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Mycobacterium avium (MAV) and M. abscessus (MAB) are ubiquitous environmental organisms increasingly recognized to cause chronic lung disease in patients with apparently normal immune function. Little is yet known about their human pathophysiology. Our objective was to examine cytokine and chemokine responses (protein and gene expression) and signaling pathways triggered by reference and clinical isolates of MAB and MAV in human peripheral blood mononuclear cells, monocytes, and murine bone marrow–derived macrophages in vitro. MAB-induced TNF-α production was higher than that induced by MAV. IFN-γ, IL-1β, and the chemokines macrophage inflammatory protein-1α and regulated on activation, normal T cell expressed and secreted were equally up-regulated. Differences between MAB and MAV do not require replication and are heat stable. We found no differential effect due to rough or smooth colonies within the same species. Similar to MAV, MAB triggered mitogen-activated protein kinase (MAPK) signaling and nuclear factor-κB translocation. Induction of TNF-α was dependent on MAPK pathways, since pre-incubation of cells with signaling inhibitors led to more than 85% reduction in cytokine secretion. MAB also triggered a Toll-like receptor 2 (TLR2)-mediated response that led to TNF-α production by human monocytes. Accordingly, stimulation of murine TLR2- or myeloid differentiation factor 88–deficient bone marrow–derived macrophages did not elicit TNF-α, reinforcing a critical role for TLR2 in MAB-induced cell activation. We concluded that MAB signals human cells through MAPK and TLR2 pathways and triggers more pronounced pro-inflammatory cytokines and chemokines than MAV.
This article demonstrates for the first time fundamental differences in the innate immunogenicity between Mycobacterium abscessus and M. avium in human cells, which may play roles in clinical prevalence and disease manifestations, and may impact treatment.
Mycobacteria can be categorized into the M. tuberculosis (MTB) complex and nontuberculous mycobacteria (NTM). NTM can be further classified by growth rate. M. avium (MAV), a slow-growing mycobacterium (SGM), is the most common agent of NTM lung disease, while M. abscessus (MAB), an emerging pulmonary pathogen, is responsible for the majority of lung infections due to rapid growers (RGM) (1, 2). In the United States, MAB is the third leading cause of NTM lung infection, is responsible for approximately 80% of RGM lung disease, and is associated with significant morbidity and mortality (3, 4).
NTM cause disseminated disease mainly in those with primary or acquired immune deficiencies (3–5). In contrast, lung disease is predominantly unassociated with recognized immune defects, but is seen in other chronic lung diseases such as chronic obstructive pulmonary disease (COPD) and cystic fibrosis. In addition, NTM lung infection has been increasingly recognized to occur in otherwise apparently normal individuals (5, 6). Despite in vitro susceptibilities, MAB lung disease is clinically resistant to most antibiotics and rarely cured, while MAB skin and soft tissue infections are relatively treatable (2, 7). Both TNF-α and IFN-γ play critical roles in protective immunity to mycobacterial infections and immunopathology. The relevance of these cytokines and pathways is reinforced by naturally occurring human mutations in the genes of the IFN-γ/IL-12 axis (8, 9), nuclear factor-κB (NF-κB) essential modulator (NEMO), and the increased susceptibility to mycobacterial infections seen with therapeutic TNF-α antagonists (10, 11).
Mycobacteria trigger signaling pathways, such as mitogen-activated protein kinase (MAPK) and NF-κB, involved in cytokine response and inflammation (12). These responses are linked to engagement of Toll-like receptor 2 (TLR2) and the myeloid differentiation factor 88 (MyD88), as demonstrated for MAV and MTB (13, 14). However, very little information is available on human cellular responses to MAB (15).
It has been postulated that pathogenic mycobacteria successfully reside within macrophages by inhibiting several host processes. Variability among strains is also related to colony morphology, as NTM have long been recognized to have rough and smooth colony phenotypes (16). Because lung disease due to MAB and MAV are inexplicably different, with significant clinical implications, we sought to characterize in the human system the similarities and differences between these two major pathogens. Therefore, we investigated the cytokine and transcriptional responses induced by clinical and reference strains of MAB and MAV, as well as smooth and rough colony morphotypes.
Additional detail on the methodology is provided in the online supplement.
