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Resuscitation from hemorrhagic shock induces profound changes in the physiologic processes of many tissues and activates inflammatory cascades that include the activation of stress transcriptional factors and upregulation of cytokine synthesis. This process is accompanied by acute organ damage (e.g., lungs and liver). We have previously demonstrated that the inducible nitric oxide synthase (iNOS) is expressed during hemorrhagic shock. We postulated that nitric oxide production from iNOS would participate in proinflammatory signaling. Using the iNOS inhibitor N6-(iminoethyl)-l-lysine or iNOS knockout mice we found that the activation of the transcriptional factors nuclear factor κB and signal transducer and activator of transcription 3 and increases in IL-6 and G-CSF messenger RNA levels in the lungs and livers measured 4 h after resuscitation from hemorrhagic shock were iNOS dependent. Furthermore, iNOS inhibition resulted in a marked reduction of lung and liver injury produced by hemorrhagic shock. Thus, induced nitric oxide is essential for the upregulation of the inflammatory response in resuscitated hemorrhagic shock and participates in end organ damage under these conditions.
Hemorrhagic shock initiates an inflammatory response characterized by the upregulation of cytokine expression (1) and accumulation of neutrophils (2) in a variety of tissues. These changes are prominent in the lungs and liver and are likely to contribute to end organ damage and resultant dysfunction after shock. The mechanisms by which hemorrhage triggers this inflammatory response remain poorly understood. Heightened adrenergic activity (3) and systemic release of proinflammatory agents from the gut (4, 5) have been hypothesized to contribute to acute lung injury after hemorrhage. In addition, reactive radicals are produced after ischemia/reperfusion and resuscitation from hemorrhagic shock, and have been implicated in a number of signal transduction pathways (6).
Among the important radicals produced during hemorrhagic shock is the bioregulatory molecule nitric oxide (NO)1 generated catalytically by three enzymes collectively termed NO synthases. We (7) and others (8) have shown that the inflammatory or inducible NO synthase (iNOS or NOS2) is upregulated in both the lungs and liver during shock. Therefore, this isoform may be capable of catalyzing the sustained production of NO after the tissue reperfusion associated with fluid resuscitation. NO can have both direct effects on cell signaling as well as indirect actions mediated by the reaction products formed when NO interacts with other molecules such as oxygen or superoxide (9). We hypothesized that enhanced NO production resulting from iNOS expression would contribute to proinflammatory signaling in hemorrhagic shock. Hemorrhagic shock experiments were therefore carried out in rats treated with the iNOS-selective inhibitor N6-(iminoethyl)-l-lysine (L-NIL; reference 10) and mice genetically deficient in iNOS. We report here that iNOS inhibition or deficiency prevents the upregulation of the inflammatory cytokines IL-6 and granulocyte colony-stimulating factor (G-CSF), as well as the activation of key proinflammatory transcriptional factors nuclear factor (NF)-κB and signal transducer and activator of transcription (Stat)3, and reduced organ damage after hemorrhage. These data indicate that under conditions of redox stress such as hemorrhagic shock, induced NO production plays an essential role in the initiation of the inflammatory response.
