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Infection and Immunity, November 2004, p. 6666-6675, Vol. 72, No. 11
0019-9567/04/$08.00+0     DOI: 10.1128/IAI.72.11.6666-6675.2004
Copyright © 2004, American Society for Microbiology. All Rights Reserved.

Both Inducible Nitric Oxide Synthase and NADPH Oxidase Contribute to the Control of Virulent Phase I Coxiella burnetii Infections

Robert E. Brennan, Kasi Russell, Guoquan Zhang, and James E. Samuel*

Department of Medical Microbiology and Immunology, Texas A&M University System Health Science Center, College Station, Texas

Received 29 February 2004/ Returned for modification 15 April 2004/ Accepted 14 July 2004


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ABSTRACT
 
Host control of Coxiella burnetii infections is believed to be mediated primarily by activated monocytes/macrophages. The activation of macrophages by cytokines leads to the production of reactive oxygen intermediates (ROI) and reactive nitrogen intermediates (RNI) that have potent antimicrobial activities. The contributions of ROI and RNI to the inhibition of C. burnetii replication were examined in vitro by the use of murine macrophage-like cell lines and primary mouse macrophages. A gamma interferon (IFN-{gamma}) treatment of infected cell lines and primary macrophages resulted in an increased production of nitric oxide (NO) and hydrogen peroxide (H2O2) and a significant inhibition of C. burnetii replication. The inhibition of replication was reversed in the murine cell line J774.16 upon the addition of either the inducible nitric oxide synthase (iNOS) inhibitor NG-monomethyl-L-arginine (NGMMLA) or the H2O2 scavenger catalase. IFN-{gamma}-treated primary macrophages from iNOS–/– and p47phox–/– mice significantly inhibited replication but were less efficient at controlling infection than IFN-{gamma}-treated wild-type macrophages. To investigate the contributions of ROI and RNI to resistance to infection, we performed in vivo studies, using C57BL/6 wild-type mice and knockout mice lacking iNOS or p47phox. Both iNOS–/– and p47phox–/– mice were attenuated in the ability to control C. burnetii infection compared to wild-type mice. Together, these results strongly support a role for both RNI and ROI in the host control of C. burnetii infection.


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INTRODUCTION
 
Coxiella burnetii, the etiologic agent of Q fever, is an obligate intracellular bacterium. Q fever is a zoonosis that is found worldwide, with a broad host range that includes wild and domestic mammals, birds, arthropods, and humans (9). For humans, the primary route of infection is through the inhalation of contaminated aerosols associated with domestic ruminants (40). Following inhalation, the organism is taken up primarily by resting alveolar macrophages, replicates to high numbers, and disseminates to a variety of tissues upon host cell rupture. Q fever can manifest as an acute illness that resembles influenza or as a chronic illness that is most often characterized by endocarditis. Clinically, acute Q fever is generally a self-limiting febrile illness that can be readily treated with tetracyclines to accelerate recovery (49). Conversely, chronic Q fever is refractory to antibiotics, with significant mortality rates even when patients receive the most effective treatment currently available, which is doxycycline plus chloroquine for at least 18 months (51).

C. burnetii has the unique ability among bacteria to replicate within an acidified vacuole of a resting host cell despite the presence of toxic host factors such as acid hydrolases and defensins (4). Although both infection with viable C. burnetii and vaccination with killed whole-cell C. burnetii lead to the development of humoral and cell-mediated immune responses, the host defense appears to be dependent on the enhanced microbicidal mechanisms of macrophages that are activated by specifically sensitized T cells (7, 33, 36). Previous studies have demonstrated that the activation of guinea pig monocytes, THP-1 monocytes, L929 murine fibroblasts, and primary mouse macrophages by gamma interferon (IFN-{gamma}) results in the inhibition of C. burnetii replication (20, 31, 32, 54, 57). However, only a few studies have been done to determine the mechanisms used by either professional or nonprofessional phagocytes to control C. burnetii replication. Dellecasagrande et al. reported that infected THP-1 monocytes stimulated with IFN-{gamma} were able to inhibit phase I C. burnetii replication and suggested that a tumor necrosis factor alpha-driven apoptotic mechanism may be involved (20). Recently, Howe et al. demonstrated that nitric oxide (NO) reversibly inhibits the replication of avirulent phase II C. burnetii in IFN-{gamma}-treated L929 murine fibroblasts (32). Zamboni and Rabinovitch reported that phase II C. burnetii induced NO in primary mouse macrophages and that this NO was partially responsible for reducing the numbers of C. burnetii organisms in these cells. They also demonstrated that IFN-{gamma}-treated primary macrophages from inducible nitric oxide synthase-negative (iNOS–/–) mice controlled phase II C. burnetii infections, which suggests that NO-independent mechanisms were also involved (57).

IFN-{gamma}-activated macrophages are capable of generating reactive oxygen intermediates (ROI) and reactive nitrogen intermediates (RNI) that enhance the ability of these cells to control the growth of intracellular organisms. IFN-{gamma} stimulation results in the activation of NADPH oxidase and iNOS. NADPH oxidase reduces oxygen to a superoxide anion (O2–), which can then enter the phagosome and be changed to hydrogen peroxide (H2O2) by a dismutase (17). iNOS synthesizes NO from L-arginine and oxygen. Reactive oxygen and nitrogen intermediates can inactivate [4Fe-4S] cluster-containing enzymes, damage DNA, and oxidize cellular membranes and enzymes (21, 27, 56). The antimicrobial activities of these intermediates have been demonstrated in vitro as well as in vivo. Mycobacterium tuberculosis, Leishmania donovani, and Rickettsia conorii have all been shown to be susceptible to H2O2 killing in vitro (22, 34, 43). Mice lacking gp91phox, which results in an NADPH oxidase deficiency, have an increased susceptibility to M. tuberculosis and L. donovani infections (2, 44). Mice lacking a functional iNOS were more susceptible to a challenge with virulent M. tuberculosis and died earlier after the challenge than did wild-type mice (38, 52). Also, the inhibition of iNOS resulted in a more rapid progression of chronic tuberculosis in wild-type mice (38). While prior studies have investigated the role of NO in controlling phase II C. burnetii infections in vitro, the goal of this study was to evaluate the roles that RNI and ROI play in the inhibition of virulent phase I C. burnetii infections in vitro and in vivo. To accomplish this goal, we conducted experiments in vitro, using J774 macrophage-like cell lines and primary macrophages from iNOS and p47phox knockout (KO) mice, and in vivo challenge experiments, using iNOS and p47phox KO mice.


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MATERIALS AND METHODS
 
Macrophage killing experiments. (i) Reagents. Murine recombinant IFN-{gamma}, hypoxanthine, and xanthine oxidase were purchased from Calbiochem (La Jolla, Calif.). Griess reagent, NG-monomethyl-L-arginine, catalase, horseradish peroxidase (HRPO), phenol red, and Hanks' balanced salt solution were purchased from Sigma (St. Louis, Mo.). Experiments with macrophages were conducted in a biosafety level III laboratory.