Mycobacteria were grown to logarithmic phase in suspension, at which time aliquots were frozen and stored at −70°C until use. For confirmation of bacterial numbers, representative vials were thawed and enumerated for viable colony-forming units (CFU). NTM reference strains were MAB (ATCC 19977; ATCC, Rockville, MD), M. avium avium (MAV; ATCC 35717), M. intracellulare (MAI; ATCC 13950) and the nonpathogenic M. smegmatis (MSMg; ATCC 14468). Clinical strains were isolated from blood (disseminated; n = 4) or sputum (pulmonary; n = 11), distributed as follows: MAB, n = 5; MAV, n = 5; MAI, n = 2; and the two new species belonging to the M. abscessus/M. chelonae group, M. massiliense and M. bolletii (17, 18). Mycobacteria samples were also identified as rough (n = 7) or smooth (n = 8) isolates. For experiments using dead mycobacteria, MAV and MAB were heat-killed (80°C, 30 min) and mycobacteria was found to be greater than 99% nonviable as determined by CFU counts.
For visualization of acid-fast bacilli (AFB) in infected cultures, cells seeded on coverslips were Kinyoun stained and examined by light microscopy. For selected experiments, SYTO9-labeled (BacLight viability staining kit; Molecular Probes, Eugene, OR) live mycobacteria were used to infect the cells, which allowed their detection by flow cytometry or confocal microscopy.
Human peripheral blood mononuclear cells (PBMCs) were obtained by Ficoll-Hypaque gradient centrifugation, and elutriated monocytes were isolated from heparinized venous blood of healthy volunteers (Dept. of Transfusion Medicine, National Institutes of Health, Bethesda, MD) in accordance with approved protocols by the Institutional Review Boards of the National Institutes of Health. Cells were seeded in RPMI 1640 and infected with single-cell suspensions of each mycobacterium for different periods of time. Supernatants were harvested and assayed for detection of cytokines through a multiplex bead-based assay (Bio-Rad Laboratories, Hercules, CA), and the cells processed for RNA isolation.
Bone marrow–derived macrophages (BMM) were obtained from 6- to 8-week-old C57BL/6, TLR2-, TLR4-, or MyD88-deficient mice as previously described (19, 20). Cells were then cultured in the presence of the mycobacteria for 1, 4, and 20 h, when supernatants and cellular RNA were harvested for further use.
Total RNA was extracted from the cultured cells with the RNeasy mini kit (Qiagen, Valencia, CA), reverse transcribed, and the cDNA amplified by PCR in the ABI 7500 Sequence detector using Taqman expression assays (Applied Biosystems, Foster City, CA).
PBMCs or elutriated monocytes (106 cells/well) were pre-treated with the p38 signaling inhibitor SB203580 or the ERK1/2-selective inhibitor U0126 (10 μM) for 30 to 60 minutes before infection and then infected with MAB or MAV. In parallel experiments, cells were pre-incubated (1 h) with anti-TLR2 mAb (4 μg/ml) and stimulated further with the TLR2 agonist Pam3Cys (2 μg/ml) or the mycobacteria. Culture supernatants were harvested and assayed for cytokine activity.
After stimulation with the mycobacteria, monocytes or PBMCs (3 × 106 cells) were harvested, lysed, and processed for detection of phospho-p38 MAPK using the phospho-p38a enzyme-linked immunosorbent assay (ELISA) as directed by the manufacturer (Cell Signaling, Danvers, MA). For Western blot analysis, samples were separated on 10% SDS-PAGE, transferred to polyvinylidene difluoride membrane (Invitrogen, Carlsbad, CA), and immunoblotted with the antibodies anti–phospho-p38, anti–total p38 (Cell Signaling), and anti–β-actin (Abcam, Cambridge, MA). Reaction was detected using an enhanced chemiluminescence detection system (Amersham, Piscataway, NJ).
To evaluate NF-κB translocation, monocytes (2 × 106 cells) settled on glass coverslips were stimulated with the mycobacteria, the wells were washed, and the cells fixed in PF 3.7%. Cells were permeabilized with PBS-0.5% triton X-100, labeled with a primary antibody against phospho-p65 (Cell Signaling), followed by incubation with the secondary antibody (Chemicon International, Temecula, CA); the nuclei were stained with DAPI and images acquired on a confocal microscope.
Visualization by confocal microscopy was performed on a Leica SP5 confocal microscope (Leica Microsystems, Exton, PA) using ×20 and ×40 oil immersion objectives NA 1.4. Differential interference contrast (DIC) images were collected simultaneously with the fluorescence images using a transmitted light detector. Images were processed using Leica LAS-AF version 1.6.3 and Adobe Photoshop.
