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Comparative Signature-Tagged Mutagenesis Identifies Pseudomonas Factors Conferring Resistance to the Pulmonary Collectin SP-A

  • Shiping Zhang,

    Affiliation Division of Pulmonary and Critical Care Medicine, University of Cincinnati College of Medicine, Cincinnati, Ohio, United States of America

  • Yi Chen,

    Affiliation Division of Pulmonary and Critical Care Medicine, University of Cincinnati College of Medicine, Cincinnati, Ohio, United States of America

  • Eric Potvin,

    Affiliation Centre de Recherche sur la Fonction Structure et Ingenierie des Proteines, Universite Laval, Ste-Foy, Quebec, Canada

  • Francois Sanschagrin,

    Affiliation Centre de Recherche sur la Fonction Structure et Ingenierie des Proteines, Universite Laval, Ste-Foy, Quebec, Canada

  • Roger C Levesque,

    Affiliation Centre de Recherche sur la Fonction Structure et Ingenierie des Proteines, Universite Laval, Ste-Foy, Quebec, Canada

  • Francis X McCormack,

    Affiliation Division of Pulmonary and Critical Care Medicine, University of Cincinnati College of Medicine, Cincinnati, Ohio, United States of America

  • Gee W Lau

    To whom correspondence should be addressed. E-mail:

    Affiliation Division of Pulmonary and Critical Care Medicine, University of Cincinnati College of Medicine, Cincinnati, Ohio, United States of America

Comparative Signature-Tagged Mutagenesis Identifies Pseudomonas Factors Conferring Resistance to the Pulmonary Collectin SP-A

  • Shiping Zhang, 
  • Yi Chen, 
  • Eric Potvin, 
  • Francois Sanschagrin, 
  • Roger C Levesque, 
  • Francis X McCormack, 
  • Gee W Lau


The pulmonary collectin, surfactant protein A (SP-A), is a broad spectrum opsonin with microbicidal membrane permeabilization properties that plays a role in the innate immune response of the lung. However, the factors that govern SP-A's microbial specificity and the mechanisms by which it mediates membrane permeabilization and opsonization are not fully understood. In an effort to identify bacterial factors that confer susceptibility or resistance to SP-A, we used comparative signature-tagged mutagenesis to screen a library of 1,680 Pseudomonas aeruginosa mutants for evidence of differential pulmonary clearance in SP-A-sufficient (SP-A+/+) and SP-A-deficient (SP-A−/−) mice. Two SP-A-sensitive P. aeruginosa mutants harboring transposon insertions in genes required for salicylate biosynthesis (pch) and phosphoenolpyruvate-protein-phosphotransferase (ptsP) were recovered. The mutants were indistinguishable from the parental wild-type PA01 with regard to opsonization by SP-A, but they exhibited increased susceptibility to SP-A-mediated membrane permeabilization. These results suggest that bacterial gene functions that are required to maintain membrane integrity play crucial roles in resistance of P. aeruginosa to the permeabilizing effects of SP-A.


Everyday, normal breathing deposits numerous microorganisms on the surfactant membrane that lines the air-exchanging surfaces of the lung. Surfactant protein SP-A, a component of the surfactant membrane, helps to maintain the lung in a germ-free state by aggregating inhaled microorganisms and facilitating their ingestion by immune cells, and by increasing the permeability of their cell membranes. However, the bacterial pathogen Pseudomonas aeruginosa is resistant to SP-A-mediated membrane disruption.

Using a genetic tool called comparative signature-tagged mutagenesis, the authors have identified two P. aeruginosa genes, pch and ptsP, that are required to resist SP-A-mediated membrane permeabilization. Molecular analyses indicate that the pch gene encodes an enzyme that synthesizes salicylate, a compound utilized by bacteria to acquire essential metal ions. The ptsP gene encodes an enzyme called phosphoenolpyruvate-protein-phosphotransferase. The loss of salicylate and phosphoenolpyruvate-protein-phosphotransferase weakens the P. aeruginosa cell membrane, which allows SP-A to poke holes on the membrane and kill the bacteria.

This is the first known report of the roles played by salicylate and phosphoenolpyruvate-protein-phosphotransferase in maintenance of bacterial membrane, and consequently, protecting bacteria from killing by SP-A, through disruption of membrane integrity.


Pulmonary surfactant is a protein-phospholipid complex that lines the air-liquid interface of alveoli, forming the first point of contact with inhaled microbial pathogens [1,2]. A multitude of in vitro studies have demonstrated that the pulmonary collectins, surfactant protein A (SP-A) and surfactant protein D (SP-D), bind and aggregate bacterial, fungal, viral, and mycobacterial organisms, directly activate macrophages, and enhance the in vitro phagocytosis and intracellular killing of a variety of pulmonary pathogens [3,4]. Recognition of diverse microbial species by the pulmonary collectins is mediated by the C-type lectin domain, which selectively binds to carbohydrates that are prevalent on the surface of microbes, but not to the predominant terminal sugars on surface molecules of mammalian cells [5]. More recently, SP-A and SP-D have been reported to possess potent antimicrobial properties [68]. They directly inhibit the proliferation of bacteria and fungi in a macrophage- and aggregation-independent manner, by increasing the permeability of the microbial cell membrane. In particular, rough strains of Gram-negative bacteria, containing truncated lipopolysaccharide (LPS) domains are uniquely vulnerable to permeabilization by the collectins [6], as has been well known for other antimicrobial peptides and proteins.

Although the collectins inhibit microbial growth, the factors that govern the specificity and the mechanisms of membrane disruption by the collectins are not understood. In this study, we employed comparative signature-tagged mutagenesis (STM) as a tool to identify bacterial factors required to resist SP-A-mediated clearance, in vivo. STM relies on the ability of the pathogen in question to replicate in vivo as a mixed population and allows for the identification of the mutants whose phenotypes cannot be trans-complemented by other virulent strains present in the same inoculum [9]. Two Pseudomonas factors that are specifically required to protect P. aeruginosa from killing by SP-A were identified and characterized.


SP-A−/− Mice Are Susceptible to Infection by P. aeruginosa

Levine et al [10] have reported that outbred SP-A−/− mice exhibit delayed clearance of a clinical P. aeruginosa strain from the lung, suggesting that SP-A plays a role in pulmonary innate immunity against this organism. We also found that the inbred C3H/HeN SP-A−/− mice were more susceptible to P. aeruginosa infection, in this case by strain PA01. SP-A+/+ mice cleared 63-fold (1.8 log) more of intranasally inoculated PA01 by 16 h (Figure 1A). In contrast, the bacterial load increased by 22 fold (1.34 log) in SP-A−/− mice (Figure 1A). In the absence of infection, SP-A−/− mice are healthy, and the histopathological analyses of their non-infected lungs revealed no significant differences when compare to the lungs of SP-A+/+ mice (unpublished data). When infected with PA01 however, SP-A+/+ mice developed broncho-pneumonia with mild pulmonary infiltrates (Figure 1B). In contrast, SP-A−/− mice developed more extensive consolidation with areas of lobar pneumonia.