(ii) J774 mouse macrophage experiments. Two murine phagocytic cell lines—J774.16, a strong oxidative burst-competent cell line (18), and J774D.9, which fails to generate an oxidative burst after phorbol myristate acetate stimulation (24)—were assessed for the ability to control C. burnetii replication with and without activation by IFN-{gamma}. Hypoxanthine/xanthine oxidase (HX/XO) (an ROI donor) (12), catalase, and NG-monomethyl-L-arginine (NMMLA) (a nitric oxide synthase inhibitor) (30) were included to determine the effects of ROI and RNI on bacterial replication. Briefly, cells were plated at 105/ml in 24- or 96-well tissue culture plates and then allowed to adhere for 4 h. Macrophages were infected with purified C. burnetii (Nine Mile, phase I, RSA 493) at a multiplicity of infection of 35:1, incubated overnight at 37°C in 5% CO2, and then washed three times with warm medium to remove any uninternalized bacteria. Infected cells were then left untreated or were treated with IFN-{gamma} (100 U/ml) alone or in combination with 1 mM NMMLA, 100 µM catalase, or 250 µM/30 µM HX/XO on days 1, 2, 3, 4, and 5 postinoculation. The ability of C. burnetii to replicate in these cells was assessed at 2, 4, and 6 days postinfection. The generation of NO and H2O2 was detected spectrophotometrically by the use of Griess reagent (25) and by the horseradish peroxidase-dependent oxidation of phenol red (47), respectively, in 96-well plates. The replication of C. burnetii was monitored by real-time PCR as previously described (14), using cells harvested from 24-well plates. Cell viability was determined by trypan blue exclusion.

(iii) Primary macrophage experiments. Peritoneal macrophages were harvested from C57BL/6, p47phox–/– (C57BL/6), and iNOS–/– (C57BL/6) mice (Taconi Farms Inc., Germantown, N.Y.) to obtain macrophages that were competent in both respiratory burst and nitric oxide production and macrophages that lacked a functional respiratory burst or nitric oxide production. Resident peritoneal macrophages (PM{phi}) were collected by washing the peritoneal cavity of CO2-euthanized mice with 6 ml of cold RPMI containing 10% fetal bovine serum. The cells were plated in 24- and 96-well tissue culture plates at 2 x 105 cells/well in cold RPMI containing 10% fetal bovine serum, 1% L-glutamine, 5% L-cell medium, and 1% penicillin-streptomycin and were allowed to adhere for 24 h at 37°C in 5% CO2.

Primary macrophages were infected with purified C. burnetii (Nine Mile, phase I, RSA 493) at a multiplicity of infection of 35:1, incubated overnight at 37°C in 5% CO2, and then washed three times with warm medium to remove any uninternalized bacteria. Infected cells were then treated with IFN-{gamma} (100 U/ml) or were left untreated.

C. burnetii infection in mice. C57BL/6, p47phox–/– (C57BL/6), and iNOS–/– (C57BL/6) mice (Taconi Farms Inc.) were challenged intraperitoneally with 104 or 107 phase I C. burnetii cells suspended in phosphate-buffered saline. The mice were observed daily for morbidity and mortality for 28 days postchallenge. Body weights were measured on days 14 and 28 postchallenge. On days 14 and 28 postchallenge, the mice were euthanized by the use of CO2, and their spleens were collected and evaluated for splenomegaly. Spleen, lung, liver, and heart valve samples were also collected for histopathology and immunocytochemistry. Experiments were conducted in a biosafety level III laboratory.

Histopathology and immunocytochemistry. Lungs, livers, spleens, and heart valves were collected at 14 and 28 days postinfection, fixed for 48 h in 10% buffered formalin, and then stored in 70% ethanol until sectioning. Sectioned tissues were embedded in paraffin, cut to a 5-µm thickness, affixed to slides, and stained with hematoxylin and eosin. The distribution of C. burnetii cells was determined by immunocytochemistry, using a rabbit anti-C. burnetii Nine Mile phase I antiserum, goat anti-rabbit immunoglobulins, and an avidin-biotin complex (ABC; Vector Laboratories, Burlingame, Calif.).

Measurement of nitric oxide. Cell culture supernatants were collected, and the accumulation of NO2–, a stable end product of NO formation, was measured as an indicator of NO production. One hundred microliters of each supernatant plus 100 µl of Griess reagent was incubated at room temperature for 15 min, and then the absorbance was measured at 570 nm. The concentration of NO in the samples was calculated from a standard curve of sodium nitrite (25).

Measurement of hydrogen peroxide. Supernatants were removed from the wells of the plates, and the macrophages were covered with 100 µl of a phenol red-HRPO solution containing stimulants per well. One vertical row served as a blank and contained 100 µl of the phenol red-HRPO solution per well plus 10 µl of 1 N NaOH. The plates were incubated for 1 h at 37°C in 5% CO2. The reaction was interrupted by the addition of 10 µl of 1 N NaOH per well. After a 3-min interval, the absorbance was read at 630 nm. The concentration of H2O2 was calculated from a standard curve of H2O2 (47).

Estimation of bacterial doubling times. Doubling times for C. burnetii were calculated by using the formula G = t/[3.3 x log(b/B)], where G is the generation time, t is the time interval, in hours or minutes, b is the number of bacteria at the end of the interval (144-h time point), and B is the number of bacteria at the beginning of the time interval (96-h time point) (http://textbookofbacteriology.net/growth.html).

Statistics. Significant differences between means were determined by the Student t test by use of the Microsoft Excel statistics analysis pack. Differences were considered statistically significant when P values were <0.05 (indicated by asterisks in the figures). Significant differences between the replication rates were determined by performing a two-tailed Student t test on the average growth rates in each cell type calculated between the 96- and 144-h time points. Differences were considered statistically significant when P values were <0.05.


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RESULTS
 
C. burnetii replication rates. Bacterial loads were determined by real-time PCR on days 2, 4, and 6 postinfection in J774.16 and J774D.9 cells (Fig. 1A) and in PM{phi} (Fig. 1B). The estimated doubling times for bacteria were 45 h in J774.16 cells, 20 h in J774D.9 cells, 26 h in wild-type PM{phi}, 19 h in p47phox–/– PM{phi}, and 17 h in iNOS–/– PM{phi}. Although there does appear to be some differential uptake of C. burnetii by the various cell types, particularly as shown in Fig. 1B, the ability of a cell to take up bacteria is not directly related to the bacterial growth rate once the bacteria have been phagocytized. Therefore, calculating the doubling times of bacteria in cells demonstrating differential uptake rates is justified. The doubling times of C. burnetii were significantly shorter (P < 0.05) in cells that were defective for NADPH oxidase or iNOS. These results suggest that wild-type macrophages provide a more growth-restrictive environment than NADPH oxidase- or iNOS-defective macrophages and that the expression of oxygen and nitrogen radicals contributes to this growth suppression. Bacterial doubling times in all cell types were calculated for the interval from 96 to 144 h in an effort to estimate bacterial growth rates during the period of exponential growth.