Values are expressed as mean ± SD. Differences between groups were assessed by the paired two-tailed Student's t test and the Mann-Whitney U test, using InStat/Prism software (GraphPad Software, San Diego, CA) with level of significance P < 0.05.
To determine the ability of MAB to stimulate cytokine production in primary human cells, PBMCs (n = 15) were infected in vitro (multiplicity of infection [MOI] 2.5), and the response after 20 hours of culture was compared with that of the well-characterized MAV. MAB induced significantly more TNF-α than M. avium (P = 0.014, Figure 1A) or MAI (P = 0.01, n = 8). IFN-γ (P < 0.01, Figure 1B) and IL-6 (P < 0.05, Figure 1C) were also more strongly induced by MAB than MAV or MAI. Similar profiles were also seen for IL-1β (MAB 4,550 ± 416 pg/ml, MAV 1,870 ± 640 pg/ml, MAI 1,345 ± 310 pg/ml; P = 0.01), granulocyte macrophage colony-stimulating factor (P < 0.05), and granulocyte colony-stimulating factor (P < 0.03). In contrast, production of the anti-inflammatory cytokine TGF-β was negligible during the whole culture period, whereas for IL-10, significant differences between MAB and MAV were noted (P < 0.05).
The differential response observed at the protein level was confirmed at the transcriptional level, as well. As shown in Figure 1D, TNF-α, IFN-γ (P < 0.01), and IL-6 (P < 0.05) mRNA expression in PBMCs was higher for MAB 4 hours after stimulation.
Similar patterns of mycobacteria-induced cytokines were seen regardless of whether purified elutriated monocytes or monocyte-derived macrophages (MDM) were used. The responses of monocytes to increasing bacterial ratios reached a plateau at MOI 5 to 10, with declining TNF-α production at higher MOIs. MAB induced consistently and significantly more TNF-α at all MOI tested (Figure 1E; differences were marginally significant at MOI 50, P = 0.049). Human PBMCs behaved similarly to monocytes (data not shown). Even though total cytokine production was much lower in the MDM cultures, the differential cytokine response was maintained (see Figure E1 in the online supplement). Interestingly, heat-killed MAB persistently elicited more response than heat-killed MAV both at 4 (P < 0.05) or 20 hours culture (Figure 1F, P = 0.008).
MAB in vitro production of the chemokines macrophage inflammatory protein (MIP)-1α and regulated on activation, normal T cell expressed and secreted (RANTES) in culture supernatants was significantly higher than MAV (Figure 2A, P < 0.01). In contrast, MIP-1β and monocyte chemoattractant protein-1 (MCP-1) were similarly strongly induced by the different NTM (Figure E2).
MAB- and MAV-induced TNF-α and IFN-γ secretion in PBMC cultures was assessed at 1, 4, 12, and 20 hours (Figure 2B). Although low cytokine levels were noted 1 hour after stimulation (MAB TNF-α 30 ± 47 pg/ml; IFN-γ 4 ± 5.7 pg/ml), by 3 to 4 hours cytokine values were easily detectable. Cytokine induction by MAB was consistently higher and was well established by 4 hours. IL-10 and IL-1β protein levels were detected in the culture supernatants mainly after 20 hours (not shown). This profile was sustained at the mRNA level as well: TNF-α message peaked at 4 hours for both mycobacteria (Figure 2C, left panel); for IL-10, peak of response occurred at 12 hours (not shown), whereas for IFN-γ, up-regulation of mRNA was still detected after 20 hours (Figure 2C, right panel).
Cultured monocytes on coverslips were fixed with methanol and Kinyoun stained for determination of rate of AFB infection (Figure 3A). At 4 to 6 hours of culture, bacteria were associated with 15 to 18% of cells (total 200–300 cells counted per slide), increasing to 35 to 40% at 20 hours. After adding the mycobacteria to the PBMC cultures, small aggregates of cells were already seen after 1 to 4 hours. These aggregates progressively increased in number and size after 18 to 24 hours (Figure 3B). Labeling mycobacteria with a fluorescent dye before infection followed by confocal microscopy confirmed the bacteria to be mainly inside the cells and within the cell aggregates (Figures 3C and 3D). The total percentage of CD14+ cells containing labeled bacteria at 20 hours in culture was confirmed by flow cytometer (38.4 ± 6.4% for MAB and 36.6 ± 5.5% for MAV).
