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First published online 19 December 2006
doi: 10.1242/jcs.03318
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Research Article |
Department of Medicine, Duke University Medical Center, Durham, NC 27710, USA
* Author for correspondence (e-mail: piant001{at}mc.duke.edu)
Accepted 26 October 2006
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Summary |
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, and of mitochondrial transcription factor A (TFAM), which augmented the copy number of mitochondrial DNA (mtDNA). This is independent of nitric oxide synthase (NOS), as demonstrated by the identical responses in wild-type and endothelial NOS (eNOS)-deficient mice, and by the inhibition of inducible NOS (iNOS). In the heart and in isolated cardiomyocytes, CO activation involved both guanylate cyclase and the pro-survival kinase Akt/PKB. Akt activation was facilitated by mitochondrial binding of CO and by production of hydrogen peroxide (H2O2). Interference with Akt activity by blocking PI 3-kinase and by mitochondrial targeting of catalase to scavenge H2O2 prevented binding of NRF1 to the Tfam promoter, thereby connecting mitochondrial H2O2 to the pathway leading to mtDNA replication. The findings disclose mitochondrial CO and H2O2 as new activating factors in cardiac mitochondrial biogenesis.
Key words: Reactive oxygen species, Carbon monoxide, Heme oxygenase, Nitric oxide, Mitochondrial DNA
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Introduction |
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; Piantadosi, 2002), but also allow for adaptation (Maines, 1988; Thom et al., 2000). Endogenous CO produced by heme catabolism has physiological roles in eukaryotic cells (Verma et al., 1993), and both endogenous and exogenous CO ameliorate experimental cardiac, lung and vascular injuries (Otterbein et al., 2003; Sato et al., 2001; Song et al., 2003), and protect against certain inflammatory states (Fujita et al., 2001). Thus, CO can exhibit anti-inflammatory (Wagener et al., 2003), anti-proliferative (Taille et al., 2003) and anti-apoptotic effects (Zhang et al., 2003) by largely undetermined physiological mechanisms.
The cellular physiology of CO is complex because the gas binds to multiple heme proteins, including cytochrome P450, guanylate cyclase and cytochrome c oxidase (Coburn and Forman, 1987). The latter inhibits mitochondrial electron transport, which can be deleterious to aerobic contractile function (Liao et al., 1996). However, we considered that the physiological activities of CO might be linked to oxidative metabolism (especially with respect to adaptation) by optimizing mitochondrial biogenesis. This requires nuclear and mitochondrial genomic orchestration by regulatory factors, including nitric oxide (NO), which activates guanylate cyclase and yields transcriptional response of, for example, peroxisome proliferator-activated receptor gamma coactivator 1 alpha (PPARGC1A, hereafter referred to as PGC-1) (Nisoli and Carruba, 2006; Nisoli et al., 2003).
CO specifically binds to reduced cytochrome a3 but has a weak affinity for guanylate cyclase – much less than NO – and, therefore, may be poised to play a complementary role in mitochondrial biogenesis. This idea derives from observations that cytochrome c oxidase naturally metabolizes CO to carbon dioxide (CO2) (Young and Caughey, 1986), binding of CO to cytochrome oxidase a3 heme increases the mitochondrial H2O2 leak rate (Zhang and Piantadosi, 1992), and the pro-survival phosphatidylinositide 3-kinase (PI3-K)/Akt pathway (Cantley, 2002) activates replication of mitochondrial DNA (mtDNA) by oxidant-dependent regulation of phosphorylation of nuclear respiratory factor 1 (NRF1) and expression of Tfam (Piantadosi and Suliman, 2006). Our hypothesis was that mitochondrial H2O2 production deriving from CO binding to cytochrome c oxidase is an activating factor in mitochondrial biogenesis.
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Results |
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In mice, cardiac mitochondrial protein content increased for all five respiratory complexes by 2D gel electrophoresis within 24 hours of CO exposure (Fig. 1B). Mitochondrial state–state-3 respiration and coupling were preserved, although succinate-linked state-3 increased after CO (Fig. 1C). Low temperature spectra (77°K) of succinate-stimulated mitochondria before and after CO incubations demonstrated the formation of a CO–cytochrome-a3 complex and early selective reduction of the cytochrome bc1 region of the chain (Fig. 1D). As detected by electron microscopy (EM), the cross-sectional area and, hence, volume density of interfibrillar mitochondria increased at 24 hours by 
30%, and was accompanied by profuse budding and ultrastructual heterogeneity characteristic of mitochondrial biogenesis (Fig. 1E). Overall, Fig. 1 illustrates that CO activates cardiac mitochondrial biogenesis in vivo.
In mouse heart tissue, the physiological CO concentration was on average 9 picomoles/mg and increased five- to 20-fold after 1 hour of incubation with CO (Fig. 2A, left panel). The intracellular CO content rose rapidly with the formation of carboxyhemoglobin (COHb), which increases the tissue capillary diffusion barrier and causes retention of endogenous CO (Cronje et al., 2004). At 6 hours, cellular CO concentration had declined to baseline (not shown) but expression of PGC-1 mRNA had increased (Fig. 2A, middle) in relation to the measured cardiac CO concentration (Fig. 2A, right).