Figure 1. SP-A Deficient Mice Are More Susceptible to Infection by P. aeruginosa

(A) SP-A+/+ and SP-A−/− mice (group of six) were infected intranasally with 1 × 107 P. aeruginosa PA01. Bacteria were recovered from homogenized lung tissue 16 h after inoculation. p < 0.01.

(B) Representative lung histology sections (stained with hematoxylin and eosin) from SP-A+/+ and SP-A−/− mice 16 h post intranasal instillation of PA01. Original magnification: 10 ×.

Identification of P. aeruginosa Genes Conferring Resistance to SP-A by Comparative STM Screening

We exploited the PCR-based STM technique and the P. aeruginosa PA01 STM mutant library [11] to identify putative microbial targets for SP-A. SP-A+/+ and SP-A−/− mice, in groups of three, were intranasally challenged with pools of 72 oligo-tagged STM mutants. Lungs were harvested at 16 h, homogenized, and plated. At least 10,000 bacterial colonies grown on Luria broth (LB) agar plates were harvested from each lung for bacterial genomic DNA extractions and oligo-tag amplification. We screened for differential clearance of individual STM mutants using PCR. If the PCR product of a mutated gene was absent on the output gel in SP-A+/+ mice, but present in SP-A−/− mice (Figure 2A, see arrows), we postulated that the bacterial protein encoded by the mutated gene was required to overcome the host defense activities of SP-A.

Figure 2. PCR-Based Signature-Tagged Mutagenesis

(A) Schematic drawing of PCR-based STM. Pools of 72 uniquely tagged mutants were intranasally inoculated into SP-A+/+ and SP-A−/− mice; 16 h later, lungs were harvested, homogenized, and plated. Approximately 10,000 colonies were harvested from the plates for genomic DNA extraction. PCR-amplification of tags was performed on the genomic DNA to screen for the presence or absence of DNA tags of each of the 72 mutants. Mutants whose DNA tags were present in the input pool and in the SP-A−/− pool, but absent in the SP-A+/+ pool (see white arrows) were further screened for susceptibility to SP-A.

(B) Agarose gel of PCR-based STM, identifying the pch mutant (left panel). Attenuation in the first SP-A+/+ mouse (right panel, m1) was confirmed in two additional SP-A+/+ mice (right panel, m2 and m3).

(C) Genetic loci of P. aeruginosa, when mutated, conferred increased sensitivity to in vivo killing by SP-A. DNA regions flanking pUTmini-Tn5 transposon insertions were cloned and sequenced. Similarity BLAST searches were performed against P. aeruginosa PA01 genomic sequence on NCBI and on Black arrows indicate the approximate insertion site within the mutated ORFS.

(D) TLC analyses indicate that the pch STM mutant is unable to synthesize pyochelin (see arrows). Wild-type PA01 grown in LB and the pch mutant grown in LB supplemented with 1 mM salicylate produced green color pyochelin (see arrows). In contrast, no observable pyochelin was produced by the pch and PA06331 strains. Pure pyochelin was used as control.

(E) Restriction fragment length polymorphism analysis between parental wild-type PA01 and STM mutants confirmed that mutations in pch and ptsP were caused by a single insertion.

We comparatively screened 1,680 STM mutant strains in SP-A+/+ and SP-A−/− mice. Two mutants with increased sensitivity to SP-A (i.e., failed to survive in SP-A+/+ mice) were recovered, for a 0.12% recovery rate. We have cloned and sequenced both STM mutants by plasmid rescue [11]. DNA sequences were analyzed by comparison with online databases ( The output from Pool 4 (mutant pch, see below) is shown in Figure 2B (left panel). In the presence of SP-A, the pch mutant, which is disrupted in a gene required for salicylate biosynthesis, was unable to survive in the SP-A+/+ lung (missing band in the box, Figure 2B). In absence of SP-A, the pch mutant was able to grow in the lung, as indicated by the presence of an oligo-tag amplified by PCR (Figure 2B, left panel, SP-A−/− lane; right panel, lane m1). The results were confirmed by PCR analysis of the output pool of two additional mice (Figure 2B, right panel, lanes m2 and m3).

The pch STM mutant carries a transposon pUTminiTn5Km2 insertion within an intergenic region in between the 10th and 11th nucleotide after the stop codon of the pchA (PA4231) gene (Figure 2C). The pchA gene encodes an isochorismate synthase that participates in the biosynthesis of the siderophores, salicylate, and pyochelin [1214]. Because transposon inserted within the intergenic region immediately downstream of the pchA gene, it might have affected the mRNA stability of the pchDCBA transcript. Thus, we named the STM mutant as pch. We examined whether the pch mutant had lost the ability to synthesize pyochelin by using thin layer chromatography (TLC) assays. TLC analysis of pyochelin extracted from bacteria cultured in M63 minimal medium confirmed that the pch mutant is unable to synthesize the green-colored pyochelin (Figure 2D, pch lane). In contrast, the parental wild-type PA01 produced pyochelin (Figure 2D, PA01 lane). When the pch STM mutant was grown in the presence of 1 mM salicylate, however, the ability to synthesize pyochelin was restored (Figure 2D, pch + 1mM salicylate lane). The expression of the genes within the downstream operon (PA4232 and PA4233), which is transcribed in opposite orientation to the pchADCBA operon, was found to be unaffected by transposon insertion as assessed by mRNA expression analyses (unpublished data). Collectively, these data suggest that susceptibility to SP-A-mediated clearance is caused by the loss of pch gene function, most probably by affecting the mRNA stability of the pchDCBA operon.

The second SP-A-susceptible STM mutant had the transposon pUTminiTn5Km2 inserted in between the 2,213th and 2,214th nucleotides of the ptsP (PA0337) gene (Figure 2C). The ptsP gene encodes a phosphoenolpyruvate-protein-phosphotransferase, a homolog of the E. coli Enzyme Initrogen (EINtr) [15]. The transposon pUTminiTn5Km2 insertion into ptsP is predicted to cause polarity and interrupt the transcription of PA0338.

Both STM mutants were judged to harbor a single transposon pUTminiTn5Km2 insertion after hybridization with the transposon vector (unpublished data). DNA fragments that flanked both ends of the transposon integrations in pchA and ptsP genes were cloned from the wild-type PA01. They were used to confirm gene interruption by the integrating transposon, by comparing restriction fragment length polymorphisms (RFLP) between wild-type PA01 and the STM mutants. As shown in Figure 2E, transposon-flanking DNA probes hybridized to DNA fragments with higher molecular weights in the chromosomes of both the pch and ptsP mutants than their parental strain PA01, indicating transposon insertion.

SP-A-Sensitive STM Mutants Are as Virulent as Parental Wild-Type in SP-A−/− Mice

Apart from confronting pulmonary host defenses, our STM screens require each mutant to compete with 71 other STM mutants within individual library pools. Competitive mixed infection assays have been widely used to assess the fitness of individual mutants versus their parental strains during in vivo infection [16,17]. As shown in Figure 3A, when co-administered with the parental wild-type PA01 by intranasal inoculation into mice, both STM mutants were less competitive than PA01 in SP-A+/+ mice. Specifically, mutant strains pch and ptsP were only 53% and 46% as competitive as PA01, respectively. In contrast, both mutants performed equally well as, if not better than, the wild-type strain in SP-A−/− mice (Figure 3A).