To determine whether the differences observed between the two mycobacterial species were maintained among clinical isolates, monocytes were cultured (n = 10) with different clinical samples. Clinical isolates from MAB (clinAB1, clinAB2, clinAB3) and MAV (clinAV1, clinAV2, clinAV3) were assayed in parallel. TNF-α protein and message, and IFN-γ secretion (assessed at 4 and 20 h), confirmed among clinical isolates the significant differences observed between the reference strains (Figures 4A and 4B). In addition, two clinical isolates of MAI (MAIclin1, TNF-α 17,497 ± 1,050 and MAIclin2 15,184 ± 3,995 pg/ml) and of the recently characterized MAB-related rapid growers, M. massiliense (M. mass.1, 42,176 ± 4,900; M. mass.2, 28,147 ± 2,550) and M. bolletii (34,303 ± 950 pg/ml), showed similar strain-related differences in TNF production in the infected cells as did reference MAB and MAV (Figure 4C).
To explore further the clinical isolates compared with the reference strains, we grouped mycobacteria according to whether their culture morphotype was rough or smooth. We found no significant differences (P > 0.05) in induced TNF-α levels by rough (rg) or smooth (sm) isolates within the same group (MAB or MAV) (MABrg, 38,595 ± 4,557; MABsm, 47,750 ± 7,783; MAVrg, 15,654 ± 3,840; MAVsm, 18,244 ± 6,414pg/ml) (Figure 4D). Accordingly, differences between the reference strains (smooth morphotype) and between MAB and MAV clinical isolates were maintained despite their characteristic morphotypes (P < 0.05).
To compare MAV and MAB responses to those of nonpathogenic mycobacteria, PBMCs (or monocytes) were challenged with MSMg. MSMg induced significantly more TNF-α than did MAB, MAV, or MAI after 4 (not shown) and 20 hours in culture (Figure E3, P < 0.05).
We investigated p38 MAPK activation in primary human monocytes after mycobacterial stimulation in vitro. A kinetic analysis of p38 phosphorylation evaluated by an enzymatic binding assay was performed in cultured cells infected with either MAB or MAV (MOI 5) with cell lysates harvested at 2, 10, and 30 minutes, and at 1, 2, 12, and 20 hours. Both MAB and MAV (Figure 5A) triggered p38 MAPK phosphorylation by 2 minutes, which persisted up to 20 hours, without major differences between them. MAPK phosphorylation by ELISA correlated with the expression pattern seen on immunoblot (Figure 5B, also shown by densitometry). Both reference strains and clinical isolates of MAB and MAV induced rapid and sustained p38 MAPK phosphorylation (Figure E4).
To establish whether MAPK activation was necessary for mycobacteria-induced monocytes or PBMC TNF-α production, cells were pre-treated with the p38 MAPK inhibitor SB203580 or the ERK inhibitor UO126 and then challenged with viable mycobacteria. Neither cell viability (trypan blue exclusion) nor extent of infection was affected by the inhibitors (not shown). Pre-treatment of cultures with the p38 MAPK inhibitor SB203580 reduced TNF-α release induced by either MAB and MAV or their corresponding clinical isolates (data not shown) to less than 5% of vehicle control (Figure 5C and Table 1). Results were similar at both MOI 5 and 2.5.
Blocking the ERK 1/2 pathway also reduced TNF-α to less than 20% of vehicle in response to MAB or MAV (Table 1). Both inhibitors showed the same effect whether mycobacteria colony morphotype was rough or smooth (not shown). However, the inhibitors had different impacts on the production of other monocyte-secreted cytokines. In the presence of the p38 inhibitor, IL-10 was greatly reduced (> 90%), whereas IL-6 was only moderately affected; on the other hand, the ERK1/2 inhibitor interfered only partially with IL-6 and IL-10 (35–45% inhibition, Table 1).
Mycobacteria are known to trigger the NF-κB pathway, which is also involved in cytokine response. We assayed the ability of MAB to induce NF-κB translocation in monocytes or MDM cultures by confocal analysis. Specific staining for phosphorylated p65 showed MAB-induced activation of NF-κB in cultured cells to the same extent as seen with MAV (Figure 6).
Both p38 and NF-κB signaling pathways are activated by engagement of TLRs. To evaluate whether MAB triggered TLR2 signaling, human monocytes were infected in the presence or absence of an anti-human TLR2 monoclonal antibody. Mycobacteria-induced TNF-α production was reduced by 52 ± 12% in treated cultures (Figure 7A), whereas TNF-α induction by the specific TLR2 agonist Pam3Cys was completely abrogated.