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A comparison of wild-type (Wt) mice and endothelial nitric oxide synthase (eNOS)-deficient (eNOS–/–) mice was performed to evaluate the role of NO in CO-induced mitochondrial biogenesis (Clementi and Nisoli, 2005; Nisoli and Carruba, 2006; Nisoli et al., 2003; Nisoli et al., 2004). In Wt and eNOS–/– strains, mRNA expression for the mitochondrial transcription factor A (TFAM) and DNA polymerase 
(Pol) was increased after treatment with CO, and cardiac TFAM and Pol protein had tripled at 24 hours (Fig. 2B, left and middle panels for western blots). Cardiac mtDNA content increased in both strains (Fig. 2B, right). The initial mtDNA content was lower in eNOS–/– than Wt hearts, but increased 2.5- to 3-fold in both strains after treatment with CO, demonstrating eNOS-independence. The possibility that inducible NOS (iNOS) caused the CO response in eNOS–/– mice was excluded by inhibiting iNOS with 1400 W (Cayman Chemical, Ann Arbor, MI), which did not alter the responses (data not shown).
The levels of mRNA for NRF1, NRF2 and PGC-1, the transcription factors and the coactivator that regulate mitochondrial biogenesis, responded to the presence of CO in Wt and eNOS–/– mouse hearts followed by Tfam mRNA expression (Fig. 3A-D). In Wt mice, mRNA of PGC-1 peaked at 2 hours (Fig. 3A, fourfold; P<0.05), of NRF1 and NRF2 at 2-6 hours (Fig. 3B,C, four- to sixfold; P<0.05) and of Tfam at 24 hours (Fig. 3D, fivefold; P<0.01). In eNOS–/– mice, levels of these transcripts were lower than in Wt mice but the temporal profiles were comparable.
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or NRF1 (Fig. 3E,F). To confirm the requirement for binding of CO to heme protein in vivo, CO treatment was given in conjunction with hyperbaric oxygen to prevent binding of CO to reduced cytochrome a3 by raising mitochondrial PO2 levels (Piantadosi, 2002). Hyperbaric oxygen abrogated the effect of CO on mRNA levels of both proteins.
Activation of p38 MAP kinase and PI3-K/Akt
Mitogen-activated protein (MAP) kinases, most notably p38, are activated by reactive oxygen species (ROS) (Sugden and Clerk, 1998) and by CO (Zhang et al., 2003). We used the p38 inhibitor SB203580 in vivo to prevent CO-induced phosphorylation of cardiac p38 (Fig. 4A). SB203580 did not affect mRNA levels of PGC-1, NRF1 or Tfam, or the increase in mtDNA in Wt or eNOS–/– mice after treatment with CO (Fig. 4A).
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The pro-survival, anti-apoptotic serine/threonine kinase Akt is cardioprotective, in part by phosphorylating and activating eNOS (Dimmeler et al., 1999). CO activates cardiac Akt in Wt and eNOS–/– mice (Fig. 4B, top, P<0.05, densitometry not shown). Akt activation had the expected anti-apoptotic effect, e.g. phosphorylation of Bad (Fig. 4B, middle) (Matsui et al., 2001). In Wt mice, hypoxia (or treatment with hyperbaric oxygen and CO as negative control) did not yield phosphorylation of Akt; moreover, inhibition of p38 did not prevent Akt activation (Fig. 4B, bottom panel). Akt activation by CO, however, was attenuated more than 50% by inhibiting heme oxygenase (data not shown), supporting the hypothesis that cardiac Akt is also activated by endogenous CO.
Role of H2O2
Rat heart H9c2 cells were treated with the CO-generating molecule dichloromethane (DCM) to increase cellular CO levels via cytochrome P450 activity (Kubic and Anders, 1975). CO dose and CO time responses are shown in Fig. 5A (left panel) with cGMP production (middle panel). Mitochondrial viability and function, assessed by MTT assay, was initially unaffected (at 12-24 hours) but increased significantly 36 and 48 hours after treatment with DCM and CO generation, commensurate with mitochondrial biogenesis (Fig. 5A, right panel).
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In H9c2 cells, CO led to Akt and p38 phosphorylation, but we focused on Akt because the in vivo data did not implicate p38. Moreover, CO-activated Akt phosphorylation in H9c2 cells was unaffected by p38 inhibition, partially abrogated by guanylate cyclase inhibition, and blocked by PI3-K inhibition (Fig. 5D). Full Akt expression was also reduced by heme oxygenase inhibition (data not shown). Akt activation by CO was disrupted by the insertion of catalase into the mitochondria (Fig. 5D), thus demonstrating a role for mitochondrial H2O2 in Akt regulation.
Activation of mitochondrial biogenesis in H9c2 cells by CO was indicated by three- to fourfold increases in NRF1, NRF2, PGC-1 and TFAM protein expression by western blot analysis (Fig. 5E). Guanylate cyclase blockade halved the CO response, but p38 blockade had no effect. By contrast, inhibition of PI3-K/Akt blocked expression of NRF1 and TFAM and attenuated that of PGC-1 and NRF2 (Fig. 5E). CO also increased the copy number of mtDNA, which was prevented by inhibition of guanylate cyclase or PI3-K but not p38 (Fig. 5F).
NRF1 and PGC-1 are binding partners in Tfam expression; therefore NRF1 binding to PGC-1 was checked by co-immunoprecipitation (Fig. 6). NRF1–PGC-1 binding was enhanced in H9c2 cells after treatment with CO, and was sensitive to PI3-K/Akt inhibition. Tfam promoter activation by NRF1 and NRF2 by CO was demonstrated by chromatin immunoprecipitation assay (Fig. 6B). NRF1-Tfam promoter binding after CO in H9c2 cells was abrogated by mitochondrial-targeted catalase (Fig. 6B).