Figure 3. SP-A-Sensitive P. aeruginosa STM Mutants Compete Effectively with Parental Wild-Type PA01 in SP-A−/− , but Not in SP-A+/+ Mice

(A) In vivo competition assays between the wild-type and individual STM mutants after intranasal pulmonary inoculation of 6-wk-old SP-A+/+ and SP-A−/− mice. The mean CFU recovered from four mice in each group is shown. The CI is defined as the output ratio of mutant to wild-type bacteria divided by the input ratio of mutant to wild-type bacteria. *p < 0.013, #p < 0.011.

(B) Single respiratory tract infection of pch and ptsP mutants in SP-A+/+ and SP-A−/− mice was performed as described for Figure 1. Attenuation is defined as the log10 difference in CFU between wild-type and mutant bacteria recovered from lung tissue 16 h after inoculation. The mean ± standard error of six mice is shown. *p < 0.019, #p < 0.045.

We further tested the mutants, pch and ptsP, in single infection studies. When infected singly into wild-type mice, the viable bacterial counts of pch and ptsP mutant bacteria were 32-fold (1.5 log) and 25-fold (1.4 log) higher, respectively, in SP-A−/− mice than in SP-A+/+ mice (Figure 3B). Our results indicate that SP-A plays an important role in clearance of PA01 mutants with defective pch or ptsP gene function.

Preferential Clearance of the STM Mutants from SP-A+/+ Lung Is Independent of Macrophages

Previous studies have suggested that SP-A opsonizes P. aeruginosa and increases uptake by macrophages [10,18]. To determine if SP-A-mediated opsonization contributes to the early clearance of STM mutants, we compared the phagocytosis of pch and ptsP to PA01 in the presence and absence of SP-A. When live, green fluorescence protein (GFP)-expressing bacteria were exposed to mouse alveolar macrophages in the presence of SP-A, the uptake of PA01, its pch, or ptsP mutant was increased by 1.8, 1.3, and 1.6 fold, respectively, over that which occurred in the absence of SP-A (Figure 4A). However, the SP-A mediated increase in opsonization was only statistically significant in PA01 (p<0.01). The magnitude of the increase in the uptake of PA01 in the presence of SP-A was similar to previously published reports [10,18]. Although the addition of SP-A increased the macrophage uptake of STM mutants, enhancement of phagocytosis was slightly lower than that of wild-type PA01. Therefore, it does not appear that SP-A-mediated opsonization is responsible for the preferential clearance of pch and ptsP mutants from SP-A+/+ mice.

Figure 4. Bacterial Opsonization by SP-A Does Not Result in Differential In Vivo Phagocytosis and Killing of STM Mutants

(A) In vitro phagocytosis assays were performed using live, GFP-expressing PA01 and isogenic pch and ptsP bacteria, with alveolar macrophages isolated from SP-A+/+ mice. Internalized bacteria were counted using a phase contrast fluorescence microscope. The means of three experiments are shown. Two hundred macrophages were counted for each mouse. p = 0.0058 (PA01 vs PA01 + SP-A), p = 0.075 (pch vs pch + SP-A), and p = 0.109 (ptsP vs ptsP + SP-A).

(B) In vitro phagocytosis of PA01, pch, and ptsP by human neutrophils isolated from healthy volunteers. Phagocytosis experiments were performed as described for (A). p = 0.037 (PA01 vs PA01 + SP-A), p = 0.577 (pch vs pch + SP-A), and p = 0.919 (ptsP vs ptsP + SP-A).

(C–E) SP-A did not affect uptake or killing of STM mutants. PA01 (C), but not the STM mutants pch (D) and ptsP (E) were killed in significant amounts by neutrophils, independent of SP-A. The mean of three separate experiments is shown. p < 0.001 when comparing PA01 versus PA01 + neutrophils, and when comparing PA01-SP-A versus PA01-SP-A + neutrophils.

Preferential Clearance of the STM Mutants in SP-A+/+ Lung Is Independent of Neutrophils

Neutrophils are known to play a major role in protecting the lung against bacterial infection. We examined whether bacterial phagocytosis and killing by neutrophils might have led to preferential clearance of pch and ptsP. As shown in Figure 4B, the uptake of PA01 and the pch and ptsP mutants was not increased in the presence of SP-A. In fact, SP-A-opsonized PA01 bacteria were phagocytosed less efficiently by neutrophils than untreated bacteria. Interestingly, only wild-type PA01 bacteria were susceptible to killing by neutrophils, with approximately 73.7% killed in the absence of SP-A, and 57.2% killed in the presence of SP-A (Figure 4C). In contrast, both pch and ptsP mutants were not susceptible to neutrophil killing (Figure 4D and 4E). These results indicate that neutrophils kill P. aeruginosa by using a mechanism independent of SP-A opsonization, and lend support to the notion that neutrophils play a less critical role in the preferential clearance of pch and ptsP mutants from the SP-A+/+ mice than other anti-pseudomonal mechanisms.

The Loss of pch and ptsP Gene Functions Render P. aeruginosa Susceptible to SP-A-Mediated Membrane Permeabilization

Recent studies have indicated that SP-A is capable of directly killing bacteria and fungi by membrane permeabilization and inhibition of macro-molecular synthesis, independent of macrophage-mediated phagocytosis [6,7]. We examined whether direct membrane permeabilization contributed to the clearance of the SP-A-sensitive mutants. Due to the previously described importance of LPS in resistance to SP-A-mediated membrane permeabilization [6,19], we used a LPS mutant wbpL, which is deficient in the production of “initial” glycosyltransferase essential for the biosynthesis of both the A-band and B-band O-antigen of LPS [20], as positive control for membrane permeabilization assays. Permeabilization of the wbpL mutant was approximately 2.7-fold greater than the wild-type strain PA01 at 60 min (Figure 5A). In contrast, STMG2A7, an irrelevant mutant that is virulent in both SP-A+/+ and SP-A−/− mice, was found to be as resistant as parental wild-type PA01 to SP-A-mediated membrane permeability (Figure 5B).

Figure 5. The pch and ptsP Mutants Are Preferentially Permeabilized and Killed by SP-A

(A) Fluorescence of a cleavage-activated phosphatase substrate ELF97 was examined in the presence or absence of 50 μg hSP-A for a period of 60–90 min. Human SP-A (hSP-A) preferentially permeabilized LPS mutant wbpL, but not the parental wild-type PA01. The wbpL strain was used as positive control for membrane permeability. The difference in membrane permeabilization between wbpL mutant and PA01 was significant from the 28th min onward. *p < 0.05.

(B) A mutant strain STMG2A7 that is virulent in both SP-A+/+ and SP-A−/− mice was as resistant to SP-A-mediated membrane permeabilization as the parental wild-type PA01.

(C–D) Membrane permeability of the STM mutant pch and PA06331, a P. aeruginosa strain which is deleted in all of the structural genes required for pyochelin biosynthesis (Table 1.). The difference in membrane permeabilization between the mutants against wild-type PA01 was significant from the 35th and 18th min onward for mutant strains pch and PA06331, respectively. *p < 0.05.