To further confirm the importance of TLR2 signaling for MAB responses, murine BMM cultures from TLR2-deficient and wild-type (WT) C57BL/6 mice were established and infected with either MAB or MAV (MOI 5). After 1, 4, or 20 hours, supernatants were harvested and assayed for cytokines by specific ELISA. TNF-α induction by the two NTM species in the WT BMM cultures, although not statistically significant, showed a trend for higher values in response to MAV earlier in culture (1 and 4 h), and in response to MAB only after 20 hours of stimulation (Figure 7B). Moreover, cells from TLR2- or MyD88-deficient (Figure 7C), but not TLR4−/− mice (not shown), showed no TNF-α protein release or mRNA (Figure 7D) expression after exposure to either NTM. Control experiments showed the response of BMM cells to LPS to be abolished in the TLR4−/− and MyD88−/− mice (Figure E5).
Murine bone marrow–derived dendritic cells (BMDCs) were also generated from both WT and TLR2−/− mice as previously described (20). In contrast to WT BMDC cultures, neither TNF-α nor IL-12p40 were induced at 4 or 20 hours after challenge of TLR2−/−BMDCs with mycobacteria (not shown), confirming an essential role for TLR2 signaling in MAB and MAV interaction with macrophages and dendritic cells.
M. abscessus is a significant pulmonary pathogen in patients with bronchiectasis. However, despite its relative importance, very little has been learned about its human pathophysiology. We challenged freshly isolated primary human PBMCs and monocytes with a number of reference and clinical bacterial isolates in vitro. Both reference and clinical strains of MAB were more potent inducers of cytokine and chemokine secretion from human mononuclear cells than MAV. This property was somewhat specific, with increased production of TNF-α, IFN-γ, IL-1β, RANTES, and MIP-1α, but not MIP-1β or MCP-1. The prompt enhanced production of both TNF-α and IFN-γ implies a prominent immediate T cell response induced by MAB. To our knowledge, this is the first description of the profile and kinetics of MAB-induced response in primary human cells.
The differential ability of species of NTM (e.g., MAV, MSMg) and MTB to induce TNF-α production seems to be inversely related to their virulence, as assessed in murine models and human macrophages (21–24). Studies in the monocytic cell line THP1 showed similar profiles when comparing BCG, MTB, and M. leprae (12, 23, 24). It has been suggested that “virulent” strains elicit less activation of cellular effector mechanisms, thereby escaping early elimination and allowing establishment of infection. In line with this, MAV is a much more common pulmonary and disseminated pathogen than MAB. The additional observation that MSMg induced even higher cytokine response than MAB reinforces this hypothesis.
The dual roles of TNF-α in protection and pathology are well recognized (25). Our observation that MAB induces more inflammatory response than MAV could be associated with the limited number of patients within this infection population compared with MAV, and may explain the devastating lesions induced by MAB when infection is established, which is also consistent with the clinical observation of MAB infection in patients receiving TNF-inhibitor therapies (11).
TNF-α and IFN-γ are central to granuloma formation, directly and through the regulation of chemokines. RANTES and MIP-1α are chemotactic for macrophages, neutrophils, and lymphocytes; are up-regulated during inflammation in pulmonary alveolar macrophages; and play a role in the pathogenesis of COPD (25–27). It is therefore tempting to hypothesize that in the setting of NTM lung disease MAB-induced up-regulation of RANTES and MIP-1α could exacerbate the clinical picture. In vitro models allow study of the expression of these molecules in granulomas (28). The cellular aggregates found in the infected culture wells may be surrogate makers for cell interaction, as reported previously (29) and may well represent the actual site at which the response occurs.
Previous studies have shown that mycobacteria trigger signaling pathways such as MAPK and NF-κB through engagement of TLRs (12, 14, 30–32). Similar to MAV, MAB induces NF-κB nuclear translocation and activates the p38 and ERK1/2 MAPK signaling pathways. Published data have indicated p38 and ERK activation to be required for mycobacteria-induced TNF-α secretion (12, 21, 31). Here we confirmed and demonstrated that these pathways were necessary for appropriate TNF-α response to MAB as well, since specific pharmacologic inhibitors interfered with MAV- and MAB-induced cytokine secretion. Early signal transduction events induced by NTM also showed differential induction of IL-10 and IL-6. In contrast to a previous study (33), we found induction of those cytokines to be critically dependent on p38 MAPK activity, but only partially dependent on the ERK1/2 pathway. Such differential requirements for the activity of both pathways for TNF and IL-10 release could be related to the type of cell used in the experiments and/or to the bacterial isolates tested, which in the former case were obtained from patients with AIDS (33).