This study was approved by the University of Pittsburgh Institutional Review Board for animal experimentation and conforms to National Institutes of Health guidelines for the care and use of laboratory animals. Fasted male Sprague Dawley rats (270–290 g) were obtained from Charles River Breeding Laboratory (Cambridge, MA). iNOS-deficient mice were prepared as previously described (11). We have previously described in detail our rat model of resuscitated hemorrhagic shock (12). In brief, animals were anesthetized with methoxyfluorane, and then ventilated via endotracheal tubes using a 2.5-ml tidal volume of room air at 72 breaths/min. The right carotid artery was cannulated for continuous blood pressure monitoring, and the left jugular vein was cannulated for blood withdrawal and fluid administration. After an initial bleed of 2.25 ml/100 g body weight over 10 min, blood was withdrawn into a heparinized syringe or returned as needed to maintain a mean arterial blood pressure (MAP) of 40 mm Hg. At the point in time at which 35% of the shed blood had been returned (total shed blood volume 7.8 ± 0.5 ml), the animals were resuscitated to a MAP of 80 mm Hg by administration of the remaining shed blood plus two times the shed blood volume in lactated Ringers solution. Total shock time averaged 157 ± 2.3 min. Animals were killed 4 h after the initiation of resuscitation. Control animals underwent cannulation and anesthesia for an identical period of time as shock animals but were not bled. One group of animals (n = 6) received L-NIL (Alexis Corp., Laufelfingen, Switzerland) at 50 μg/kg/h, whereas the control group (both sham and shock animals) received saline infusion. L-NIL was dissolved in 1 ml of sterile saline fluid and was infused at the initiation of resuscitation for a period of 1 h.
The hemorrhagic shock protocol was modified as follows when performed on mice (11). The animals were anesthetized with methoxyfluorane. Both femoral arteries were surgically prepared and cannulated, one for continuous blood pressure monitoring, the contralateral artery for blood withdrawal or fluid administration. Animals were subjected to hemorrhagic shock by withdrawal of blood with a MAP maintained at 30 mm Hg for 3 h with continuous monitoring of blood pressure. Animals were resuscitated by infusion of the shed blood and intraperitoneal injection of 1 ml of saline. Animals were killed by exsanguination 4 h after resuscitation.
The release of the hepatocellular enzyme alanine aminotransferase (ALT) into plasma was used as an index of hepatic injury. Blood samples were collected into heparinized syringes at the end of observation period. The samples were centrifuged and the plasma was frozen at −70°C for subsequent analysis. ALT release was determined by an automated procedure using an autoanalyzer (RA 500; Technitron Inc., Tarrytown, NY).
After flushing the carcasses with cold (4°C) isotonic saline solution via the venous catheter, the lungs and livers were removed. Samples were immediately frozen in liquid nitrogen and stored at −80°C. Total cellular RNA was extracted from the samples using the method of Chomczyinski et al. (13). Cohort groups of rats (n = 5) were used for determination of lung wet to dry ratio and lung histology. After median sternotomy and preparation of the trachea, the left pulmonary hilus was isolated and ligated. The left lung was excised and removed for wet to dry ratio. The right lung was fixed by inflating with formaldehyde solution (4%) for histopathological examination. Tissue embedding and sectioning were performed using standard procedures. For histopathological examination, the lungs of animals were sectioned and stained with hematoxylin and eosin and for myeloperoxidase (MPO) as described (12). 10 randomly chosen fields of each lung specimen were examined at ×400 and blindly scored for number of intensely staining MPO-positive PMNs as described (12).
Total RNA (2.5 μg) was subjected to first-strand cDNA synthesis using oligo (dT) primer and Moloney murine leukemia virus (MMLV) reverse transcriptase (14). Primers were designed to amplify rat G-CSF, IL-6, and iNOS with the assistance of a PCR primer design program (PCR Plan; Intelligenetics, Mountain View, CA). The primers used to amplify rat G-CSF cDNA were as described (12). The sequence of the IL-6 5′ primer was ACAGCGATGATGCACTGTCAG, corresponding to nucleotide numbers 297–317 bp of the rat IL-6 cDNA sequence (15). The sequence of the IL-6 3′ primer was ATGGTCTTGGTCCTTAGCCAC, corresponding to nucleotide numbers 633–613 bp. The sequence of the iNOS 5′ primer was TTGGGTCTTGTTAGCCTAGTC, corresponding to nucleotide numbers 114–134 bp of the rat iNOS cDNA sequence (16). The sequence of the iNOS 3′ primer was TGTGCAGTCCCAGTGAGGAAC, corresponding to nucleotide numbers 375–355 bp. The primers amplified products of 560 bp for G-CSF (12), 339 bp for IL-6, and 264 bp for iNOS. The identity of the amplified cDNA fragment obtained from reverse transcriptase PCR (RT-PCR) reaction with IL-6, G-CSF, and iNOS primers was confirmed using restriction site analysis as described (12). PCR conditions were as follows: denaturation at 94°C for 1 min, annealing at 57°C for 1 min, and polymerization at 72°C for 2 min. PCR reactions were performed in a Perkin Elmer 480 thermocycler (480; Perkin-Elmer Corp., Norwalk, CT) using different numbers of cycles to detect a linear range of input RNA. The optimal cycle number was identified as 30 cycles. Rat peritoneal macrophages elicited with thyoglycolate and RAW cells (RAW 264.7 macrophage cell line) stimulated in vitro with LPS served as positive controls for G-CSF, IL-6, and iNOS messenger RNA (mRNA). The negative control for each set of PCR reactions contained water instead of DNA template. PCR product (20% of the reaction volume) of qualitative RT-PCR was electrophorectically separated on a 2% agarose gel and stained with ethidium bromide.