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Discussion |
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Mitochondrial biogenesis is regulated by the coordinated expression of specialized nuclear transcription factors that activate genes for mitochondrial proteins (Hood, 2001; Hood et al., 2003). These transcriptional elements were stimulated by CO in the mouse heart by a hypoxia-independent effect. The transcriptional activation mechanisms are not delineated here, but the responses produced significant increases in the copy number of mtDNA, content of OXPHOS protein and mitochondrial density in vivo. The response to CO was confirmed in cardiomyocytes, which in association with cGMP expression and mitochondrial ROS production also showed apposite increases mitochondrial DNA synthesis and functional mitochondria.
The increases in cardiac mtDNA content in Wt and eNOS–/– mice were the same, unaffected by iNOS inhibition and, in view of the low nNOS content of the heart, support NO-independent effects of CO on mitochondrial biogenesis. The molecular data imply an overlap in the mechanism of action of the two gases: NO relies on guanylate cyclase (Nisoli et al., 2003), whereas CO has dual guanylate-cyclase-dependent and guanylate-cyclase-independent effects – the latter requires mitochondrial production of H2O2 and activation of Akt.
CO requires classical O2-dependent heme-protein binding demonstrated by the effect of hyperbaric oxygen, which keeps oxylabile transition metal centers in the oxidized state. This test is definitive because CO binds only reduced cytochrome oxidase a3 heme in intact mitochondria (Coburn and Forman, 1987; Piantadosi, 2002). CO elicits other features of mitochondrial redox signaling: inhibition of electron transport (Coburn and Forman, 1987), H2O2 generation (Zhang and Piantadosi, 1992) and reversibility by oxygenation (Young and Caughey, 1986).
The binding of CO to cytochrome a3 promotes reduction of the respiratory carriers in the cytochrome bc1 region, raising PO2 levels and increasing mitochondrial H2O2 production (Zhang and Piantadosi, 1992), shown here by low-temperature heart-muscle spectra and CC-1 cell labeling studies suggesting an accelerated mitochondrial H2O2 leak rate. CO also upregulates SOD2, which scavenges superoxide, augments mitochondrial H2O2 release, and may modulate redox signaling (Zhang et al., 2002). In cardiomyocytes, mitochondrial CC-1 uptake in the presence of CO was blocked by mitochondrial-targeted catalase. The loss of mitochondrial H2O2 disrupted Akt activation, NRF1 phosphorylation and its binding to the Tfam promoter, events that can be regulated by H2O2 (Piantadosi and Suliman, 2006). This role of mitochondrial H2O2 is also consistent with the ability of exogenous peroxides to increase cell mitochondrial mass (Lee et al., 2002; Piantadosi and Suliman, 2006).
Mitochondrial biogenesis entails mtDNA replication and transcription, which depend on nuclear-encoded transcription of Tfam (Moraes, 2001) regulated by NRF1 and NRF2 in association with PGC-1 (Virbasius and Scarpulla, 1994; Wu et al., 1999). NRF1 and NRF2 also partner with PGC-1 to activate other components of mitochondrial biogenesis (Kelly and Scarpulla, 2004; Schreiber et al., 2003) including genes encoding components of the respiratory subunit, e.g. cytochrome c and ATP synthase (Kelly and Scarpulla, 2004; Schreiber et al., 2003). PGC-1 is activated by cGMP (Nisoli et al., 2003) and transcriptional activity of GA-repeat-binding protein (mouse NRF2 homologue) forms a positive feedback loop that drives nuclear gene expression for mitochondrial proteins (Mootha et al., 2004).
CO activates two requisite processes in the current paradigm for mitochondrial biogenesis. First, like NO, CO activates guanylate cyclase which promotes mitochondrial biogenesis. Second, CO activates Akt through an established oxidant mechanism involving NRF1, which in concert with NRF2 activates Tfam expression. cGMP may also influence PI3-K-Akt signaling (Li et al., 2000), but H2O2 activates Akt by oxidizing cysteine in counter-regulatory phosphatases, such as PTEN, that oppose PI3-K (Leslie et al., 2003). In H9c2 cells, Akt activation by CO was eliminated by two structurally dissimilar PI3-K inhibitors. Likewise, Tfam expression was inhibited, confirming the importance of this pathway in Tfam regulation (Piantadosi and Suliman, 2006). Akt activation was abrogated by mitochondrial-targeted catalase, establishing mitochondrial H2O2 as a signal. By contrast, guanylate cyclase inhibition interfered little with Akt activation by CO, thereby implicating H2O2 as the primary PI3-K/Akt activation mechanism in this case.
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) but we could not implicate it in early activation of mitochondrial biogenesis. We did not explore the disruption of PGC-1 binding to p160 myb – a negative regulator of its transcriptional activity and of respiration (Fan et al., 2004) – by p38 or the cross-talk postulated between p38 and PI3-K/Akt (Iwasa et al., 2003), because p38 signaling in the heart is complex. Some studies have found p38 protective (Baines et al., 1999), whereas others find it pro-apoptotic (Petrich and Wang, 2004; Ren et al., 2005).
An interpretation of picomolar CO as a respiratory inhibitor must be placed in the context of micromolar cytochrome oxidase in the heart. The CO to cytochrome a3 stoichiometry was too low to compromise aerobic energy production to the point of damage, and indicated a high gain of mitochondrial biogenesis to mitochondrial oxidation-reduction state. For instance, the spectral data suggest that the CO:O2 ratio adjusts electron transport in conjunction with the Q cycle to regulate superoxide production and the H2O2 leak rate via SOD2 (Trumpower, 1990; Zhang et al., 2002) (Fig. 7). CO is advantaged by binding only the reduced cytochrome oxidase a3 heme, whereas other terminal inhibitors, such as CN and NO, bind both ferrous (Fe2+) and ferric (Fe3+) heme. Work on those gases will be of interest but, like CO, requires care to avoid ATP depletion and additional stimulation of biogenesis. Because the Michaelis-Menten constant (Km) of cytochrome c oxidase for O2 is low, the reduced cytochrome oxidase a3 heme available to react with CO is also low, but increases under hypoxic and State 3 conditions (Chance et al., 1970).