(E–F) Membrane permeability of the STM mutant ptsP and the ΔptsP, a P. aeruginosa strain with a nonpolar, inframe deletion of the ptsP gene. The difference in membrane permeabilization between the mutants against wild-type PA01 was significant from the 29th and 28th min onward, for mutant strains ptsP and ΔptsP, respectively. *p < 0.05.

The STM mutant pch, and a mutant strain, PA06331, in which the pyochelin biosynthetic genes encompassing pchDCBA, pchR, and pchEFGHI operons had been removed [14], were permeabilized by SP-A to an extent that was 3.4- and 2.55-fold greater than the wild-type strain PA01, respectively (Figure 5C and 5D) after 60–90 min exposure to SP-A. Similarly, STM mutant ptsP, and an in-frame, nonpolar deletion mutant, ΔptsP, were permeabilized by SP-A to an extent that was 3.0- and 3.8-fold greater than the wild-type strain PA01, respectively (Figure 5E and 5F), at 60–90 min post-exposure to SP-A. These data are comparable to the approximately 3-fold increase in membrane permeability that SP-A exposure induces in E. coli K12 [6].

SP-A-Mediated Membrane Permeabilization Directly Kills the pch and ptsP Mutants

We next determined if SP-A mediated permeability kills STM mutants. Live/dead staining, based on exclusion of propidium iodide from the live cells, was performed on bacterial cells following membrane permeability assays. Viable cells are stained green while dead cells are stained red. As shown in Figure 6A, SP-A did not kill wild-type PA01 (green stained). In contrast, mixtures of green- and red-stained cells of pch and ptsP were visible following treatment with SP-A. Approximately 11% and 9 % of pch and ptsP cells, respectively, were killed (Figure 6B) within 60 min, in comparison to about 40% of E. coli K12 (unpublished data). In addition, in contrast to the robust SP-A-induced aggregation of E. coli K12 (Figure 6A), SP-A did not aggregate P. aeruginosa PA01, pch, or ptsP. These results suggest that the loss of intact LPS (i.e. rough LPS), or the inability to synthesize salicylate and phosphoenolpyruvate-protein-phosphotransferase, renders the cells vulnerable to membrane permeabilization and killing by SP-A. Furthermore, bacterial aggregation does not play a role in preferential clearance of the pch and ptsP mutants.

Figure 6. SP-A-Mediated Membrane Permeabilization Directly Kills the pch and ptsP Mutants

(A) Live/Dead staining was performed on E. coli K12, PA01, pch, and ptsP cells, following 1 h membrane permeabilization with 100 μg/ml SP-A. Green-stained cells are alive whereas red-stained cells are dead.

(B) Enumeration of live or dead bacteria following a 1 h exposure to hSP-A. At least 600–1,000 bacterial cells were counted under a fluorescence microscope. The mean of two experiments is shown.

Complementation of the pch and ptsP Mutants Restores Their Resistance to SP-A-Mediated Membrane Permeabilization

The susceptibility of STM mutants to SP-A mediated membrane permeabilization can be exploited for complementation analyses. As the pch mutant is disrupted in a gene required for salicylate biosynthesis, we performed complementation analysis by growing the pch mutant bacteria in the presence of 1 mM sodium salicylate. As shown in Figure 7A, the pch mutant bacteria grown in LB were susceptible to SP-A-mediated membrane permeabilization. In contrast, the pch mutant bacteria grown in LB supplemented with 1 mM sodium salicylate were fully resistant to membrane permeabilization by SP-A. We further examined whether the increased susceptibility to SP-A-mediated membrane permeability was due to the inability pch bacteria to synthesize the siderophore pyochelin. The pch bacteria cultured in pyochelin-supplemented LB or iron-deficient minimal medium were still membrane permeabilized by SP-A (unpublished data). Collectively, these results suggest that the increased susceptibility to SP-A-mediated membrane permeability in the pch bacteria is due to their inability to synthesize salicylate, or both salicylate and pyochelin. However, we cannot completely rule out the possibility that pyochelin may be involved in resistance to SP-A-mediated membrane permeability until we have exhausted all the growth conditions and optimal pyochelin concentrations for the assays.

Figure 7. Complementation Studies of SP-A-Sensitive Mutants pch and ptsP

(A) Culturing pch bacteria in LB supplemented with sodium salicylate restored its resistance to SP-A mediated membrane permeabilization.

(B) In control experiments, we demonstrated that the enzymatic activity of bacterial phosphatases in ptsP bacterial cells was not inhibited by 1 mM sodium salicylate.

(C) Provision of the wild-type ptsP gene on the pUCP19 in trans (pUCP-ptsP) restores the ability of STM mutant ptsP to resist SP-A mediated membrane permeabilization. In contrast, ptsP mutant expressing GFP gene on the pUCP19 (pstP-gfp) is permeabilized to similar levels as ptsP.

To rule out the possibility that 1 mM sodium salicylate may inactivate the enzymatic activity of the periplasmic phosphatases that cleaves the impermeant substrate, ELF97, in our permeability assay, we also tested ptsP mutant bacteria cultured in the presence or absence of 1 mM sodium salicylate. The ptsP mutant bacteria were permeabilized to the same extent, regardless of whether they were grown in the presence or absence of 1 mM sodium salicylate (Figure 7B), suggesting that salicylate did not inactivate phosphatase. These results suggest that the loss of pch gene function results in susceptibility of P. aeruginosa to clearance by SP-A by rendering the organism susceptible to membrane permeabilization.

We next tested if providing the wild-type ptsP gene in trans to the ptsP STM mutant bacteria could restore the resistance to SP-A-mediated membrane permeabilization. As shown in Figure 7C, the resulting strain, pUCP-ptsP was as resistant to SP-A-mediated membrane permeabilization as the wild-type PA01. In contrast, providing an irrelevant gfp gene in the ptsP bacteria (ptsP-gfp) did not restore the resistance of ptsP STM mutant to SP-A, nor did it alter the resistance or susceptibility of the parental wild-type PA01 (PA01-gfp) to permeabilization by SP-A (Figure 7C). These results suggest that ptsP gene function protects P. aeruginosa from membrane permeabilization by SP-A.

LPS Profiles of STM Mutants

Previous studies in E. coli [6] and Bordetella pertussis [19] have demonstrated that the structures of LPS on the surface of bacterial cells determine resistance to SP-A-mediated aggregation and membrane permeabilization. P. aeruginosa LPS mutants are also sensitive to SP-A-mediated membrane permeability, but are not aggregated by the collectin (Figure 5A; unpublished data). To examine if the pch and ptsp mutants have LPS defects, we compared the LPS profiles after separation by SDS-PAGE and silver staining. The LPS from wild-type PA01 and the pch mutant were indistinguishable (unpublished data). However, the two major LPS core bands of the ptsP mutant showed a reversal in relative abundance compared with the PA01 (unpublished data). Thus, there may be changes in LPS, at least in terms of the proportion of two different cores made. More detailed molecular analyses will be required to determine if LPS modification occurs within pch and ptsP mutants.