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  		FIG. 1. Estimated generation times for C. burnetii in J774 cells and primary murine macrophages. Generation times were calculated by the formula G = t/[3.3 x log(b/B)], where G is the generation time, t is the time interval, in hours, b is the number of bacteria at the end of the time interval, and B is the number of bacteria at the beginning of the time interval. (A) Replication rates in J774.16 cells. J774.16, 45 h; J774D.9, 20 h. (B) Replication rates in peritoneal macrophages. Wild-type PM{phi}, 26 h; p47phox–/– PM{phi}, 19 h; iNOS–/– PM{phi}, 17 h. C. burnetii replication rates in cells lacking either iNOS or NADPH oxidase were significantly (P < 0.05) faster than replication rates in wild-type cells.

Effects of nitric oxide and H2O2 on C. burnetii replication in J774 cell lines. Nitric oxide production by J774 cell lines and primary macrophages was determined by measuring nitrite, a stable end product of nitric oxide production. The results show that C. burnetii infection alone was not sufficient to stimulate J774.16 or J774D.9 cells to produce significant levels of nitrite (Fig. 2A and B). IFN-{gamma} treatment of infected macrophages resulted in a significant (P < 0.01) increase in nitrite production in both macrophage cell lines at 96 and 144 h postinfection. The nitric oxide inhibitor NMMLA was able to suppress nitrite production by 90% in J774.16 cells and by 74% in J774D.9 cells. IFN-{gamma} treatment of infected macrophages also resulted in a significant (P < 0.05) production of H2O2 by J774.16 cells, but not J774D.9 cells (Fig. 2C and D). The H2O2 scavenger catalase reduced H2O2 levels by 85% in J774.16 cells. IFN-{gamma}-activated J774.16 cells significantly (P < 0.05) inhibited the replication of C. burnetii by 144 h postinfection (Fig. 3A). The replication rate was restored to nearly the level in untreated cells in the presence of the iNOS inhibitor NMMLA, suggesting that a nitric oxide-dependent mechanism is involved in controlling C. burnetii infections in macrophages. Bacterial replication was restored in J774.16 cells by the addition of catalase. Furthermore, IFN-{gamma}-activated J774D.9 macrophages, which lack a functional respiratory burst, were unable to significantly inhibit C. burnetii replication unless an exogenous source of H2O2 provided by HX/XO was added (Fig. 3B). Together, these results suggest that an oxygen-radical-dependent mechanism is also involved in controlling C. burnetii infections in macrophages.



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  		FIG. 2. Nitrite and hydrogen peroxide levels in J774.16 and J774D.9 cells. The cells were infected for 24 h with virulent phase I C. burnetii and then were treated with 100 U of murine rIFN-{gamma}/ml in thepresence or absence of the iNOS inhibitor NMMLA (1 mM) or the hydrogen peroxide scavenger catalase (100 µM). The stimulation of iNOS was indirectly determined by measuring nitrite, which is a stable end product of nitric oxide production. Hydrogen peroxide levels were determined by measuring the horseradish peroxidase-dependent oxidation of phenol red. (A) Nitrite levels in J774.16 cells. (B) Nitrite levels in J774D.9 cells. (C) Hydrogen peroxide levels in J774.16 cells. (D) Hydrogen peroxide levels in J774D.9 cells. (A and B) Stippled bars, no treatment; diagonally striped bars, treatment with 100 U of IFN-{gamma}/ml; vertically striped bars, treatment with 100 U of IFN-{gamma}/ml and 1 mM NMMLA. (C) Stippled bars, no treatment; diagonally striped bars, treatment with 100 U of IFN-{gamma}/ml; vertically striped bars, treatment with 100 U of IFN-{gamma}/ml and 100 µM catalase. (D) Stippled bars, no treatment; diagonally striped bars, treatment with 100 U of IFN-{gamma}/ml. The results are expressed as means and standard errors for three replicates from two independent experiments. Asterisks indicate significant differences between treated and untreated samples within the same time points.



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  		FIG. 3. Effects of IFN-{gamma} treatment on C. burnetii growth in J774.16 and J774D.9 cells. At 48, 96, and 144 h postinfection, infected cells were harvested, and the numbers of C. burnetii organisms, represented as numbers of Coxiella genomes, were determined by real-time PCR. (A) J774.16 cells were infected for 24 h with virulent phase I C. burnetii and then were treated with 100 U of murine rIFN-{gamma}/ml in the presence or absence of the iNOS inhibitor NMMLA (1 mM) or the hydrogen peroxide scavenger catalase (100 µM). (B) J774D.9 cells were infected for 24 h with virulent phase I C. burnetii and then were treated with 100 U of murine rIFN-{gamma}/ml in the presence or absence of the iNOS inhibitor NMMLA (1 mM) or the ROI donor HX/XO (250 µM/30 µM). The results are expressed as means and standard errors for three replicates from two independent experiments. Asterisks indicate significant differences between treated and untreated samples within the same time points.

The viabilities of untreated and treated J774.16 and J774 cells were similar and remained above 86% throughout the experiment, as determined by trypan blue exclusion, indicating that the inhibition of C. burnetii replication was not due to host cell death.

Effects of nitric oxide and H2O2 on C. burnetii replication in primary mouse macrophages. Since low levels of NO and H2O2 were still detectable in the presence of iNOS or NADPH oxidase inhibitors, we wanted to further define and clarify the contributions of NO and H2O2 to the inhibition of C. burnetii replication in vitro. To this end, we performed experiments using primary peritoneal macrophages from iNOS–/–, p47phox–/–, and wild-type C57BL/6 mice. The cells were infected for 24 h and then left untreated or treated with 100 U of IFN-{gamma}/ml for 5 days. On day 6 postinfection, the bacterial loads in the macrophages, as well as NO and H2O2 levels, were determined. As predicted, IFN-{gamma} treatment of the macrophages resulted in an increased production of NO in wild-type and p47phox–/– macrophages but not in iNOS–/– macrophages (Fig. 4A) and in an increased production of H2O2 in wild-type and iNOS–/– macrophages but not in p47phox–/– macrophages (Fig. 4B). IFN-{gamma}-treated wild-type, p47phox–/–, and iNOS–/– PM{phi} all significantly inhibited C. burnetii replication compared to untreated PM{phi} (Fig. 4C). However, when compared to wild-type PM{phi}, p47phox–/– and iNOS–/– PM{phi} were less effective at controlling replication, which supports a role for both NO and H2O2 in controlling C. burnetii infections (Fig. 4C). Peritoneal macrophages lacking NADPH oxidase were not as effective as iNOS–/– PM{phi} at controlling replication, suggesting that oxygen radicals play a larger role than NO in inhibiting C. burnetii growth in these cells.