Two observations regarding CO and hypoxia are relevant from a physiological perspective. First, the induction of hypoxia by COHb might directly activate Akt, eNOS and certain MAP kinases. This possibility was excluded by hypoxia-controls in mice and in H9c2 cells; picomolar CO stimulated mitochondrial biogenesis in aerobic conditions, mitigating hypoxia as the direct cause. Second, COHb delays endogenous CO clearance both by decreasing the PO2 level and by increasing the gas back-pressure in tissue (Cronje et al., 2004). This is a simple explanation for the rapid cytoprotection by CO that may recapitulate HO-1 induction (Akamatsu et al., 2004; Fujita et al., 2001). CO and hypoxia also induce HO-1 and mitochondrial heme release (Cronje et al., 2004; Piantadosi et al., 2006), and heme oxygenase inhibition attenuates Akt activation, thus also implicating endogenous CO in mitochondrial biogenesis. The effect is not simple, however, and was set aside for the mitochondrial H2O2 mechanism which gives purview to endogenous CO.
With respect to adaptation and cell survival, our evidence is preliminary: CO influences the mitochondrial phenotype by upregulating TFAM, SOD2, the anti-apoptotic pBAD and the resting energy expenditure. We noticed relative activation of complex II after CO despite uniform increases in respiratory complex proteins, which could, in principle, reflect differential assembly, regulation or other adaptive strategies that require energy (Fujita et al., 2001; Wagener et al., 2003). These speculations require confirmation and future investigation.
In summary, modest increases in cellular CO concentration activate mitochondrial biogenesis by a set of molecular responses that includes mitochondrial H2O2 production, activation of guanylate cyclase and Akt, and induction of HO-1, independently of eNOS, iNOS and hypoxia. We impute from the physiological behavior of CO that exogenous and endogenous CO interact, and conjecture that endogenous CO participates in accordance with heme turnover and CO clearance rates. These findings have both adaptive and pathogenic implications for conditions that substantially raise the tissue CO content and produce oxidative stress, such as smoking, air pollution, and CO poisoning, and hemolytic or inflammatory states that accelerate heme turnover.
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Materials and Methods |
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Pre-mixed CO was directed into exposure chambers at 6 l/minute (Cronje et al., 2004) and levels were monitored with a CO analyzer (Interscan, Chatsworth, CA). To control for changes in PO2, some mice were exposed to conditions mimicking higher altitude (24,000 ft) or hyperbaric conditions (final pressure 5ATA±CO). Others received intraperitoneal (i.p.) injections of 50 µg of the heme oxygenase inhibitor Sn-protoporphyrin (SnPP), of vehicle (DMSO) with or without CO or of p38 inhibitor at 4 hours and 1 hour before treatment with CO (i.p. SB2035801, TOCRIS, Ellisville, MO); control mice received vehicle (0.2 ml 5% DMSO). After euthanasia, hearts were removed for immediate use, were flash-frozen or fixed by perfusion for light microscopy and transmission electron microscopy (TEM) (Suliman et al., 2004). For EM, hearts underwent retro-aortic perfusion first with cold PBS, then with 2% paraformaldehyde and 1% glutaraldehyde in 0.1 M PBS (pH 7.4). Multiple 1-2-mm cubes of the left ventricle were cut and randomly selected for EM. After embedding, ultrathin sections (60 nm) were cut, contrasted with uranyl acetate followed by lead citrate and examined by TEM (Phillips CM12).
Tissue CO analysis was done by calibrated reduction gas chromatography (GC; RGA5; Trace Analytical, Menlo Park, CA, detection limit 1 pM) (Cronje et al., 2004). Duplicate blood-free heart or 1 x 107 cardiomyocyte samples were homogenized in cold PBS (pH 7.0) then homogenized by ultrasound for 1 minute on ice. Homogenates were spun at 2000 g for 20 seconds and 20-60 µl supernatant was placed in 2-ml vials containing 0.5% sulfosalicylic acid, used to release CO into the headspace.
Mitochondrial DNA copy number
The mtDNA copy number was quantified by competitive PCR using co-amplification of a target template with a known amount of competitor (Suliman et al., 2003a). Mouse cytochrome-b-specific primers 14335 5'-CATCAGTAACACACATTTGT-3' and 14906 5'-GATTAGCTGGTATGTAGTTG-3' amplify 571 bp of the target mtDNA and 332 bp of the competitor DNA when cut with SimI. Triplicate samples of 2 x 103 copies of competitor and 50 ng of target mtDNA were co-amplified in a thermal cycler (PE Applied Biosystems, Foster City, CA) using product optimization on ethidium bromide (EB)-stained gels in the exponential phase. PCR products were separated by electrophoresis in 2% agarose. EB-stained band intensities were measured by densitometry and mtDNA-specific products plotted against competitor density on a log-scale. Copy number was determined from the x intercept or the point at which the ratio of the 571-bp and 332-bp products was 1. A factor of 1.7 was used to correct for molecular weight.