The genome-wide mutagenesis scheme called STM was originally developed to identify novel vaccine and antibiotic targets [9]. STM relies on the ability of the pathogen in question to replicate in vivo as a mixed population, and allows the identification of the virulence genes whose mutant phenotypes cannot be trans-complemented by other virulent strains present in the same inoculum. Hundreds of virulence factors and putative drug targets have been identified by STM in at least 20 different bacterial and fungal pathogens [21]. In all of these screens, a pathogen of interest is mutated by transposon or suicide vector-based insertional strategies. The vectors are each individually tagged with a DNA oligonucleotide to allow mutant identification after selection within the host. Attenuated insertion mutants that are killed by host defense mechanisms such as exposure to SP-A, will fail to amplify from lung homogenates harvested 16 h after intratracheal inoculation (Figure 2A). Comparative STM screening using wild-type and genetically altered mice, as presented herein, represents a novel application of the STM technique. This approach allows the identification of bacterial determinants targeted by specific components of host defense, rather than the entire immune system as a whole. Thus, in contrast to conventional STM screens in wild-type mice, which yield an attenuated mutant recovery rate of 2%–10% [21], our comparative STM screen to identify factors that protect bacteria against a specific host innate immunity protein, SP-A, had a yield of only 0.12%. As STM screens, by definition, only recover mutations in non-essential genes, another reason for detecting few mutants in this screen is that these genes involved in resistance to SP-A may be essential.

In this study, we have employed STM technology to identify bacterial factors that are required for P. aeruginosa strain PA01 to confer resistance to SP-A. Both mutants were susceptible to SP-A-mediated membrane permeabilization, confirming that disruption of membrane integrity is one of the mechanisms by which SP-A mediates bacterial clearance. The degree of bacterial membrane permeabilization of the STM mutants by SP-A was comparable to that of E. coli K12, which has rough LPS [6]. Based on the results of in vitro assays, macrophages and neutrophils do not seem to play important roles in preferential clearance of the pch and ptsP mutants. However, we cannot exclude the possibility that phagocytosis contributes to the differential clearance of these two mutants in vivo.

Thus far, we have not recovered STM mutants that are susceptible to SP-A-mediated opsonization, or mutants that are disrupted in the genes required for LPS biosynthesis, which play critical roles in resistance to SP-A-mediated membrane permeability. The lack of recovery of opsonization-sensitive and LPS mutants are not particularly surprising, considering that we screened only approximately 30% of the 5,570 mutants required for 1 × genome coverage ( Additional screenings are being carried out to catalog other P. aeruginosa factors conferring resistance to SP-A.

The mechanisms by which mutations in pch and ptsP genes result in susceptibility to SP-A-mediated clearance are briefly discussed below. The pchDCBA gene encodes enzymes involved in the synthesis of iron-chelating siderophores salicylate and pyochelin [1214]. In another closely related pathogen, Burkholderia cepacia, salicylate is a major siderophore [22]. Salicylate has also been reported to chelate magnesium (Mg2+) and calcium [23]. Thus, it is possible that P. aeruginosa requires salicylate and its downstream product pyochelin to acquire cations. Divalent cations, especially Mg2+, are required to structurally stabilize LPS on the outer membrane. The recently resolved structure of SP-A protein indicates that there are two metal binding domains within SP-A, which are most likely occupied by calcium [24]. Thus, SP-A may sequester cations from alveolar lining fluid and result in a growth disadvantage for the salicylate-deficient pch mutant. Furthermore, inability to acquire cations may potentially alter the expression, stability, and modification of various transmembrane proteins and glycolipids by enzymes that require cations as cofactors. Thus, we speculate that the pch mutation may have contributed to its increased sensitivity to SP-A-mediated membrane permeabilization through direct or indirect effects on LPS integrity and membrane stability.

The ptsP gene encodes phosphoenolpyruvate-protein phosphotransferase EINtr [15], a transcriptional regulator of RpoN-dependent operons [25]. RpoN is known to regulate the expression of variety of virulence factors in pathogenic bacteria, including the upregulation of the rfaH gene, which is required for increased production of the O-antigen of LPS in Salmonella enterica serovar Typhi during the stationary phase of growth [25]. The additional O-antigen production during the stationary phase of bacterial growth may be necessary for resistance to SP-A-mediated membrane permeabilization. PtsP also coordinates carbon and nitrogen metabolism and is required for virulence in P. aeruginosa, by an unknown mechanism [26]. Mutational inactivation of the Azotobacter vinelandii ptsP ortholog affects lipidic poly-hydroxybutyrate accumulation within its cytoplasm as a carbon source for long-term starvation survival [27]. Interestingly, poly-hydroxybutyrate is found in the plasma membranes of E. coli complexed to calcium polyphosphate, and forms divalent cation-selective channels [28]. Thus, increased sensitivity to SP-A-mediated membrane permeabilization in ptsP mutants may be caused by its reduced ability to transport divalent cations necessary to maintain LPS and outer membrane integrity.

Our results suggest that the killing of P. aeruginosa PA01 and STM mutants is more robust in vivo than in vitro. One potential explanation for this discrepancy is that our in vitro membrane permeability conditions do not accurately model the environment in the lung. In addition, it is possible that multiple factors contribute to the killing of P. aeruginosa including SP-A, SP-D, lactoferrin, β-defensins, and other antimicrobial peptides and proteins [29,30]. We are currently examining whether these peptides act synergistically or cooperatively with SP-A in clearance of P. aeruginosa.

Decreased SP-A levels have been found in several respiratory diseases including bacterial pneumonia, adult respiratory distress syndrome [31,32], and cystic fibrosis [3335]. There is some in vitro evidence to suggest that decreased SP-A and SP-D levels in some of these disease states result from degradation by neutrophil proteases of the host [36,37], or by proteases of bacterial origin [38]. These proteases include bacterial elastases, and neutrophil-derived cathepsin G, elastase, and proteinase-3. The reduced levels of SP-A and SP-D in these lung diseases may contribute to increased susceptibility to infections by variety of microbial pathogens. Degradation of SP-A by P. aeruginosa proteases may also explain our failure to develop informative in vitro STM screens (unpublished data).

Antibiotic-resistant P. aeruginosa is an emerging clinical problem that can lead to denial for lung transplantation and death [39]. Thus, there is an added urgency to explore the use of novel, non-antibiotic-based, anti-Pseudomonal peptides to combat life-threatening infections with this organism. The discovery of factors governing resistance or susceptibility to SP-A may ultimately have therapeutic value.

Materials and Methods

Bacterial strains, media, and growth conditions.

Shaking cultures of E. coli DH5-α [40], SM17λpir [41], and P. aeruginosa strain PA01 [42] were grown in LB broth at 37 °C. When needed, LB was supplemented with 1.5% of bacto agar. Antibiotic selections were performed for E. coli or P. aeruginosa using the following concentrations: carbenicillin (50 or 300 μg/ml), kanamycin (50 or 250 μg/ml), and tetracycline (5 or 15–30 μg/ml).

Animal husbandry.

The C3H/HeN SP-A−/− mice were developed as previously described [6,7]. C3H/HeN control (SP-A+/+) mice were purchased from Charles River Laboratory (Boston, Massachusetts, United States). All infections were performed intranasally with age-matched, 6-wk-old mice. Animals were housed in positively ventilated microisolator cages with automatic recirculating water, located in a room with laminar, high-efficiency, particle accumulation-filtered air. The animals received autoclaved food, water, and bedding. Mice used in experimental procedures were handled in accordance with protocols approved by the Institutional Animal Care and Use Committee at University of Cincinnati College of Medicine.