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  		FIG. 4. Growth of virulent phase I C. burnetii in primary murine peritoneal macrophages. Macrophages were infected for 24 h with virulent phase I bacteria and then treated for 5 days with or without 100 U of IFN-{gamma}/ml. Nitrite and hydrogen peroxide levels were determined for primary murine peritoneal and bone marrow-derived macrophages. Levels of nitrite (A) and hydrogen peroxide (B) were measured at 144 h postinfection as described for the J774 cell lines. Stippled bars, no treatment; diagonally striped bars, treatment with 100 U of IFN-{gamma}/ml. (C) At 144 h postinfection, peritoneal macrophages were harvested, and the numbers of C. burnetii were determined by real-time PCR. Stippled bars, wild type; diagonally striped bars, p47phox–/–; vertically striped bars, iNOS–/–. The results are expressed as means and standard errors for three replicates. Asterisks indicate significant differences between treated and untreated samples.

Contributions of RNI and ROI in vivo. (i) Clinical signs and gross pathology in mice. To investigate whether oxygen or nitrogen radicals are required for resistance to C. burnetii infections in vivo, we infected wild-type, iNOS–/–, and p47phox–/– mice intraperitoneally with either 104 or 107 C. burnetii cells and evaluated them for morbidity, pathology, and bacterial distribution at 14 and 28 days postinfection (dpi). At 14 dpi, the p47phox–/– mice who were infected at the 107 dose, and to a lesser extent those who were infected at the 104 dose, failed to thrive and showed clinical signs of illness, including a hunched posture, a ruffled hair coat, and mild lethargy. No clinical signs were observed for wild-type and iNOS–/– mice who were infected with either dose of C. burnetii, except for distended abdomens due to splenomegaly. Pinpoint white foci were seen in the livers of three of four infected (107 dose) p47phox–/– and one of four infected (107 dose) iNOS–/– mice, suggesting a hematogenous dissemination of the organism. No foci were seen in the livers of the unchallenged controls or wild-type mice at either infectious dose. At 14 dpi, significant increases in spleen mass were observed for all mice who were challenged with 104 and 107 cells compared to unchallenged controls (Fig. 5A). At the 107 dose, spleens from iNOS–/– mice were significantly larger than those from wild-type mice, while p47phox–/– spleens were noticeably smaller. At 28 dpi, the p47phox–/– mice who were challenged with either 104 or 107 C. burnetii organisms had begun to resolve the clinical signs of disease, except for the distended abdomens. Infected wild-type and iNOS–/– mice remained clinically normal aside from having distended abdomens. Marked splenomegaly was still evident in all infected mice, with a higher degree of enlargement in mice infected with 107 cells (Fig. 5B). Spleens from p47phox–/– mice were significantly larger than those from wild-type or iNOS–/– mice at both infectious doses. Spleens from wild-type and iNOS–/– mice were significantly smaller at 28 dpi than at 14 dpi for mice infected with the 104 dose.



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  		FIG. 5. Splenomegaly in C57BL/6, iNOS–/–, and p47phox–/– mice. Mice were challenged intraperitoneally with 104 or 107 C. burnetii cells. At 14 (A) and 28 (B) dpi, spleens were collected and evaluated for splenomegaly. Stippled bars, wild type; diagonally striped bars, iNOS–/–; vertically striped bars, p47phox–/–. The results are expressed as means and standard errors for four mice. Asterisks indicate significant differences between wild-type and knockout mice.

(ii) Histopathology. At 14 dpi, the lungs of all mice displayed various degrees of perivascular histiocytic (granulomatous) interstitial pneumonia, with a decrease in the overall airspace. Bronchiolar involvement was occasionally seen, with increased peribronchiolar mononuclear cells and some desquamation of bronchiolar epithelial cells. The severity of the lung changes was greater for mice infected with 107 organisms than for mice infected with 104 organisms and was greatest for p47phox–/– mice (Table 1). p47phox–/– mice, even those infected at the lower dose, exhibited moderate to severe perivascular histiocytic hepatitis. Lesser changes were noted for iNOS–/– and wild-type mice (Table 1). Marked extramedullary hematopoiesis with myeloid, erythroid, and megakaryocytic hyperplasia, a normal finding in mice, was noted in the livers and spleens of all infected mice compared to uninfected controls. All infected mice had histiocytic splenitis, and again, the p47phox–/– mice displayed the largest degree of change, including rare necrotic foci in the mice infected with the 107 dose. The spleens of wild-type mice, and to a slightly lesser extent those of iNOS–/– mice, had diffuse lymphoid hyperplasia. Mild myocarditis and valvular endocarditis were noted for all infected mice. No pathological lesions were noted for control animals.


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  		TABLE 1. Severity of histopathologic changes in selected tissues of mice infected with C. burnetii

At 28 dpi, the interstitial pneumonia was resolving in all infected mice, and only a mild decrease in the airspace remained. However, moderate perivascular histiocytic pneumonia was still present in the p47phox–/– mice (Table 1). The livers continued to have granulomatous lesions, with minimal focal necrosis now present in infected animals (107 dose). Splenic plasmacytosis was noted for infected wild-type mice, indicating a resolution of the histiocytic splenitis noted at 14 dpi. The spleens of iNOS–/– mice contained more histiocytes and fewer plasma cells than those of wild-type mice. p47phox–/– mice continued to have severe perivascular histiocytic splenitis with marked extramedullary hematopoiesis, minimal focal necrosis, and a lack of follicle organization. Mild myocarditis and valvular endocarditis were noted for all infected mice. Venous microthrombi were present in multiple organs, including lungs, livers, and spleens.

(iii) Immunocytochemistry. C. burnetii cells were immunolocalized in lung, liver, spleen, and heart valve samples from wild-type, iNOS–/–, and p47phox–/– mice at 14 and 28 days postinfection. At 14 days postinfection, bacteria were detected in all of the tissues from the iNOS–/– and p47phox–/– mice at both challenge doses (Table 2). In general, more organisms were detected in a larger number of tissues in mice receiving the higher challenge dose. No bacteria were detected in the lungs of wild-type mice at either challenge dose. iNOS–/– and p47phox–/– mice were more heavily colonized with C. burnetii than wild-type mice, and the bacteria were more widely disseminated in the tissues.


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  		TABLE 2. Immunolocalization of C. burnetii in mice

In general, at 28 dpi the bacterial burdens had decreased in all infected animals at both challenge doses compared to those at 14 dpi, with the exception of the heart valves of iNOS–/– and p47phox–/– mice. The heart valves from iNOS–/– and p47phox–/– mice at both challenge doses contained larger and more numerous foci of infection at 28 dpi than at 14 dpi (Table 2). The distribution of bacteria continued to be more widespread in iNOS–/– and p47phox–/– mice than in wild-type mice in all tissues in which C. burnetii was still detected. Figure 6 illustrates the degree of bacterial deposition in the heart valves of mice who were challenged with 107 C. burnetii cells at 28 days postinfection.



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  		FIG. 6. Immunolocalization of C. burnetii in cardiac valve sections from mice challenged with 107 C. burnetii organisms at 28 days postinfection. C. burnetii was detected by the ABC method (Vector Laboratories). (A) Valve section from wild-type mouse; (B) valve section from iNOS–/– mouse; (C) valve section from p47phox–/– mouse. The red to rust-colored deposits represent the presence of C. burnetii (arrows denote examples). At, atrial side; V, ventricular side. Magnification, x40.