For semiquantitative RT-PCR (17) γ-32P–endlabeled 5′ primer was used. 15 μl of the PCR reaction was separated on a 10% polyacrylamide gel. After gel drying and exposure to a PhosphorImager screen (Molecular Dynamics, Sunnyvale, CA), the relative radioactivity of the bands was determined by volume integration using laser scanning densitometry. Each gel contained the same positive control, which permitted normalization of samples and comparison between gels.
Electrophoretic mobility shift assay (EMSA) was performed using whole-tissue extracts of lung or liver sections from the experimental groups as described (18). Binding reactions were performed using 20 μg of extracted protein and radiolabeled DNA-binding elements. The activation of NF-κB was determined using the duplex oligonucleotide based on the NF-κB binding site upstream of the murine iNOS promoter (19). Activation of Stat3 was assessed using the high-affinity serum-inducible element (hSIE) duplex oligonucleotide that preferentially binds Stat3 and Stat1 (20). EMSA was performed on a 4% polyacrylamide gel as described (21). The level of transcription factor activation was quantitated using PhosphorImager analysis of gel shift band intensities. Where indicated, EMSA-binding reactions were incubated with NF-κB protein (p)50 or p65 antibodies or antibodies specific for Stat3α or Stat3β. Antibodies specific for NF-κB p50, NF-κB p65, and Stat3α were obtained from Santa Cruz Biotechnology (Santa Cruz, CA) and were generated in goats against the amino acids 350–363 of human NF-κB p50, in goats against the amino acids 531–550 of human NF-κB p65, or in rabbits against the COOH-terminal 20 of 21 amino acid residues of murine Stat3, respectively. Stat3β-specific antibody was generated at Charles River Pharmaservices (Southbridge, MA) by immunizing chickens with the COOH-terminal 10 amino acid residues of human Stat3β conjugated to thyroglobulin. The IgY fraction was purified from egg yolk by the company.
Unless otherwise indicated, data are presented as mean ± SEM. Comparisons of means were performed using analysis of variance (ANOVA) followed by comparison of individual pairs of means using the Scheffe test. Both tests are contained within the StatView program (4.1; Abacus Concepts, Inc., Berkeley, CA).