Comparative screening of the P. aeruginosa STM library in SP-A+/+ and SP-A−/− mice.

The P. aeruginosa PA01 STM library and screening methods were previously described [11]. An adapted acute mouse lung pneumonia model of infection was employed, where adult mice rather than the infant mice were used [16]. In earlier experiments, we detected no significant difference in SP-A expression by ELISA assays at 8, 16, and 24 h in SP-A+/+ mouse lungs infected with bacteria (1 × 107 cells) from a representative pool of STM library (unpublished data). We chose the 16 h time point to screen the STM library because it gave us the most reproducible PCR amplification of DNA tags from mutants, with ≥ 10,000 colony forming units (CFU) still recoverable from the SP-A+/+ mice (unpublished data). In contrast, prolonged infection (≥ 36 h) with 1 × 107 bacteria from STM pool frequently killed SP-A−/− mice (unpublished data). Briefly, SP-A+/+ and SP-A−/− mice [6,7] were anaesthetized using isofluorane, and were intranasally inoculated with 50 μl (1 × 107 cells) of each individual STM pool. After 16 h, lungs were removed from sacrificed mice, and homogenized tissues were plated on LB agar plates. At least 10,000 bacterial colonies recovered after in vivo selection were used for multiplex PCR as described previously [11]. Twenty sets of 72 mutants (total = 1,440) were pooled and screened. An additional 240 mutants previously shown to be attenuated in a chronic model of rat lung infection [11] were also screened. The mutants that were differentially cleared by SP-A during the in vivo passaging were subsequently retested by single PCR in bacterial cells recovered from three separate mice.

In vivo competitive and single infection assays.

For competition assays, mouse lungs were inoculated intranasally with bacterial cells (1 × 107 in 50 μl) composed of a 1:1 ratio of wild-type PA01 and its isogenic STM mutants. Infected lungs were recovered 16 h after infection for bacterial load determination. The competitive index (CI) is defined as the output ratio of mutant to wild-type bacteria divided by the input ratio of mutant to wild-type bacteria [16,17]. Thus, if a mutant strain is less competitive than the parental strain from which it was derived, a CI value of < 1 will be achieved, indicating that the mutant is attenuated. Single organism inoculations with individual bacterial strains were performed by the intranasal route in SP-A+/+ and SP-A−/− mice (group of six). Attenuation was defined as the log10 difference in CFU between wild-type and mutant bacteria recovered from lung tissue 16 h after inoculation.

Mutant cloning and bioinformatics analysis.

Cloning of putative STM mutants were performed as previously described [11]. The DNA sequences were analyzed with MacVector or DNA Star software. Sequence data was compared with the database available for P. aeruginosa at

Non-polar deletion and complementation of the ptsP mutant.

Non-polar, in-frame deletion of ptsP was generated by PCR: 0.802 and 1.155-kb 5′ and 3′ segments were amplified from target PA01 genomic DNA, and each amplicon, which included an engineered restriction site, was ligated into pEX18Ap [43] to produce replacement plasmids. Inframe deletion mutants were generated in PA01 via homologous recombination by sucrose resistance selection, and confirmed by hybridization and PCR analysis (unpublished data). To complement the ptsP mutation, a 4.5-kb DNA fragment containing both the promoter and the ygdP-ptsP-PA0338 operon (Figure 2C) was PCR-amplified from the wild-type parental strain PA01 using the Expand Long Template PCR System (Roche Diagnostic, Basel, Switzerland), and cloned into E. coli-P. aeruginosa shuttle plasmid pUCP19 [44] to obtain pUCP19-ptsP. The cloned fragment was sequenced to rule out any mutation that was introduced during the amplification. The pUCP19-ptsP was introduced into P. aeruginosa STM mutant strain ptsP by heat shock. Carbenicillin-resistant transformants were selected, and verified by Southern hybridization and PCR methods (unpublished data). Complementation was assessed by resistance to SP-A-mediated membrane permeabilization.

Complementation of the pch STM mutant.

Complementation of the pch mutant was performed by culturing the bacteria into stationary phase in LB supplemented with 1 mM sodium salicylate.

Pyochelin extraction and detection.

Pyochelin production in P. aeruginosa was analyzed using the method previously described [45]. M63 minimal medium (5 ml) was inoculated with fresh colonies of individual P. aeruginosa strains and incubated at 37 °C for 24 h with shaking. A fresh 30 ml of M63 supplemented with 0.5% w/v casamino acids was then inoculated with 0.3 ml of starter culture, and incubated for 36 h at 37 °C with shaking. The culture was then centrifuged at 13,000 rpm for 10 min in 1.5 ml aliquots in a microcentrifuge. The supernatants were removed into a 50 ml polypropylene screw-capped centrifuge tube, pooled, adjusted to (pH 2.0) with 1M HCl, using universal indicator paper to estimate pH, and filter sterilized through a 0.22 μM membrane. Pyochelin was extracted by the addition of 0.4 volumes of ethyl acetate, followed by vigorous vortexing. The two phases were separated by centrifugation at 2,000 rpm for 5 min in a bench top centrifuge, and the upper, organic phase was removed to a separate tube. Pyochelin extract was concentrated by rotary evaporation at 40 °C in 100 ml round bottomed flasks, and the residue was dissolved in 300 μl of methanol. Pyochelin extracts (10 μl) was separated by TLC (silica gel 60, plastic backed, from Sigma, St. Louis, Missouri, United States), using acetone:methanol:0.2M acetic acid (5:2:1) as a development solvent. The chromatography tank was left to stand for several minutes with its lid on to allow the air inside to become saturated with solvent vapor. Pyochelin, which is fluorescent, naturally occurs as two stereoisomers. When visualized under a UV transilluminator, it is revealed as two green fluorescent bands. Pyochelin standard was generously provided by Dr. J. M. Meyer (Université Louis Pasteur).

Purification of human SP-A.

Human SP-A (hSP-A) was purified from lung washings of patients with the lung disease alveolar proteinosis, as previously described [6]. SP-A preparations were re-suspended in 5 mM Tris, 150 mM NaCl. SP-A preparations were determined to contain 140–190 pg of LPS/μg of SP-A by the Limulus Amebocyte Lysate (BioWhittaker, Rockland, Maryland, United States).

Assays of P. aeruginosa permeability.

The effect of the SP-A on P. aeruginosa cell wall integrity was assessed by determining permeability to a phosphatase activity substrate, Enzyme-Labeled Fluorescence 97 (ELF-97, Molecular Probes, Eugene, Oregon, United States) as described [7]. SP-A was incubated with 1 × 108 bacterial cells/ml in 100 μl of 5 mM Tris, 150 mM NaCl for 15 min at 37 °C, and 100 μM ELF97 phosphatase substrate was added. Fluorescence was measured at excitation and emission wavelengths of 355 and 535 nm, respectively, for a period of 60–90 min.

In vitro macrophage and neutrophil phagocytosis assays.