Mitochondrial protein, function and spectra
Fresh cardiac interfibrillar mitochondria were isolated, their yield was determined and respiratory complexes were separated by Blue native polyacrylamide gel electrophoresis (BN-PAGE) (Suliman et al., 2004). Samples (2 mg) were mixed in 6-aminocaproic acid (200 µl 0.75 M) Bis-Tris (50 mM, pH 7.0) and 37.5 µl DDM (10%), centrifuged (100,000 g) and Serva Blue was added to the supernatant before 4-12% gradient electrophoresis. Complexes were identified by elution order and in-gel activity stains. Peptides were resolved by 2D Tricine-SDS-PAGE electrophoresis; BN-PAGE bands were excised, incubated in 1% SDS/1% mercaptoethanol for 2 hours and loaded onto 16% separating gels. After electrophoresis, gels were stained with Coomassie Blue followed by silver. Multiple sets of gels, each with tissue from one control and one CO-exposed mouse were carried simultaneously through separation, staining and densitometry. Low-temperature difference spectra of rat heart mitochondria, frozen in 50% glycerol after reduction with sodium dithionite or 1% CO gas, using oxygenated mitochondria as a reference, were used to demonstrate binding of CO to cytochrome-a3 and reduction of the cytochrome-bc1 region (Piantadosi, 1989). Mitochondrial function was assessed by polarography in 2-ml thermostatically controlled glass chambers or by conversion of 3-(4,5-dimethylthiazol-2-yl)-2,5-diphenyl-tetrazolium) bromide (MTT) to formazan. H9c2 cells were plated at a density of 5 x 104 cells/well in 96-well plates and exposed to DCM at 37°C and 5% CO2 and stained with MTT. The formazan was dissolved with DMSO and absorbance measured at 540 nm on a plate reader. MTT reduction was defined by untreated controls [100x (absorbance of treated cells) ÷ (absorbance of control cells)].
Western blot analysis
Proteins were separated by SDS-PAGE (Suliman et al., 2003b). Membranes were incubated with validated polyclonal rabbit Abs against mouse PGC-1, NRF1, TFAM, and Pol, or Akt, pAkt, p38, p-p38 and SOD2 (Santa Cruz Biotechnology, Santa Cruz, CA), or anti-tubulin or 
-actin (1:1000; Sigma). After five washes in TBST, membranes were incubated at a 1:10,000 dilution of HRP-conjugated goat anti-rabbit or anti-mouse IgG (Amersham). Blots were developed with ECL, proteins quantified on digitized images from the mid-dynamic range and expressed relative to tubulin or -actin.
RNA extraction and real time quantitative PCR
Total RNA was prepared from heart or H9c2 cells using Trizol reagent (Invitrogen Corp., Carlsbad, CA). One µg of RNA was reverse-transcribed using Random Hexomer primers and a Superscript enzyme (Invitrogen). Real-time reverse transcriptase (RT)-PCR was performed using the ABI Prism 7000 and SYBR Green master mix (Applied Biosystems, Foster City, CA). After PCR, samples were subjected to melting curve analysis. 18S RNA or -actin were used as internal controls. ABI Prism 7000 SDS Software was used to quantify differences in gene expression. The threshold cycle (Ct) was determined in the exponential amplification phase. The amount of transcript was normalized to 18S RNA or -actin by subtracting the mean Ct values for each condition. Because of the exponential PCR reaction, a difference of n in Ct values represents a twofold difference in transcript levels. PCR was performed in triplicate.
Cell culture
H9c2 cells (embryonic rat cardiomyocytes, ATCC, Rockville, MD) were maintained in Dulbecco's modified Eagle's medium (DMEM; Invitrogen) supplemented with 10% fetal bovine serum (Invitrogen) and 2 mmol/l L-glutamine. Cells were incubated with dichloromethane (DCM, 10-150 µM) diluted in 10% DMSO using 10% DMSO in controls. SKF-525A, ODQ, SB203580, Wortmannin and LY294002 were added 30 minutes before treatment at final concentrations of 20 µM, 20 µM, 10 µM, 20 nM, and 25 µM, respectively. H9c2 cells grown to confluence on 96-well plates were assayed with the BioTrak kit (Amersham Pharmacia). Cells were pre-treated for 10 minutes with 0.2 mM IBMX to prevent cGMP degradation followed by DCM/CO. Cells were lysed, centrifuged and supernatants mixed with rabbit anti-cGMP Ab. Aliquots were added to 96-well plates pre-coated with anti-rabbit Ab cGMP-peroxidase conjugate, washed, and peroxidase substrate added. The reaction was terminated with H2SO4 and OD450 was read against standards.
In situ oxidant detection
Redox Sensor Red CC-1 dye (CC-1; Molecular Probes, Eugene, OR), which localizes upon oxidation to mitochondria or lysozomes was used with mitochondrial-selective dye MitoTracker Green FM (MitoTracker; Molecular Probes). H9c2 cells at near confluence were exposed to CO (100 µM DCM) for 8 and 24 hours, and CC-1 (5 µM) and MitoTracker (1 µM) were added for 10 minutes at 37°C. Cells were washed twice in PBS. Localization of MitoTracker (488 nm) and CC-1 (568 nm) was examined using an LSCM (Model 410; Carl Zeiss MicroImaging Inc.). Control and treated samples were scanned at identical parameters and magnification. Confocal images were collected in fluorescence mode followed by electronic image merging.