Hemorrhagi c shock followed by resuscitation results in the upregulation of proinflammatory cascades in the lung as well as in other organs (1). The inflammatory response includes the expression of iNOS during the shock phase after hemorrhage (7, 8). In these experiments, we found that lung iNOS mRNA levels were increased by 8.7-fold over sham-treated animals (P = 0.001) 4 h after resuscitation from hemorrhagic shock (Fig. (Fig.1).1). To determine if induced NO participates in the upregulation of cytokine expression after hemorrhagic shock, rats were subjected to resuscitated hemorrhagic shock without or with treatment with the iNOS inhibitor L-NIL. IL-6 and G-CSF mRNA levels have been previously shown to be consistently elevated in the lungs after resuscitation from hemorrhagic shock (18) where they may contribute to leukocyte recruitment and activation (22). The predominant site for G-CSF mRNA production is the bronchoepithelial cells lining the luminal side of distal bronchioles (12). 4 h after resuscitation from hemorrhagic shock, IL-6 and G-CSF mRNA were increased 3.4- and 2.5-fold, respectively, compared to sham animals (P = 0.03 and P = 0.04, respectively; Fig. Fig.2).2). This upregulation was reduced 80 and 53%, respectively (P = 0.004 and P = 0.04, respectively) by administration of the iNOS inhibitor L-NIL. L-NIL alone had minimal effect on IL-6 or G-CSF mRNA levels in the sham animals (Fig. (Fig.2)2) and did not alter iNOS mRNA levels in the shocked animals (Fig. (Fig.1).1).
Activation of stress transcriptional factors such as NF-κB and STAT proteins contributes to the upregulation of cytokines such as IL-6 and G-CSF (23) and may also be a consequence of exposure of cells and tissues to these cytokines (24). Therefore, experiments were carried out to measure the activation of these transcriptional factors with and without iNOS inhibition. NF-κB activation was determined by EMSA using the duplex oligonucleotide based on a well-characterized NF-κB–binding sequence (19). Lungs of animals 4 h after resuscitation from shock demonstrated a 2.5-fold increase in NF-κB activation (P = 0.001) compared to sham controls (Fig. (Fig.33 A). After L-NIL treatment, levels of NF-κB activation decreased 70% in shocked animals (P = 0.003). To confirm the identity of the activated protein–DNA complex, binding assays were preincubated with a specific antibody against p50 or p65. The activated NF-κB complex was partially supershifted with p50 (Fig. (Fig.33 C), and reduced by 50% with antibody against p65 (data not shown) indicating that the complex was composed, in part, of both p50 and p65. Binding of the protein to labeled NF-κB–binding element was completely inhibited by 25-fold excess of NF-κB duplex oligonucleotide, but not by up to 100-fold excess of unlabeled hSIE duplex oligonucleotide (Fig. (Fig.33 D).
If iNOS-induced NF-κB activation contributes to the upregulation of cytokine expression (e.g., G-CSF), then NF-κB activity capable of binding the NF-κB–containing elements within the G-CSF promoter should be present and increased within the lungs of animals subjected to hemorrhagic shock. The promoter region of G-CSF contains a functional binding site for NF-κB (23) known as consensus decanucleotide 5′GRGRTTNCYY3′ (CK-1). EMSA using a labeled oligonucleotide based on the CK-1 sequence revealed a twofold increase of CK-1–binding activity (P = 0.03) over sham control animals in the lungs of animals subjected to hemorrhagic shock (Fig. (Fig.4,4, A and B). This binding activity was inhibited completely by 100-fold excess cold CK-1 duplex oligonucleotide and reduced substantially by 100-fold excess cold NF-κB duplex oligonucleotide. In contrast, binding activity was unaffected by 100-fold excess cold hSIE duplex oligonucleotide (Fig. (Fig.44 C).