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DISCUSSION
 
C. burnetii is an obligate intracellular pathogen that survives by multiplying in acidified vacuoles of monocytes/macrophages and whose virulence depends on the expression of lipopolysaccharide (LPS). Virulent, phase I bacteria express a complete, or smooth-type, LPS and can be recovered from infected animals, whereas avirulent, phase II bacteria express a truncated, or rough-type, LPS and cannot be recovered from infected animals (29). However, phase I and phase II bacteria are able to replicate in numerous cell types in vitro (4, 13, 20, 31, 32, 54, 57), and several studies have demonstrated the ability of cytokine-activated cells to inhibit phase I and phase II C. burnetii replication (20, 32, 54, 57). Recent reports have demonstrated roles for NO in phase II inhibition in L929 murine fibroblasts (32, 57) and a possible role for apoptosis in the elimination of phase I bacteria from human monocytes (20). However, the potential contributions of ROI in controlling C. burnetii infections have not been fully investigated. Zamboni et al. reported that the addition of catalase or superoxide dismutase to phase II-infected bone marrow-derived macrophages had no effect on the relative bacterial loads in untreated or IFN-{gamma}-treated bone marrow-derived macrophages. This report alluded to a finding that C. burnetii expresses superoxide dismutase and catalase activities (3) and suggested that these enzyme systems can fully protect C. burnetii from ROI (57). However, other pathogens such as Salmonella enterica serovar Typhimurium and Brucella abortus, which also express superoxide dismutase and catalase enzymes, are susceptible to ROI killing (35, 55), indicating that possessing and expressing ROI defense mechanisms does not necessarily equate protection from the high level of ROI induced by IFN-{gamma} activation. Dellecasagrande et al. have shown that THP-1 monocytes, monocytes from healthy humans, and monocytes from patients suffering from chronic granulomatous disease controlled phase I C. burnetii infections despite undetectable levels of RNI or ROI (20). The differences in the capacities of monocytes and macrophages to generate ROI and RNI have been well documented (1, 16); thus, the apoptotic mechanism of controlling C. burnetii replication may be a unique but effective alternative for cells such as monocytes that lack the traditional microbicidal capacities of macrophages. Howe et al. proposed that since the phagocytosis of C. burnetii does not stimulate a respiratory burst, as defined by the detection of O2– (5), C. burnetii would not be exposed to toxic peroxynitrite (ONOO–), which is formed through the interaction of superoxide with nitric oxide. However, our results demonstrate that the respiratory burst is activated upon the stimulation of infected macrophages with IFN-{gamma}, as defined by the detection of H2O2. We also detected superoxide (O2–) produced by IFN-{gamma} activation (data not shown). Recently, Korshunov et al. demonstrated that under acidic conditions, protonated superoxide penetrated lipid membranes at rates similar to water and reported that when Escherichia coli CuZnSOD mutants were exposed to superoxide at a low pH, cytosolic fumerase B was damaged (37). Protonated superoxide can also react with itself to form H2O2 (42). Therefore, due to the acidic nature of the vacuole in which C. burnetii resides, we propose that C. burnetii is exposed to a variety of toxic radicals, including O2–, NO, H2O2, and ONOO–. In this report, we demonstrated that both RNI and ROI contribute to controlling phase I C. burnetii infections in vivo as well as in vitro.

The doubling times for C. burnetii were determined in cloned and primary macrophages. Bacterial loads were determined at 48, 96, and 144 h postinfection. Twenty-four-hour time points were not taken because the overall goal of the project was to investigate the effects of iNOS and NADPH oxidase on bacterial replication. Thus, the 48-h time point represents the first time point (24 h after treatments) for which comparisons could be made regarding the effects of iNOS and NADPH oxidase on C. burnetii growth in untreated and treated cells. The doubling times were calculated for untreated samples. Doubling times were determined by using the 96- and 144-h time points as time zero and the end time, respectively, in an effort to calculate doubling times only during the period of exponential growth. The use of these time points also diminished any effects of initial bacterial uptake on the calculated growth rates. The replication rates of C. burnetii were approximately two times faster in NADPH oxidase- or iNOS-defective macrophages, suggesting that RNI and ROI may be partially responsible for the slower growth rates in immunocompetent cells. These findings are similar to those of a previous report that demonstrated that phase II bacterial loads were larger in unstimulated primary macrophages treated with iNOS-inhibiting agents than in unstimulated, untreated primary macrophages (57). One possibility for the extended doubling times observed in NADPH oxidase and iNOS competent cells is that C. burnetii may devote more energy to up-regulating genes that are necessary to detoxify low levels of reactive nitrogen and oxygen intermediates that may be present in resting macrophages. For example, stationary-phase infectious Legionella pneumophila has been demonstrated to express several virulence traits, including catalase and superoxide dismutase, that are thought to be important for L. pneumophila to establish an infection (10, 11, 53).

To determine the effects of iNOS and NADPH oxidase on phase I C. burnetii infections in vitro, we monitored bacterial replication in IFN-{gamma}-activated J774 cell lines that differed in the ability to produce ROI. IFN-{gamma}-activated J774.16 macrophages significantly inhibited bacterial replication, and this inhibition was reversed by the addition of either the iNOS inhibitor NMMLA or the H2O2 scavenger catalase, suggesting that RNI and ROI both contribute to controlling C. burnetii infections. Interestingly, the inhibition of iNOS did not fully rescue the growth defect of C. burnetii in IFN-{gamma}-treated macrophages, whereas the inhibition of H2O2 did appear to fully rescue and possibly promote bacterial replication, suggesting that ROI, and H2O2 in particular, may play a larger role than RNI in controlling infections in these cells. Similar effects were seen by Feng and Walker in cytokine-treated Rickettsia conorii-infected human umbilical vein endothelial cells (22). The addition of NMMLA to cytokine- and chemokine-treated infected human umbilical vein endothelial cells resulted in an approximately 85% recovery of bacterial growth, while the addition of catalase led to an approximately 160% recovery. This apparent augmentation of replication may be a result of relieving the stress of endogenous ROI as well as exogenous ROI. IFN-{gamma}-activated J774D.9 macrophages, which lack a functional NADPH oxidase, only significantly inhibited bacterial replication when an exogenous source of H2O2 was added, which also indicates the importance of ROI in controlling infections. The finding that the inhibition of either iNOS or NADPH oxidase resulted in a rescue of growth suggests that the control of C. burnetii is in part due to the synergistic effects of RNI and ROI.