Plasmids expressing mitochondrial-targeted catalase
Mitochondrial-targeted catalase (mtCAT)-expression vectors were constructed as a chimeric cDNA of mouse MnSOD mitochondrial leader sequence and mouse CAT. The MnSOD leader sequence was amplified using a sense primer flanked by a NheI restriction site (5'-GCTAGCGTGTAAACCTCAATAATGTTGTGTCGG-3') and an antisense primer flanked by an Hpy188I restriction site (5'-GTCCGACATTGCCGGGAGCCCGCGGCCA-3'). The mouse CAT-coding sequence (GenBank accession number X52108) was equipped with an Hpy188I site at the 5' end with oligonucleotide linkers, using the primers 5'-ATGTCGGACAGTCGGGACCCAGC-3' and 5'-CAGGTTAGCTTTTCCCTTCGCAGCCAT-3'. PCR fragments of the leader sequence and CAT-coding region were cloned into pGEM-T System I (Promega, Madison, WI). The pGEM-T vector containing the mitochondrial leader sequence was linearized with Hpy188I; the catalase region was removed, treated with Hpy188I and ligated into the pGEM-T-MnSOD linearized vector. The MnSOD-CAT construct was subcloned in-frame into pcDNA3 expression vector. H9c2 cells were transfected with the DNA vector using FuGENE-HD (Roche) and expression verified by lack of H2O2 production using CC-1 dye. Cells transfected with the pcDNA3 vector lacking the insert were the controls.
Immunoprecipitation and CHIP assays
H9c2 cells were lysed and centrifuged at 16,000 g for 30 minutes. Supernatant proteins were cleared with mouse or rabbit IgG and immunoprecipitated with anti-PGC-1. Immunoprecipitates were resolved by SDS-10% PAGE and transferred to nitrocellulose membranes. NRF1 was detected by western blot analysis using a validated Ab.
H9c2 cells (4.0 x 106) cultured in 15 cm plates were treated with DCM (100 µM) for indicated times and then cross-linked with 1% formaldehyde for 7.5 minutes, harvested, and sonicated to 500bp fragments, incubated for 30 min at 37°C and quenched with 0.125 M glycine. Cells were washed with PBS, harvested and processed for ChIP It assay with anti-NRF1 or anti-NRF2. After ethanol precipitation, DNA was re-suspended in 200 µl/107 cells and 2-5 µl as PCR template. Input samples representing 1% of total DNA were diluted 1:5 and IP fractions 1:2. PCR was carried out on 1 µl samples using sense, 5'-GGCAGTTTGCTGCTGGGT-3', and antisense, 5'-GGCACTGTGGGAGGCCCA-3' primers that amplified a 331-bp segment of Tfam from –359 to –28 relative to the transcription start site (Piantadosi and Suliman, 2006).
Bromodeoxyuridine incorporation
H9c2 cells were grown in chamber slides and treated with DCM (100 µM) for 48 hours. Twelve hours before fixation, medium was changed to growth medium without pyruvate, uridine or antibiotics supplemented with 1 µM 5-bromo-2'-deoxy-uridine (BrdU) (Roche). After 12 hours, the medium was removed and the cultures were washed with pre-warmed HBSS (37°C). Cells were fixed at room temperature in 4% phosphate-buffered paraformaldehyde and 4% sucrose and washed in PBS. Fixed cells were incubated in methanol (–20°C) for 10 minutes and washed again with PBS. Cultures were incubated for 25 minutes at 37°C in 200 nM MitoTracker (Molecular Probes), washed in PBS and incubated 100 minutes at 37°C with mouse anti-BrdU Ab (Roche) in buffer, or buffer only. Cells were washed and incubated for 60 minutes at 37°C in goat anti-mouse FluoroLink Cy3-labeled Ab (Molecular Probes), rinsed, coverslipped and observed by fluorescence confocal microscopy (Zeiss 410 LSCM, 620x).
Statistics
Mouse and cell data were expressed as the mean + standard error (s.e.) for n=3-8 for each time and condition. Experimental and control group comparisons were carried out by Student's t-test. Time series data were analyzed by two-way ANOVA, with repeated measure corrections as indicated, and by Fisher's post-hoc test. P values of P<0.05 were considered significant.
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References |
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Akamatsu, Y., Haga, M., Tyagi, S., Yamashita, K., Graca-Souza, A. V., Ollinger, R., Czismadia, E., May, G. A., Ifedigbo, E., Otterbein, L. E. et al. (2004). Heme oxygenase-1-derived carbon monoxide protects hearts from transplant associated ischemia reperfusion injury. FASEB J. 18, 771-772.
Baines, C. P., Cohen, M. V. and Downey, J. M. (1999). Signal transduction in ischemic preconditioning: the role of kinases and mitochondrial K(ATP) channels. J. Cardiovasc. Electrophysiol. 10, 741-754.[Medline]
Cantley, L. C. (2002). The phosphoinositide 3-kinase pathway. Science 296, 1655-1657.
Chance, B., Erecinska, M. and Wagner, M. (1970). Mitochondrial responses to carbon monoxide toxicity. Ann. N. Y. Acad. Sci. 174, 193-204.[Medline]
Clementi, E. and Nisoli, E. (2005). Nitric oxide and mitochondrial biogenesis: a key to long-term regulation of cellular metabolism. Comp. Biochem. Physiol. 142A, 102-110.
Coburn, R. F. and Forman, H. J. (1987). Carbon Monoxide. Rockville, MD: American Physiological Society.
Cronje, F. J., Carraway, M. S., Freiberger, J. J., Suliman, H. B. and Piantadosi, C. A. (2004). Carbon monoxide actuates O(2)-limited heme degradation in the rat brain. Free Radic. Biol. Med. 37, 1802-1812.[CrossRef][Medline]
Dimmeler, S., Fleming, I., Fisslthaler, B., Hermann, C., Busse, R. and Zeiher, A. M. (1999). Activation of nitric oxide synthase in endothelial cells by Akt-dependent phosphorylation. Nature 399, 601-605.[CrossRef][Medline]
Fan, M., Rhee, J., St-Pierre, J., Handschin, C., Puigserver, P., Lin, J., Jaeger, S., Erdjument-Bromage, H., Tempst, P. and Spiegelman, B. M. (2004). Suppression of mitochondrial respiration through recruitment of p160 myb binding protein to PGC-1alpha: modulation by p38 MAPK. Genes Dev. 18, 278-289.