We have previously shown that hemorrhagic shock results in activation of STAT proteins in the lungs of rats (25). G-CSF and IL-6 are among the cytokines known to activate Stat3 after binding to their specific receptors (24). Therefore, EMSA for Stat3 was performed to determine whether the reduced cytokine expression seen with iNOS inhibition was accompanied by a reduction in Stat3 activation. The activation of Stat3 was determined in EMSA using the hSIE, a DNA-binding element that preferentially binds Stat3 and Stat1. Stat3 and Stat1 proteins bind hSIE as dimers to form three distinct serum-inducible factor (SIF) complexes, SIF-A (Stat3 homodimer), SIF-B (Stat1 and Stat3 heterodimer), and SIF-C (26). SIF-A predominates in protein extracts of hemorrhagic shock tissues (Fig. (Fig.5).5). After resuscitation from hemorrhagic shock, Stat3 activation (SIF-A complex) increased 4.7-fold (P = 0.002) compared to sham controls; this increase was almost completely inhibited by L-NIL treatment. Although G-CSF and IL-6 both induce activation of Stat3, each activates a distinct isoform of Stat3; IL-6 activates Stat3α (27), whereas extracts of G-CSF–stimulated PMN contained only Stat3γ, a short isoform of Stat3 derived from proteolytic cleavage of Stat3α (28, and Tweardy, D.J., unpublished data). A third isoform of Stat3, known as Stat3β (p83), is derived from alternative RNA splicing (21). Animals subjected to hemorrhagic shock demonstrated activation of all three isoforms as determined by supershift assays using antibodies specific for Stat3α and Stat3β (Fig. (Fig.55 B). Incubation with the Stat3α- or Stat3β-specific antibody resulted in supershift of Stat3α and Stat3β, respectively; however, incubation with both antibodies did not completely supershift the SIF-A complex. The nonsupershifted portion demonstrated mobility similar to Stat3γ. DNA-affinity purification of whole- tissue extracts of hemorrhagic shock lungs followed by immunoblotting with Stat3-specific monoclonal antibody that recognizes all Stat3 isoforms confirmed the activation of all three Stat3 isoforms including Stat3γ (data not shown). After L-NIL treatment, a marked reduction in the activation of all three Stat3 isoforms was observed (Fig. (Fig.55 A). Reduction in the Stat3γ isoform was consistent with reduced PMN infiltration into the lung as seen in histological assessment (see below). These data provide indirect evidence for reduced cytokine action within the tissue that is subjected to downregulation of cytokine production by the inhibition of iNOS.
One consequence of the upregulation of inflammatory cascades after hemorrhagic shock is organ damage manifested by accumulation of PMNs and interstitial fluid. In this study we examined whether or not the reduction in cytokine production and proinflammatory signaling in L-NIL–treated rats was associated with a decrease in lung injury. Lung injury was assessed by histology as well as wet to dry ratio. After hemorrhagic shock, lung PMN infiltration increased by 4.7-fold (P = 0.001) at 4 h resuscitation, as determined by MPO staining (Fig. (Fig.6).6). L-NIL treatment resulted in a 44% decrease in PMN accumulation (P = 0.02). The wet to dry ratio increased by 24% in untreated shocked animals compared to sham animals (P = 0.01, Fig. Fig.66 C). This was accompanied by the histologic markers of tissue fluid leak, including widened interstitium due to interstitial edema (Fig. (Fig.66 A). The increase in lung wet to dry ratio comparing shock and sham animals was inhibited by L-NIL treatment by 33% (P = 0.03), which was accompanied by an obvious reduction in the histologic appearance of interstitial fluid accumulation (Fig. (Fig.66 A).
Hemorrhagic shock with resuscitation is commonly viewed as a whole body ischemia/reperfusion insult. Although the degree of ischemia may be variable in the pulmonary circulation, the splanchnic viscera experience a marked reduction in blood flow during circulatory shock and hypovolemia. To examine an organ subjected to severe ischemia/reperfusion during hemorrhagic shock and resuscitation as well as to establish whether similar proinflammatory effects of L-NIL treatment occurred outside of the lungs, we examined cytokine expression and transcriptional factor upregulation in the liver. Animals subjected to hemorrhagic shock and resuscitation demonstrated a 6.7-fold increase in IL-6 mRNA levels (P = 0.002), and a 3.3-fold increase in G-CSF mRNA levels (P = 0.003) compared to sham animals (Fig. (Fig.7).7). By contrast, L-NIL treatment reduced mRNA levels for IL-6 by 56% (P = 0.01) and for G-CSF by 51% (P = 0.02) when compared to untreated hemorrhaged animals. In shocked animals, the activation of NF-κB and the activation of Stat3 homodimer (SIF-A) were increased by 2.8- and 4.3-fold, respectively, in the liver compared to sham animals (P = 0.002 and P = 0.001, respectively; Fig. Fig.8).8). After L-NIL treatment, shocked animals demonstrated a marked reduction in the activation of both stress transcriptional factors. NF-κB activation was inhibited by 83% (P = 0.001) compared to the untreated shock group, whereas activated Stat3 was reduced by 58% (P = 0.001). In addition, we found that liver damage measured by plasma transaminase levels was significantly reduced in the NIL-treated rats subjected to hemorrhagic shock (J. Menezes, unpublished observations). Thus, the response of the liver after hemorrhagic shock was comparable to that observed in the lung and was mediated, in part, by induced NO.