In an effort to substantiate the in vitro findings from the cloned cell lines, we employed primary macrophages that differed in the ability to produce ROI and RNI, which allowed us to avoid the use of inhibitors or donors that may have had incomplete or nonspecific effects. Although IFN-{gamma}-activated iNOS–/– and p47phox–/– macrophages did not produce significant amounts of NO or H2O2, respectively, they did inhibit bacterial replication significantly more than untreated controls. These data suggest that in addition to RNI- and ROI-dependent mechanisms, the activation of macrophages results in bacteriostatic mechanisms that are independent of iNOS and NADPH oxidase. Several investigators have demonstrated that IFN-{gamma} activation results in iron limitation and tryptophan starvation, which serve to inhibit the growth of other intracellular pathogens (23, 26, 39, 46). Interestingly, activated iNOS–/– peritoneal macrophages were only slightly less effective while activated p47phox–/– peritoneal macrophages were significantly less effective at controlling infections than activated wild-type peritoneal macrophages, suggesting that ROI may play a more significant role in controlling C. burnetii infections than RNI in these cells.

This hypothesis was further supported by the finding that mice lacking iNOS were less effective at controlling C. burnetii infections than wild-type mice and that NADPH oxidase-deficient mice were even less effective than iNOS–/– mice. Although a dose-dependent splenomegaly was apparent in all infected mice, the phenotypes of the iNOS–/– and p47phox–/– mice were markedly different from that of wild-type mice. The iNOS–/– mice appeared to have an initial period of increased susceptibility followed by a period of recovery, as indicated by the presence of liver foci and significant splenomegaly at 14 dpi and by no liver foci and splenomegaly similar to that of wild-type mice at 28 dpi. The p47phox–/– mice appeared to have a more severe phenotype than the iNOS–/– mice. At 14 dpi, more of these mice possessed liver foci and developed clinical signs of illness, and by 28 dpi these mice demonstrated significantly more splenomegaly than wild-type mice. These data support the general hypothesis that ROI play a more significant role in protection than RNI in the infection of mice.

The findings that both iNOS–/– and p47phox–/– mice were more susceptible to infection than wild-type mice and that either iNOS or H2O2 inhibitors were able to rescue growth defects in vitro indicate that RNI and ROI both contribute, possibly in a synergistic fashion, to controlling C. burnetii infections. Synergy between RNI and ROI can occur through various interactions. For example, the interaction of NO with O2– results in the formation of toxic peroxynitrite (ONOO–), which has the ability to directly oxidize DNA bases and sulfhydryl groups and to cause lipid peroxidation (41). Nitric oxide has also been demonstrated to inactivate Fe-S-containing enzymes such as aconitase, resulting in the release of Fe2+, which can then interact with H2O2 as part of the Haber-Weiss reaction to form toxic hydroxyl radicals that are also capable of oxidizing proteins, DNA, and lipids (28, 41). The synergistic effects of RNI and ROI on the inhibition of pathogens have been previously demonstrated. Pacelli et al. reported that hydrogen peroxide-dependent killing of E. coli increased 1,000-fold in the presence of nitric oxide and could be prevented by the chelation of iron (45). Another study, by Darrah et al., demonstrated that mice lacking iNOS or gp91phox were more susceptible to lethal challenges of Rhodococcus equi than wild-type mice and also demonstrated in vitro that efficient killing of R. equi cells was observed in the presence of peroxynitrite but not in the presence of nitric oxide or superoxide alone (19). The passage of protonated superoxide into the C. burnetii-containing vacuole could potentiate the formation of ONOO–. It was previously demonstrated that NO contributed to the inhibition of C. burnetii replication in cytokine-stimulated L929 cells by preventing the formation of large replicative vacuoles (32). Further investigation is required to determine if ROI are also involved in this mechanism. Finally, the finding that an iNOS- and NADPH oxidase-independent mechanism(s) may also be involved in controlling C. burnetii infections illustrates the probable complexity and possible redundancy of the innate immune response to bacterial infections.

The dissemination and lack of clearance of C. burnetii in the heart valves of iNOS–/– and p47phox–/– mice suggest that RNI and ROI may play critical roles in the prevention of C. burnetii-associated endocarditis, which is the major clinical presentation of chronic Q fever. The development of chronic Q fever has often been associated with immunodeficiency (15, 48, 50) and has only been demonstrated in lab animals that were either immunosuppressed or had previously damaged heart valves. Atzpodien et al. reported the dissemination of C. burnetii by 10 days postinfection in cardiac valves of mice treated with cyclophosphamide, and more recently, Andoh et al. demonstrated that SCID mice infected with C. burnetii developed endocarditis resembling the pathology seen in human Q fever endocarditis (6, 8). Those studies involved widespread and nonspecific immunosuppression affecting several potential immune system mechanisms at various levels. In this study, we have demonstrated that the specific lack of a functional iNOS or NADPH oxidase contributes to the colonization and persistence of C. burnetii in cardiac valves. It is possible that the C. burnetii-associated endocarditis documented in previous studies may have been in part due to the lack of adequately activated macrophages and to a poor stimulation of iNOS and NADPH oxidase. Further characterization of these and other mouse strains is required to adequately evaluate their usefulness as models of Q fever endocarditis.


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ACKNOWLEDGMENTS
 
This work was supported by Public Health Service grants AI37744 and AI448191 from the National Institute of Allergy and Infectious Diseases.

We thank Vernon Tesh and Renée Tsolis for their critical reviews of the manuscript.


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FOOTNOTES
 
* Corresponding author. Mailing address: Department of Medical Microbiology and Immunology, Texas A&M University System Health Science Center, College Station, TX 77843-1114. Phone: (979) 862-1684. Fax: (979) 845-3479. E-mail: jsamuel{at}tamu.edu. Back