Freshly lavaged mouse macrophages (~ 5 × 105 from 3 SPA+/+ mice) were cultured on chamber plastic culture slides, coated with 5% poly-D-lysine with 200 μl RPMI (Dulbecco's, containing 2.5 mg/L gentamycin and 0.1% BSA) and used immediately. Macrophages were allowed to adhere for 2 h at 37 °C in 5% CO2. Live GFP-expressing PA01 or isogenic STM mutants in RPMI were opsonized with or without 25 μg/ml human SP-A for 1 h at 37 °C with rotation. The medium was removed from each well and replaced with 250 μl of opsonized PA01 or STM mutants, and incubated for 1 h at 37 °C in 5% CO2 at a ratio of 100 bacteria to 1 macrophage. Chamber slides were washed three times with PBS containing 1 mM CaCl2. Extracellular bacteria were quenched with crystal violet (0.8 mg/ml). Following two additional washes, cells were fixed with 1% paraformaldehyde in PBS plus 1 mM CaCl2 for 10 min, and stained with Evans blue for 2 min. The percentage of macrophages with engulfed bacteria was quantified under a phase contrast fluorescence microscope. At least 200 macrophages were counted. Human neutrophils were purified and cultured as previously described [46]. Neutrophil phagocytosis was performed as described for macrophages.

LIVE/DEAD bacterial staining.

The viability of SP-A exposed bacteria was determined by LIVE/DEAD BaclightTM Bacterial Viability Kit (Molecular Probes). Briefly, stationary phase E. coli or P. aeruginosa bacteria were washed three times with 5 mM Tris, 150 mM NaCl, and adjusted to an of OD600 = 1.0. A 100-μl aliquot of the cells was added to culture tubes containing 100 μl of SP-A (100 μg/ml) or 100 μl of 5 mM Tris, 150 mM NaCl, as a control. The mixtures were incubated at 37 °C, 300 rpm for 1 h, and stained according to the instructions provided by the supplier. The viability of the cells was checked under a fluorescence microscope. At least 1, 000 cells were counted.

LPS preparations.

LPS was isolated from P. aeruginosa by acetone/phenol extraction [47]. LPS samples were size-fractionated on 4%–12% Bis-Tris PAGE gels (NuPAGE Novex Gels; Invitrogen, San Diego, California, United States) and stained with silver.

Statistical analysis.

Statistical analysis was performed using the Student's t-test and one-way analyses of variance (ANOVA). A significant difference was considered to be p < 0.05.


This work was supported by grants from the NIH (1R03AI057915), an American Lung Association research grant (RG-131-N), and a University of Cincinnati College of Medicine Dean Discovery Fund to GWL; and the NIH (HL-61612) and the Department of Veterans Affairs (Merit Award) to FXM. Work on STM in R. C. Levesque's laboratory is funded by the Canadian Institute for Health Research as part of the CIHR Genomics Program. R. C. Levesque is also funded by a Research Scholar of Exceptional Merit from Le Fonds de la Recherche en Santé du Québec. E. Potvin obtained a studentship from CIHR. We thank Drs. Jeff Whitsett and Tom Korfhagen for the gift of Swiss Black SP-A−/−mice. We thank Dr. C. Reimmann for the gifts of the PA06331 and pyochelin purification methods, Dr. J.M. Meyer (Laboratoire de Microbiologie et Génétique, Université Louis Pasteur) for her generous supply of purified pyochelin, and Dr. Herbert Budzikiewicz (Institut fuer Organische Chemie, Koeln) for his generous advice on pyochelin TLC and purification.

Author Contributions

SZ, YC, FXM, and GWL conceived and designed the experiments. SZ, YC, FS, and GWL performed the experiments. SZ, YC, FS, FXM, and GWL analyzed the data. EP, FS, RCL, FXM, and GWL contributed reagents/materials/analysis tools. GWL wrote the paper.


