova M, Pantano C, Heintz NH, Heim J, Ho YS, Matthews DE, et al. Dynamic redox control of NF-kappaB through glutaredoxin-regulated S-glutathionylation of inhibitory kappaB kinase beta. Proc Natl Acad Sci USA 2006;103:13086–13091. [PubMed]
54. Kanayama A, Inoue J, Sugita-Konishi Y, Shimizu M, Miyamoto Y. Oxidation of Ikappa Balpha at methionine 45 is one cause of taurine chloramine-induced inhibition of NF-kappa B activation. J Biol Chem 2002;277:24049–24056. [PubMed]
55. Toledano MB, Leonard WJ. Modulation of transcription factor NF-kappa B binding activity by oxidation-reduction in vitro. Proc Natl Acad Sci USA 1991;88:4328–4332. [PubMed]
56. Lu Y, Wahl LM. Oxidative stress augments the production of matrix metalloproteinase-1, cyclooxygenase-2, and prostaglandin E2 through enhancement of NF-kappa B activity in lipopolysaccharide-activated human primary monocytes. J Immunol 2005;175:5423–5429. [PubMed]
57. Khadaroo RG, Kapus A, Powers KA, Cybulsky MI, Marshall JC, Rotstein OD. Oxidative stress reprograms lipopolysaccharide signaling via SRC kinase-dependent pathway in raw 264.7 macrophage cell line. J Biol Chem 2003;278:47834–47841. [PubMed]
58. True AL, Rahman A, Malik AB. Activation of NF-kappaB induced by H(2)O(2) and TNF-alpha and its effects on ICAM-1 expression in endothelial cells. Am J Physiol Lung Cell Mol Physiol 2000;279:L302–L311. [PubMed]
59. Nill MR, Oberyszyn TM, Ross MS, Oberyszyn AS, Robertson FM. Temporal sequence of pulmonary cytokine gene expression in response to endotoxin in C3H/hen endotoxin-sensitive and C3H/hej endotoxin-resistant mice. J Leukoc Biol 1995;58:563–574. [PubMed]
60. Lin HZ, Yang SQ, Chuckaree C, Kuhajda F, Ronnet G, Diehl AM. Metformin reverses fatty liver disease in obese, leptin-deficient mice. Nat Med 2000;6:998–1003. [PubMed]
61. Marchesini G, Brizi M, Bianchi G, Tomassetti S, Zoli M, Melchionda N. Metformin in non-alcoholic steatohepatitis. Lancet 2001;358:893–894. [PubMed]
62. Hattori Y, Suzuki K, Hattori S, Kasai K. Metformin inhibits cytokine-induced nuclear factor kappab activation via AMP-activated protein kinase activation in vascular endothelial cells. Hypertension 2006;47:1183–1188. [PubMed]
63. El-Mir MY, Nogueira V, Fontaine E, Averet N, Rigoulet M, Leverve X. Dimethylbiguanide inhibits cell respiration via an indirect effect targeted on the respiratory chain complex I. J Biol Chem 2000;275:223–228. [PubMed]

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