The reproducibility of the relationships between reference and clinical isolates by species is striking. When we tested different clinical isolates of either MAB or MAV, we repeatedly found differential cytokine response in the clinical isolates similar to what was seen between the reference strains. Such an array of responses induced by NTM is likely due to the diverse lipids in the outer layer of the bacterial cell wall including glycolipids, glycopeptidolipids (GPLs), and phenolglycolipids (PGL). PGL, carried by the hypervirulent MTB W-Beijing and the PGL-1 of M. leprae, seem to play a major role in pathogenicity by interfering with the host immune system (34–37). Previous studies of the NTM colony morphotypes (16, 38) implied the rough variant to have different or to lack GPLs and induce more inflammatory response than the smooth morphotype (16, 38–40). Surprisingly, despite differences between species, we did not find any significant differences between rough and smooth morphotypes within the same species in terms of cytokine production or MAPK signaling.
There is also a lack of association between mycobacterial colonial morphotype and clinical features in our patients infected with either MAB or MAV (S. M. Holland, unpublished data). Moreover, mycobacterial isolates from the same patient can grow both rough and smooth morphotypes, even from the same clinical sample (Y. Shea, unpublished data).
The genetic and biochemical bases for the different morphotypes remain unclear. Recently, genome sequencing of two RGM that cause human infections, MAB and M. chelonae (41), found that GPL genes are scattered, unlike in MSMg, where they are clustered. Such studies may help to better understand lipid synthesis and regulation by the different mycobacteria.
TLRs are activated by components of pathogens, and more than one TLR molecule may mediate protection from and response to mycobacteria (14, 20). Engagement and activation of TLR2 by MAB was confirmed by experiments with both human and mouse cells, similar to what has been shown for MAV (13, 42). Complete abrogation of TLR response in the human system is difficult to achieve in vitro, and may reflect either incomplete TLR2 blockade by existing reagents or the existence of other receptors that lead to cell stimulation in response to NTM. However, experiments using cells from TLR2 knockout and MyD88 knockout mice confirmed the nonredundant roles of TLR2 and the downstream adaptor molecule MyD88 (13, 42) in host resistance and response to MAB and MAV.
IFN-γ, T cell response, and TNF-α are essential for control of M. abscessus in a mouse model (43). Our data strongly support these findings and show cellular immune mechanisms involved in the early human response to M. abscessus. Innate immune responses induced by these mycobacteria may set the stage for clinical features and outcomes that are specific manifestations of infection with MAB and MAV.
Differences between MAB and MAV are seen early after infection, with MAB causing higher responses than MAV as early as 4 hours after stimulation. Heat-killed MAB still elicit more TNF than heat-killed MAV, indicating that the different inflammatory factors between MAB and MAV do not require replication or metabolism and are heat stable. After TLR activation, it is possible that other components that lead to down-regulation of immune/inflammatory response may be more prominently triggered by MAV, including the activation of phosphatases that will ultimately inactivate MAPKs. Such factors can be induced in macrophages by mycobacterial components, such as lipomannan (44), and offers an attractive feedback loop for modulating mycobacterially induced cell response in vivo. Experiments to characterize these activities are underway.
In conclusion, the initiation of marked gene transcription and cytokine/chemokine responses induced by NTM in vitro begins within minutes after infection and is already significantly different between species at very early time points. This in vitro effect may reflect the inflammation and clinical features caused by MAB, and may help to provide new targets for future clinical intervention in NTM induced lung disease.
The authors are grateful to K. Olivier for helpful scientific discussion, to J. Root and D. S. Carvalho for technical assistance, and to A. Woodworth for efficient secretarial help. Thanks are also due to M. Czapiga and D. Stephany for professional assistance with the confocal and flow cytometry experiments.
This study was supported by the Division of Intramural Research of the NIAID, National Institutes of Health ZO1-AI-00647–06 (to S.M.H.) and funding from the NIH/FIOCRUZ interchange research program.
This article has an online supplement, which is accessible from this issue's table of contents at www.atsjournals.org
Originally Published in Press as DOI: 10.1165/rcmb.2007-0413OC on April 25, 2008
Conflict of Interest Statement: None of the authors has a financial relationship with a commercial entity that has an interest in the subject of this manuscript.