Although L-NIL is a selective iNOS inhibitor, it may have some activity on other NO synthase isoforms (10) or may have other nonspecific effects. Therefore, to provide confirmation that the observed effects with L-NIL were due to the inhibition of the inducible form of NO synthase, we measured the activation of NF-κB and Stat3 in the lungs and the liver of iNOS-deficient and wild-type mice 4 h after hemorrhagic shock. Similar to the results seen in rats, hemorrhagic shock followed by resuscitation resulted in NF-κB and Stat3 activation in the lung (Fig. (Fig.9)9) and liver (Fig. (Fig.10)10) compared to sham-treated mice. In mice lacking the iNOS gene, the activation of NF-κB and Stat3 was reduced by 44% (P = 0.01) and 51% (P = 0.04), respectively, in the lung, and by 62% (P = 0.02) and 54% (P = 0.01), respectively, in the liver, when compared to wild-type animals. Similar to L-NIL treatment in rats, mice lacking the iNOS gene exhibited less liver damage when subjected to resuscitated shock than wild-type animals (Fig. (Fig.11).11).
This study was undertaken to determine to what degree induced NO contributes to the inflammatory response and subsequent end organ damage after resuscitation from hemorrhagic shock. We have extended previous studies (7, 8) by showing that iNOS is not only upregulated during shock, but that it remains elevated after resuscitation. Using either the iNOS inhibitor L-NIL or iNOS knockout mice, we demonstrate that iNOS contributes to the induced expression of the cytokines IL-6 and G-CSF in the lung and liver after hemorrhagic shock. The iNOS-dependent increase in IL-6 and G-CSF mRNA levels is associated with an iNOS-dependent increase in NF-κB and Stat3 activation in these tissues. An association between the upregulation of these proinflammatory events by NO and organ injury is shown by our experiments, demonstrating reduced PMN accumulation and edema formation in the lungs, and reduced plasma levels of liver enzymes with iNOS suppression. These data provide compelling evidence, not only that iNOS is in part responsible for lung and liver damage after hemorrhage and resuscitation, but that the induction of NO synthesis is a key event in the subsequent activation of inflammatory cascades after resuscitation.