Fujita, T., Toda, K., Karimova, A., Yan, S. F., Naka, Y., Yet, S. F. and Pinsky, D. J. (2001). Paradoxical rescue from ischemic lung injury by inhaled carbon monoxide driven by derepression of fibrinolysis. Nat. Med. 7, 598-604.[CrossRef][Medline]
Hood, D. A. (2001). Contractile activity-induced mitochondrial biogenesis in skeletal muscle. J. Appl. Physiol. 90, 1137-1157.
Hood, D. A., Adhihetty, P. J., Colavecchia, M., Gordon, J. W., Irrcher, I., Joseph, A. M., Lowe, S. T. and Rungi, A. A. (2003). Mitochondrial biogenesis and the role of the protein import pathway. Med. Sci. Sports Exerc. 35, 86-94.
Iwasa, H., Han, J. and Ishikawa, F. (2003). Mitogen-activated protein kinase p38 defines the common senescence-signalling pathway. Genes Cells 8, 131-144.[Abstract]
Kelly, D. P. and Scarpulla, R. C. (2004). Transcriptional regulatory circuits controlling mitochondrial biogenesis and function. Genes Dev. 18, 357-368.
Kubic, V. L. and Anders, M. W. (1975). Metabolism of dihalomethanes to carbon monoxide. II. In vitro studies. Drug Metab. Dispos. 3, 104-112.[Abstract]
Lee, H. C., Yin, P. H., Chi, C. W. and Wei, Y. H. (2002). Increase in mitochondrial mass in human fibroblasts under oxidative stress and during replicative cell senescence. J. Biomed. Sci. 9, 517-526.[CrossRef][Medline]
Leslie, N. R., Bennett, D., Lindsay, Y. E., Stewart, H., Gray, A. and Downes, C. P. (2003). Redox regulation of PI 3-kinase signalling via inactivation of PTEN. EMBO J. 22, 5501-5510.[CrossRef][Medline]
Li, J., Yang, S. and Billiar, T. R. (2000). Cyclic nucleotides suppress tumor necrosis factor alpha-mediated apoptosis by inhibiting caspase activation and cytochrome c release in primary hepatocytes via a mechanism independent of Akt activation. J. Biol. Chem. 275, 13026-13034.
Liao, R., Nascimben, L., Friedrich, J., Gwathmey, J. K. and Ingwall, J. S. (1996). Decreased energy reserve in an animal model of dilated cardiomyopathy. Relationship to contractile performance. Circ. Res. 78, 893-902.
Maines, M. D. (1988). Heme oxygenase: function, multiplicity, regulatory mechanisms, and clinical applications. FASEB J. 2, 2557-2568.[Abstract]
Matsui, T., Tao, J., del Monte, F., Lee, K. H., Li, L., Picard, M., Force, T. L., Franke, T. F., Hajjar, R. J. and Rosenzweig, A. (2001). Akt activation preserves cardiac function and prevents injury after transient cardiac ischemia in vivo. Circulation 104, 330-335.
Mootha, V. K., Handschin, C., Arlow, D., Xie, X., St Pierre, J., Sihag, S., Yang, W., Altshuler, D., Puigserver, P., Patterson, N. et al. (2004). Erralpha and Gabpa/b specify PGC-1alpha-dependent oxidative phosphorylation gene expression that is altered in diabetic muscle. Proc. Natl. Acad. Sci. USA 101, 6570-6575.
Moraes, C. T. (2001). What regulates mitochondrial DNA copy number in animal cells? Trends Genet. 17, 199-205.[CrossRef][Medline]
Nisoli, E. and Carruba, M. O. (2006). Nitric oxide and mitochondrial biogenesis. J. Cell Sci. 119, 2855-2862.
Nisoli, E., Clementi, E., Paolucci, C., Cozzi, V., Tonello, C., Sciorati, C., Bracale, R., Valerio, A., Francolini, M., Moncada, S. et al. (2003). Mitochondrial biogenesis in mammals: the role of endogenous nitric oxide. Science 299, 896-899.
Nisoli, E., Clementi, E., Tonello, C., Moncada, S. and Carruba, M. O. (2004). Can endogenous gaseous messengers control mitochondrial biogenesis in mammalian cells? Prostaglandins Other Lipid Mediat. 73, 9-27.[CrossRef][Medline]
Otterbein, L. E., Zuckerbraun, B. S., Haga, M., Liu, F., Song, R., Usheva, A., Stachulak, C., Bodyak, N., Smith, R. N., Csizmadia, E. et al. (2003). Carbon monoxide suppresses arteriosclerotic lesions associated with chronic graft rejection and with balloon injury. Nat. Med. 9, 183-190.[CrossRef][Medline]
Petrich, B. G. and Wang, Y. (2004). Stress-activated MAP kinases in cardiac remodeling and heart failure; new insights from transgenic studies. Trends Cardiovasc. Med. 14, 50-55.[CrossRef][Medline]
Piantadosi, C. A. (1989). Spectrophotometry of b-type cytochromes in rat brain in vivo and in vitro. Am. J. Physiol. 256, C840-C848.[Medline]
Piantadosi, C. A. (2002). Biological chemistry of carbon monoxide. Antioxid. Redox Signal. 4, 259-270.[CrossRef][Medline]
Piantadosi, C. A. and Suliman, H. B. (2006). Mitochondrial transcription factor A induction by redox activation of nuclear respiratory factor 1. J. Biol. Chem. 281, 324-333.