Editor: F. C. Fang


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REFERENCES
 
    1
  1. Adams, D. O., and T. A. Hamilton. 1984. The cell biology of macrophage activation. Annu. Rev. Immunol. 2:283-318.[CrossRef][Medline]
    2. 2
  2. Adams, L. B., M. C. Dinauer, D. E. Morgenstern, and J. L. Krahenbuhl. 1997. Comparison of the roles of oxygen and nitrogen intermediates in the host response to mycobacterium tuberculosis using transgenic mice. Tuber. Lung Dis. 78:237-246.[CrossRef][Medline]
    3. 3
  3. Akporiaye, E. T., and O. G. Baca. 1983. Superoxide anion production and superoxide dismutase and catalase activities in Coxiella burnetii. J. Bacteriol. 154:520-523.[Abstract/Free Full Text]
    4. 4
  4. Akporiaye, E. T., J. D. Rowatt, A. A. Aragon, and O. G. Baca. 1983. Lysosomal response of a murine macrophage-like cell line persistently infected with Coxiella burnetii. Infect. Immun. 40:1155-1162.[Abstract/Free Full Text]
    5. 5
  5. Akporiaye, E. T., D. Stefanovich, V. Tsosie, and G. Baca. 1990. Coxiella burnetii fails to stimulate human neutrophil superoxide anion production. Acta Virologica 34:64-70.[Medline]
    6. 6
  6. Andoh, M., T. Naganawa, A. Hotta, T. Yamaguchi, H. Fukushi, T. Masegi, and K. Hirai. 2003. SCID mouse model for lethal Q fever. Infect. Immun. 71:4717-4723.[Abstract/Free Full Text]
    7. 7
  7. Asher, M. S., P. B. Jahrling, D. G. Harrington, R. A. Kishimoto, and V. G. McGann. 1980. Mechanisms of protective immunogenicity of microbial vaccines: effects of cyclophosphamide pretreatment in Venezuelan encephalitis, Q fever, and tularemia. Clin. Exp. Immunol. 41:225-236.[Medline]
    8. 8
  8. Atzpodien, E., W. Baumgartner, A. Artelt, and D. Thiele. 1994. Valvular endocarditis occurs as a part of a disseminated Coxiella burnetii infection in immunocompromised Balb/cj (H-2d) mice infected with the Nine Mile isolate of C. burnetii. J. Infect. Dis. 170:223-226.[Medline]
    9. 9
  9. Babudieri, C. 1959. Q fever: a zoonosis. Adv. Vet. Sci. 5:81-84.
    10. 10
  10. Bandyopadhyay, P., B. Byrne, Y. Chan, M. S. Swanson, and H. M. Steinman. 2003. Legionella pneumophila catalase-peroxidases are required for proper trafficking and growth in primary macrophages. Infect. Immun. 71:4526-4535.[Abstract/Free Full Text]
    11. 11
  11. Bandyopadhyay, P., and H. M. Steinman. 2000. Catalase-peroxidases of Legionella pneumophila: cloning of the katA gene and studies of KatA function. J. Bacteriol. 182:6679-6686.[Abstract/Free Full Text]
    12. 12
  12. Beauchamp, C., and I. Fridovich. 1970. A mechanism for the production of ethylene from methional. The generation of the hydroxyl radical by xanthine oxidase. J. Biol. Chem. 245:4641-4646.[Abstract/Free Full Text]
    13. 13
  13. Beron, W., M. G. Gutierrez, M. Rabinovitch, and M. I. Colombo. 2002. Coxiella burnetii localizes in a Rab7-labeled compartment with autophagic characteristics. Infect. Immun. 70:5816-5821.[Abstract/Free Full Text]
    14. 14
  14. Brennan, R. E., and J. E. Samuel. 2003. Evaluation of Coxiella burnetii antibiotic susceptibilities by real-time PCR assay. J. Clin. Microbiol. 41:1869-1874.[Abstract/Free Full Text]
    15. 15
  15. Capo, C., Y. Zaffran, F. Zugan, P. Houpikian, D. Raoult, and J. L. Mege. 1996. Production of interleukin-10 and transforming growth factor ß by peripheral blood mononuclear cells in Q fever endocarditis. Infect. Immun. 64:4143-4150.[Abstract]
    16. 16
  16. Cohn, Z. A. 1978. The activation of mononuclear phagocytes: fact, fancy, future. J. Immunol. 121:813-816.[Abstract/Free Full Text]
    17. 17
  17. Clark, R. A. 1990. The human neutrophil respiratory burst oxidase. J. Infect. Dis. 161:1140-1147.[Medline]
    18. 18
  18. Damiani, G., C. Kiyotaki, W. Soeller, M. Sasada, J. Peisach, and B. R. Bloom. 1980. Macrophage variants in oxygen metabolism. J. Exp. Med. 152:808-822.[Abstract/Free Full Text]
    19. 19
  19. Darrah, P. A., M. K. Hondalus, Q. Chen, H. Ischiropoulos, and D. M. Mosser. 2000. Cooperation between reactive oxygen and nitrogen intermediates in killing of Rhodococcus equi by activated macrophages. Infect. Immun. 68:3587-3593.[Abstract/Free Full Text]
    20. 20
  20. Dellacasagrande, J., C. Capo, D. Raoult, and J.-L. Mege. 1999. IFN-{gamma}-mediated control of Coxiella burnetii survival in monocytes: the role of cell apoptosis and TNF. J. Immunol. 176:2259-2265.
    21. 21
  21. Fang, F. C. 1997. Mechanisms of nitric oxide related antimicrobial activity. J. Clin. Investig. 99:2818-2825.[Medline]
    22. 22
  22. Feng, H. M., and D. H. Walker. 2000. Mechanisms of intracellular killing of Rickettsia conorii in infected human endothelial cells, hepatocytes, and macrophages. Infect. Immun. 68:6729-6736.[Abstract/Free Full Text]
    23. 23
  23. Gebran, S. J., Y. Yamamoto, C. Newton, T. W. Klein, and H. Friedman. 1994. Inhibition of Legionella pneumophila growth by gamma interferon in permissive A/J mouse macrophages: role of reactive oxygen species, nitric oxide, tryptophan, and iron (III). Infect. Immun. 62:3197-3205.[Abstract/Free Full Text]
    24. 24
  24. Goldberg, M., L. S. Belkowski, and B. R. Bloom. 1990. Regulation of macrophage function by interferon-gamma. Somatic cell genetic approaches in murine macrophage cell lines to mechanisms of growth inhibition, the oxidative burst, and expression of the chronic granulomatous disease gene. J. Clin. Investig. 85:563-569.
    25. 25
  25. Granger, D. L., J. B. Hibbs, and L. M. Broadnax. 1991. Urinary nitrate excretion in relation to murine macrophage activation: influence of dietary L-arginine and oral NG-monomethyl-L-arginine. J. Immunol. 146:1294-1302.[Abstract]
    26. 26
  26. Gupta, S. L., J. M. Carlin, P. Pyati, W. Dai, E. R. Pfefferkorn, and M. J. Murphy, Jr. 1994. Antiparasitic and antiproliferative effects of indoleamine 2,3-dioxygenase enzyme expression in human fibroblasts. Infect. Immun. 62:2277-2284.[Abstract/Free Full Text]
    27. 27
  27. Haas, A., and W. Goebel. 1992. Microbial strategies to prevent oxygen-dependent killing by phagocytes. Free Radic. Res. Commun. 16:137-157.[Medline]
    28. 28
  28. Haber, F., and J. Weiss. 1934. The catalytic decomposition of hydrogen peroxide by iron salts. Proc. R. Soc. Lond. A 147:332-351.[Free Full Text]
    29. 29
  29. Hackstadt, T., M. G. Peacock, P. J. Hitchcock, and R. L. Cole. 1985. Lipopolysaccharide variation in Coxiella burnetii: interstrain heterogeneity in structure and antigenicity. Infect. Immun. 48:359-365.[Abstract/Free Full Text]