During hemorrhagic shock, iNOS is upregulated in several sites including the lung and liver (8). The mechanism of upregulation is unclear, but could include hypoxia (6) or the action of cytokines. We have shown that iNOS expression increases in parallel with the duration of shock (7). Others have suggested that iNOS contributes to the initial vascular decompensation in hemorrhagic shock (8, 29) and we have suggested that the iNOS expression pattern is consistent with the possibility that iNOS may contribute to the progressive vascular dysfunction seen with sustained shock (7). The current data support the idea that NO can increase cytokine expression through the activation of NF-κB, and that the activation of Stat3 may be the result of local cytokine expression (24, 30). Indirect evidence for this possibility is provided by the demonstration that NF-κB binding specific for the CK-1 element in the G-CSF promoter is present in hemorrhagic shock tissues. Furthermore, activation of Stat3 isoforms characteristic of IL-6 and G-CSF stimulation were identified as part of the activated Stat3 complex. Full resuscitation of the animals requires 20 min. However, as early as 1 h after the initiation of resuscitation, we found that the levels of IL-6 and G-CSF mRNA, as well as NF-κB and Stat3 activation in lungs and livers, were elevated to levels similar to those observed at 4 h (data not shown). Thus, it is likely that the NO-mediated signaling events that are initiated in early phases of resuscitation result in the rapid activation of downstream cascades. Although NO produced by the constitutive NO synthase has well-documented signaling functions in many systems, our novel observations provide strong evidence that induced NO also participates in lung cell signaling events in inflammation. That iNOS regulation of inflammatory gene expression is perhaps a more generalized phenomenon is supported by a recent observation that the upregulation of interferon γ and the response to IL-12 after Leishmania major infection is iNOS dependent (31, and Bogdan, C., personal communication). Our results, however, do not exclude the possibility that the observed differences in both the L-NIL– treated rats and the iNOS knockout mice are due to some degree on changes in organ perfusion and oxygen delivery resulting from reduced NO availability.
NO is known to act as a signaling molecule in other circumstances either by activation of soluble guanylyl cyclase resulting in elevated cyclic guanosine 3′,5′ monophosphate (cGMP; reference 32) or through S-nitrosylation of proteins containing cysteine residues (33). Significant differences in cytokine mRNA levels (14, 18) and transcriptional factor activation (25) between the shock and sham groups was seen only after resuscitation, indicating that reperfusion was required. This suggests that redox-sensitive mechanisms were responsible for the NO-mediated signaling. Lander et al. (6, 34) have shown that NO activates p21ras through S-nitrosylation and that this occurs more efficiently in human T cells subjected to oxidative stress. Downstream events include p38 kinase activation (35) and NF-κB activation. In hemorrhagic shock, tissues are subjected to redox stress by hypoxia and oxygen radical production making S-nitrosylation of p21ras a reasonable candidate mechanism. A recent report demonstrates a role for increased phosphatidic acid in the signaling cascade involved in macrophage cytokine synthesis after hemorrhagic shock in mice (36). A relationship between phosphatidic acid and NO is not apparent at this time.
We have previously shown that nonspecific NO synthase inhibition increases organ injury in hemorrhagic shock (37), whereas here we show that the suppression of inflammation associated with selective iNOS inhibition results in a decrease in lung and liver injury. Taken together, the findings suggest that constitutive NOS is protective, but that the quantities of NO generated by iNOS cause injury. Our results suggest that organ damage in hemorrhagic shock is due, at least in part, to the proinflammatory action of NO. NO in combination with superoxide forms peroxynitrite, which could exert direct tissue toxicity. The results in hemorrhagic shock are contrasted by the observations in endotoxemia where the role of iNOS is less clear. iNOS knockout mice treated with high-dose endotoxin showed no difference in end organ damage when compared with their wild-type counterparts (11). More recently, we have shown that iNOS inhibition during endotoxemia increases apoptosis in the liver without necrosis (38). Difference between endotoxemia and hemorrhagic shock may be related to the higher levels of superoxide production and greater oxidant stress in the latter.
Approaches to remove NO in hemorrhagic shock could have therapeutic benefit. Patients suffering severe or sustained hemorrhagic shock after trauma or due to other causes of bleeding (e.g., ruptured aortic aneurysm) can develop organ injury and dysfunction. Our results indicate that selective inhibition of iNOS may be a reasonable approach. Alternatively, NO scavengers may also preserve adequate levels of NO needed to maintain perfusion while removing the excess NO which promotes inflammation and tissue injury.
Supported by National Institutes of Health grants GM-53789, GM-44100, GM-53921, and CA-72261, and by Deutsche Forschungsgemeinschaft (DFG) grant HI 614/1-1.
The present address of J. MacMicking is Laboratory of Immunology, HHMI, The Rockefeller University, 1230 York Ave., New York 10021.