Piantadosi, C. A., Carraway, M. S. and Suliman, H. B. (2006). Carbon monoxide, oxidative stress, and mitochondrial permeability pore transition. Free Radic. Biol. Med. 40, 1332-1339.[CrossRef][Medline]
Ren, J., Zhang, S., Kovacs, A., Wang, Y. and Muslin, A. J. (2005). Role of p38alpha MAPK in cardiac apoptosis and remodeling after myocardial infarction. J. Mol. Cell. Cardiol. 38, 617-623.[CrossRef][Medline]
Sato, K., Balla, J., Otterbein, L., Smith, R. N., Brouard, S., Lin, Y., Csizmadia, E., Sevigny, J., Robson, S. C., Vercellotti, G. et al. (2001). Carbon monoxide generated by heme oxygenase-1 suppresses the rejection of mouse-to-rat cardiac transplants. J. Immunol. 166, 4185-4194.
Schreiber, S. N., Knutti, D., Brogli, K., Uhlmann, T. and Kralli, A. (2003). The transcriptional coactivator PGC-1 regulates the expression and activity of the orphan nuclear receptor estrogen-related receptor alpha (ERRalpha). J. Biol. Chem. 278, 9013-9018.
Song, R., Kubo, M., Morse, D., Zhou, Z., Zhang, X., Dauber, J. H., Fabisiak, J., Alber, S. M., Watkins, S. C., Zuckerbraun, B. S. et al. (2003). Carbon monoxide induces cytoprotection in rat orthotopic lung transplantation via anti-inflammatory and anti-apoptotic effects. Am. J. Pathol. 163, 231-242.
Sugden, P. H. and Clerk, A. (1998). "Stress-responsive" mitogen-activated protein kinases (c-Jun N-terminal kinases and p38 mitogen-activated protein kinases) in the myocardium. Circ. Res. 83, 345-352.
Suliman, H. B., Carraway, M. S. and Piantadosi, C. A. (2003a). Postlipopolysaccharide oxidative damage of mitochondrial DNA. Am. J. Respir. Crit. Care Med. 167, 570-579.
Suliman, H. B., Carraway, M. S., Welty-Wolf, K. E., Whorton, A. R. and Piantadosi, C. A. (2003b). Lipopolysaccharide stimulates mitochondrial biogenesis via activation of nuclear respiratory factor-1. J. Biol. Chem. 278, 41510-41518.
Suliman, H. B., Welty-Wolf, K. E., Carraway, M., Tatro, L. and Piantadosi, C. A. (2004). Lipopolysaccharide induces oxidative cardiac mitochondrial damage and biogenesis. Cardiovasc. Res. 64, 279-288.
Taille, C., Almolki, A., Benhamed, M., Zedda, C., Megret, J., Berger, P., Leseche, G., Fadel, E., Yamaguchi, T., Marthan, R. et al. (2003). Heme oxygenase inhibits human airway smooth muscle proliferation via a bilirubin-dependent modulation of ERK1/2 phosphorylation. J. Biol. Chem. 278, 27160-27168.
Thom, S. R., Fisher, D., Xu, Y. A., Notarfrancesco, K. and Ischiropoulos, H. (2000). Adaptive responses and apoptosis in endothelial cells exposed to carbon monoxide. Proc. Natl. Acad. Sci. USA 97, 1305-1310.
Trumpower, B. L. (1990). The protonmotive Q cycle. Energy transduction by coupling of proton translocation to electron transfer by the cytochrome bc1 complex. J. Biol. Chem. 265, 11409-11412.
Verma, A., Hirsch, D. J., Glatt, C. E., Ronnett, G. V. and Snyder, S. H. (1993). Carbon monoxide: a putative neural messenger. Science 259, 381-384.
Virbasius, J. V. and Scarpulla, R. C. (1994). Activation of the human mitochondrial transcription factor A gene by nuclear respiratory factors: a potential regulatory link between nuclear and mitochondrial gene expression in organelle biogenesis. Proc. Natl. Acad. Sci. USA 91, 1309-1313.
Wagener, F. A., Volk, H. D., Willis, D., Abraham, N. G., Soares, M. P., Adema, G. J. and Figdor, C. G. (2003). Different faces of the heme-heme oxygenase system in inflammation. Pharmacol. Rev. 55, 551-571.
Wu, Z., Puigserver, P., Andersson, U., Zhang, C., Adelmant, G., Mootha, V., Troy, A., Cinti, S., Lowell, B., Scarpulla, R. C. et al. (1999). Mechanisms controlling mitochondrial biogenesis and respiration through the thermogenic coactivator PGC-1. Cell 98, 115-124.[CrossRef][Medline]
Young, L. J. and Caughey, W. S. (1986). Mitochondrial oxygenation of carbon monoxide. Biochem. J. 239, 225-227.[Medline]
Zhang, H. J., Zhao, W., Venkataraman, S., Robbins, M. E., Buettner, G. R., Kregel, K. C. and Oberley, L. W. (2002). Activation of matrix metalloproteinase-2 by overexpression of manganese superoxide dismutase in human breast cancer MCF-7 cells involves reactive oxygen species. J. Biol. Chem. 277, 20919-20926.
Zhang, J. and Piantadosi, C. A. (1992). Mitochondrial oxidative stress after carbon monoxide hypoxia in the rat brain. J. Clin. Invest. 90, 1193-1199.[Medline]
Zhang, X., Shan, P., Otterbein, L. E., Alam, J., Flavell, R. A., Davis, R. J., Choi, A. M. and Lee, P. J. (2003). Carbon monoxide inhibition of apoptosis during ischemia-reperfusion lung injury is dependent on the p38 mitogen-activated protein kinase pathway and involves caspase 3. J. Biol. Chem. 278, 1248-1258.
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