  1. 1. McCormack FX, Whitsett JA (2002) The pulmonary collectins, SP-A and SP-D, orchestrate innate immunity in the lung. J Clin Invest 109: 707–712.
  2. 2. Wright JR (2003) Pulmonary surfactant: A front line of lung host defense. J Clin Invest 111: 1453–1455.
  3. 3. Crouch E, Wright JR (2001) Surfactant proteins A and D and pulmonary host defense. Annu Rev Physiol 63: 521–554.
  4. 4. LeVine AM, Whitsett JA (2001) Pulmonary collectins and innate host defense of the lung. Microbes Infect 3: 161–166.
  5. 5. Kuhlman M, Joiner K, Ezekowitz RA (1989) The human mannose-binding protein functions as an opsonin. J Exp Med 169: 1733–1745.
  6. 6. Wu H, Kuzmenko A, Wan S, Schaffer L, Weiss A, et al. (2003) Surfactant proteins A and D inhibit the growth of Gram-negative bacteria by increasing membrane permeability. J Clin Invest 111: 1589–1602.
  7. 7. McCormack FX, Gibbons R, Ward SR, Kuzmenko A, Wu H, et al. (2003) Macrophage-independent fungicidal action of the pulmonary collectins. J Biol Chem 278: 36250–36256.
  8. 8. Piboonpocanun S, Chiba H, Mitsuzawa H, Martin W, Murphy RC, et al. (2005) Surfactant protein A binds Mycoplasma pneumoniae with high affinity and attenuates its growth by recognition of disaturated phosphatidylglycerols. J Biol Chem 280: 9–17.
  9. 9. Hensel M, Shea JE, Gleeson C, Jones MD, Dalton E, et al. (1995) Simultaneous identification of bacterial virulence genes by negative selection. Science 269: 400–403.
  10. 10. LeVine AM, Kurak KE, Bruno MD, Stark JM, Whitsett JA, et al. (1998) Surfactant protein-A-deficient mice are susceptible to Pseudomonas aeruginosa infection. Am J Respir Cell Mol Biol 19: 700–708.
  11. 11. Potvin E, Lehoux D, Kukavica-Ibrujl I, Richard K, Sanschagrin F, et al. (2003) In vivo functional genomics of Pseudomonas aeruginosa for high-throughput screening of new virulence factors and antibacterial targets. Environ Microbiol 5: 1294–1308.
  12. 12. Gaille C, Reimann C, Haas D (2003) Isochorismate synthase (PchA), the first and rate-limiting enzyme in salicylate biosynthesis of Pseudomonas aeruginosa. J Biol Chem 278: 16893–16898.
  13. 13. Cox CD, Rinehart KL Jr, Moore ML, Cook JC Jr (1981) Pyochelin: Novel structure of an iron-chelating growth promoter for Pseudomonas aeruginosa. Proc Natl Acad Sci USA 78: 4256–4260.
  14. 14. Reimmann C, Patel HM, Serino L, Barone M, Walsh CT, et al. (2001) Essential PchG-dependent reduction in pyochelin biosynthesis of Pseudomonas aeruginosa. J Bacteriol 183: 813–820.
  15. 15. Reizer J, Reizer A, Merrick MJ, Plunkett G 3rd, Rose DJ, et al. (1996) Novel phosphotransferase-encoding genes revealed by analysis of the Escherichia coli genome: A chimeric gene encoding an Enzyme I homologue that possesses a putative sensory transduction domain. Gene 181: 103–108.
  16. 16. Lau GW, Ran H, Kong F, Hassett DJ, Mavrodi D (2004) Pseudomonas aeruginosa pyocyanin is critical for lung infection in mice. Infect Immun 72: 4275–4278.
  17. 17. Chiang SL, Mekalanos JJ (1998) Use of signature-tagged transposon mutagenesis to identify Vibrio cholerae genes critical for colonization. Mol Microbiol 27: 797–805.
  18. 18. Mariencheck WI, Savov J, Dong Q, Tino MJ, Wright JR (1999) Surfactant protein A enhances alveolar macrophage phagocytosis of a live, mucoid strain of P. aeruginosa. Am J Physiol 277: 777–786.
  19. 19. Schaeffer LM, McCormack FX, Wu H, Weiss AA (2004) Bordetella pertussis lipopolysaccharide resists the bactericidal effects of pulmonary surfactant protein A. J Immunol 173: 1959–1965.
  20. 20. Rocchetta HL, Burrows LL, Lam JS (1999) Genetics of O-antigen biosynthesis in Pseudomonas aeruginosa. Microbiol Mol Biol Rev 63: 523–553.
  21. 21. Mecsas J (2002) Use of signature-tagged mutagenesis in pathogenesis studies. Curr Opin Microbiol 5: 33–37.
  22. 22. Nair BM, Cheung KJ Jr, Griffith A, Burns JL (2004) Salicylate induces an antibiotic efflux pump in Burkholderia cepacia complex genomovar III (B. cenocepacia). J Clin Invest 113: 464–473.
  23. 23. Domenico P, Schwartz S, Cunha BA (1989) Reduction of capsular polysaccharide production in Klebsiella pneumoniae by sodium salicylate. Infect Immun 57: 3778–3782.
  24. 24. Head JF, Mealy TR, McCormack FX, Seaton BA (2003) Crystal structure of trimeric carbohydrate recognition and neck domains of surfactant protein A. J Biol Chem 278: 43254–43260.
  25. 25. Bittner M, Saldias S, Altamirano F, Valvano MA, Contreras I (2004) RpoS and RpoN are involved in the growth-dependent regulation of rfaH transcription and O antigen expression in Salmonella enterica serovar Typhi. Microb Pathog 36: 19–24.
  26. 26. Tan MW, Mahajan-Miklos S, Ausubel FM (1999) Killing of Caenorhabditis elegans by Pseudomonas aeruginosa used to model mammalian bacterial pathogenesis. Proc Natl Acad Sci USA 96: 715–720.
  27. 27. Segura D, Espin G (1998) Mutational inactivation of a gene homologous to Escherichia coli ptsP affects poly-hydroxybutyrate accumulation and nitrogen fixation in Azotobacter vinelandii. J Bacteriol 180: 4790–4798.
  28. 28. Reusch RN (1999) Polyphosphate/poly-(R)-3-hydroxybutyrate ion channels in cell membranes. Prog Mol Subcell Biol 23: 151–182.
  29. 29. Singh PK, Tack BF, McCray PB Jr, Welsh MJ (2000) Synergistic and additive killing by antimicrobial factors found in human airway surface liquid. Am J Physiol Lung Cell Mol Physiol 279: 799–805.
  30. 30. Yan H, Hancock RE (2001) Synergistic interactions between mammalian antimicrobial defense peptides. Antimicrob Agents Chemother 45: 1558–1560.
  31. 31. Baughman RP, Sternberg RI, Hull W, Buchsbaum JA, Whitsett J (1993) Decreased surfactant protein A in patients with bacterial pneumonia. Am Rev Respir Dis 147: 653–657.
  32. 32. LeVine AM, Lotze A, Stanley S, Stroud C, O'Donnell R, et al. (1996) Surfactant content in children with inflammatory lung disease. Crit Care Med 24: 1062–1067.
  33. 33. Griese M, Birrer P, Demirsoy A (1997) Pulmonary surfactant in cystic fibrosis. Eur Respir J 10: 1983–1988.
  34. 34. Postle AD, Mander A, Reid KB, Wang JY, Wright SM, et al. (1999) Deficient hydrophilic lung surfactant proteins A and D with normal surfactant phospholipid molecular species in cystic fibrosis. Am J Respir Cell Mol Biol 20: 90–98.
  35. 35. Noah TL, Murphy PC, Alink JJ, Leigh MW, Hull WM, et al. (2003) Bronchoalveolar lavage fluid surfactant protein-A and surfactant protein-D are inversely related to inflammation in early cystic fibrosis. Am J Respir Crit Care Med 168: 685–691.
  36. 36. von Bredow C, Wiesener A, Griese M (2003) Proteolysis of surfactant protein D by cystic fibrosis relevant proteases. Lung 181: 79–88.
  37. 37. Rubio F, Cooley J, Accurso FJ, Remold-O'Donnell E (2004) Linkage of neutrophil serine proteases and decreased surfactant protein-A (SP-A) levels in inflammatory lung disease. Thorax 59: 318–323.
  38. 38. Mariencheck WI, Alcorn JF, Palmer SM, Wright JR (2003) Pseudomonas aeruginosa elastase degrades surfactant proteins A and D. Am J Respir Cell Mol Biol 28: 528–537.
  39. 39. Conway SP, Brownlee KG, Denton M, Peckham DG (2003) Antibiotic treatment of multidrug-resistant organisms in cystic fibrosis. Am J Respir Med 2: 321–332.
  40. 40. Miller VL, Mekalanos JJ (1988) A novel suicide vector and its use in construction of insertion mutations: Osmoregulation of outer membrane proteins and virulence determinants in Vibrio cholerae requires toxR. J Bacteriol 170: 2575–2583.
  41. 41. Taylor RK, Manoil C, Mekalanos JJ (1989) Broad-host range vectors for delivery of TnphoA: Use in genetic analysis of secreted virulence determinants of Vibrio cholerae. J Bacteriol 171: 1870–1878.
  42. 42. Holloway BW, Krishnapillai V, Morgan AF (1979) Chromosomal genetics of Pseudomonas. Microbiol Rev 43: 73–102.
  43. 43. Hoang TT, Karkhoff-Schweizer RR, Kutchma AJ, Schweizer HP (1998) A broad-host-range Flp-FRT recombination system for site-specific excision of chromosomally-located DNA sequences: Application for isolation of unmarked Pseudomonas aeruginosa mutants. Gene 212: 77–86.
  44. 44. Schweizer HP (1991) Escherichia-Pseudomonas shuttle vectors derived from pUC18/19. Gene 97: 109–121.
  45. 45. Serino L, Reimmann C, Baur H, Beyeler M, Visca P, et al. (1995) Structural genes for salicylate biosynthesis from chorismate in Pseudomonas aeruginosa. Mol Gen Genet 249: 217–228.
  46. 46. Newman SL, Gootee L, Gabay JE (1993) Human neutrophil-mediated fungistasis against Histoplasma capsulatum. Localization of fungistatic activity to the azurophil granules. J Clin Invest 92: 624–631.
  47. 47. Westphal O, Jann K (1965) Methods in carbohydrate chemistry. New York: Academic Press. pp. 83–91. Volume 5,.