    30. 30
  30. Hibbs, J. B., Jr., Z. Vavrin, and R. R. Taintor. 1987. L-Arginine is required for expression of the activated macrophage effector mechanism causing selective metabolic inhibition in target cells. J. Immunol. 138:550-565.[Abstract]
    31. 31
  31. Hinrichs, D. J., and T. R. Jerrells. 1976. In vitro evaluation of immunity to Coxiella burnetii. J. Immunol. 117:996-1003.[Abstract/Free Full Text]
    32. 32
  32. Howe, D., L. F. Barrows, N. M. Lindstrom, and R. A. Heinzen. 2002. Nitric oxide inhibits Coxiella burnetii replication and parasitophorous vacuole maturation. Infect. Immun. 70:5140-5147.[Abstract/Free Full Text]
    33. 33
  33. Izzo, A. A., and B. A. Marmion. 1993. Variation in interferon-{gamma} responses to Coxiella burnetii antigens with lymphocytes from vaccinated and naturally infected subjects. Clin. Exp. Immunol. 94:507-514.[Medline]
    34. 34
  34. Jackett, P. S., V. R. Aber, and D. B. Lowrie. 1978. Virulence and resistance to superoxide, low pH, and hydrogen peroxide among strains of Mycobacterium tuberculosis. J. Gen. Microbiol. 104:37-45.[Abstract/Free Full Text]
    35. 35
  35. Jiang, X., B. Leonard, R. Bensen, and C. L. Baldwin. 1993. Macrophage control of Brucella abortus: role of reactive oxygen intermediates and nitric oxide. Cell. Immunol. 151:309-319.[CrossRef][Medline]
    36. 36
  36. Kishimoto, R. A., H. Rozmiarek, and R. W. Larson. 1978. Experimental Q fever infection in congenitally athymic nude mice. Infect. Immun. 22:69-71.[Abstract/Free Full Text]
    37. 37
  37. Korshunov, S. S., and J. A. Imlay. 2002. A potential role for periplasmic superoxide dismutase in blocking the penetration of external superoxide into the cytosol of gram-negative bacteria. Mol. Microbiol. 43:95-106.[CrossRef][Medline]
    38. 38
  38. MacMicking, J. D., R. J. North, R. LaCourse, J. S. Mudgett, S. K. Shah, and C. F. Nathan. 1997. Identification of nitric oxide synthase as a protective locus against tuberculosis. Proc. Natl. Acad. Sci. USA 94:5243-5248.[Abstract/Free Full Text]
    39. 39
  39. Manor, E., and I. Sarov. 1990. Inhibition of Rickettsia conorii growth by recombinant tumor necrosis factor alpha: enhancement of inhibition by gamma interferon. Infect. Immun. 58:1886-1890.[Abstract/Free Full Text]
    40. 40
  40. Marrie, T. J. 1990. Epidemiology of Q fever, p. 49-70. In T. J. Marrie (ed.), Q fever, vol. 1. The disease. CRC Press, Boca Raton, Fla.
    41. 41
  41. Miller, R. A., and B. E. Britigan. 1995. The formation and biological significance of phagocyte-derived oxidants. J. Investig. Med. 43:39-49.[Medline]
    42. 42
  42. Miller, R. A., and B. E. Britigan. 1997. Role of oxidants in microbial pathophysiology. Clin. Microbiol. Rev. 10:1-18.[Abstract]
    43. 43
  43. Murray, H. W., and D. M. Cartelli. 1983. Killing of intracellular Leishmania donovani by human mononuclear phagocytes: evidence for oxygen-dependent and -independent leishmanicidal activity. J. Clin. Investig. 72:32-39.
    44. 44
  44. Murray, H. W., and C. F. Nathan. 1999. Macrophage microbicidal mechanisms in vivo: reactive nitrogen versus oxygen intermediates in the killing of intracellular visceral Leishmania donovani. J. Exp. Med. 189:741-746.[Abstract/Free Full Text]
    45. 45
  45. Pacelli, R., D. A. Wink, J. A. Cook, M. C. Krishna, W. DeGraff, N. Friedman, M. Tsokos, A. Samuni, and J. B. Mitchell. 1995. Nitric oxide potentiates hydrogen peroxide-induced killing of Escherichia coli. J. Exp. Med. 182:1469-1479.[Abstract/Free Full Text]
    46. 46
  46. Pfefferkorn, E. R. 1984. Interferon-gamma blocks the growth of Toxoplasma gondii in human fibroblasts by inducing the host cell to degrade tryptophan. Proc. Natl. Acad. Sci. USA 81:908-912.[Abstract/Free Full Text]
    47. 47
  47. Pick, E. 1986. Microassays for superoxide and hydrogen peroxide production and nitroblue tetrazolium reduction using an enzyme immunoassay microplate reader. Methods Enzymol. 132:407-421.[Medline]
    48. 48
  48. Raoult, D. 1990. Host factors in the severity of Q fever. Ann. N. Y. Acad. Sci. 590:33-38.[Medline]
    49. 49
  49. Raoult, D. 1993. Treatment of Q fever. Antimicrob. Agents Chemother. 37:1733-1736.[Free Full Text]
    50. 50
  50. Raoult, D., P. Brouqui, B. Marchou, and J.-A. Gastaut. 1992. Acute and chronic Q fever patients with cancer. Clin. Infect. Dis. 14:127-130.[Medline]
    51. 51
  51. Raoult, D., P. Houpikian, H. Tissot Dupont, M. J. Riss, J. Arditi-Djiane, and P. Brouqui. 1999. Comparison of 2 regimens containing doxycycline and ofloxacin or hydroxychloroquine. Arch. Intern. Med. 159:167-273.[Abstract/Free Full Text]
    52. 52
  52. Scanga, C. A., V. P. Mohan, K. Tanaka, D. Alland, J. L. Flynn, and J. Chan. 2001. The inducible nitric oxide synthase locus confers protection against aerogenic challenge of both clinical and laboratory strains of Mycobacterium tuberculosis in mice. Infect. Immun. 69:7711-7717.[Abstract/Free Full Text]
    53. 53
  53. St. John, G., and H. M. Steinman. 1996. Periplasmic copper-zinc superoxide dismutase of Legionella pneumophila: role in stationary-phase survival. J. Bacteriol. 178:1578-1584.[Abstract/Free Full Text]
    54. 54
  54. Turco, J., H. A. Thompson, and H. Winkler. 1984. Interferon-{gamma} inhibits growth of Coxiella burnetii in mouse fibroblasts. Infect. Immun. 45:781-783.[Abstract/Free Full Text]
    55. 55
  55. Vazquez-Torres, A., J. Jones-Carson, P. Mastroeni, H. Ischiropoulos, and F. C. Fang. 2000. Antimicrobial actions of the NADPH phagocyte oxidase and inducible nitric oxide synthase in experimental salmonellosis. I. Effects on microbial killing by activated peritoneal macrophages in vitro. J. Exp. Med. 192:227-236.[Abstract/Free Full Text]
    56. 56
  56. Weiss, S. J. 1986. Oxygen, ischemia and inflammation. Acta Physiol. Scand. 548(Suppl.):9-37.
    57. 57
  57. Zamboni, D. S., and M. Rabinovitch. 2003. Nitric oxide partially controls Coxiella burnetii phase II infection in mouse primary macrophages. Infect. Immun. 71:1225-1233.[Abstract/Free Full Text]

Infection and Immunity, November 2004, p. 6666-6675, Vol. 72, No. 11
0019-9567/04/$08.00+0     DOI: 10.1128/IAI.72.11.6666-6675.2004
Copyright © 2004, American Society for Microbiology. All Rights Reserved.



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