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Infect Immun. 2017 April; 85(4): e00897-16.
Published online 2017 March 23. Prepublished online 2017 January 30. doi:  10.1128/IAI.00897-16
PMCID: PMC5364298

The Type II Secretion System of Legionella pneumophila Dampens the MyD88 and Toll-Like Receptor 2 Signaling Pathway in Infected Human Macrophages

Craig R. Roy, Editor
Craig R. Roy, Yale University School of Medicine;

ABSTRACT

Previously, we reported that mutants of Legionella pneumophila lacking a type II secretion (T2S) system elicit higher levels of cytokines (e.g., interleukin-6 [IL-6]) following infection of U937 cells, a human macrophage-like cell line. We now show that this effect of T2S is also manifest upon infection of human THP-1 macrophages and peripheral blood monocytes but does not occur during infection of murine macrophages. Supporting the hypothesis that T2S acts to dampen the triggering of an innate immune response, we observed that the mitogen-activated protein kinase (MAPK) and nuclear transcription factor kappa B (NF-κB) pathways are more highly stimulated upon infection with the T2S mutant than upon infection with the wild type. By using short hairpin RNA to deplete proteins involved in specific pathogen-associated molecular pattern (PAMP) recognition pathways, we determined that the dampening effect of the T2S system was not dependent on nucleotide binding oligomerization domain (NOD)-like receptors (NLRs), retinoic acid-inducible protein I (RIG-I)-like receptors (RLRs), double-stranded RNA (dsRNA)-dependent protein kinase receptor (PKR), or TIR domain-containing adaptor inducing interferon beta (TRIF) signaling or an apoptosis-associated speck-like protein containing a CARD (ASC)- or caspase-4-dependent inflammasome. However, the dampening effect of T2S on IL-6 production was significantly reduced upon gene knockdown of myeloid differentiation primary response 88 (MyD88), TANK binding kinase 1 (TBK1), or Toll-like receptor 2 (TLR2). These data indicate that the L. pneumophila T2S system dampens the signaling of the TLR2 pathway in infected human macrophages. We also document the importance of PKR, TRIF, and TBK1 in cytokine secretion during L. pneumophila infection of macrophages.

KEYWORDS: Legionella pneumophila, TLR2, cytokine, innate immunity, macrophage, type II secretion

INTRODUCTION

Legionella pneumophila, a Gram-negative bacterium that is widespread in aquatic habitats, is the principal agent of Legionnaires' disease pneumonia (1,6). In the lungs, Legionella bacteria invade and grow in resident macrophages and then trigger severe inflammation (2). In macrophages, L. pneumophila evades the degradative lysosomal pathway and replicates to large numbers within a membrane-bound vacuole, the Legionella-containing vacuole (LCV) (7, 8). Two protein secretion systems, Lsp type II secretion (T2S) and Dot/Icm type IV secretion (T4S), play major roles in the pathogenesis of L. pneumophila (9, 10). In T2S, protein substrates are first translocated across the inner membrane, and upon the action of the T2S pilus-like apparatus, they then exit the bacterial cell through a specific outer membrane pore (11). Using proteomics and enzymatic assays, we have shown that the T2S system of L. pneumophila secretes >25 proteins, including 18 confirmed enzymes and novel proteins, which, in some instances, appear to be unique to Legionella (12, 13). In the aquatic environment, T2S promotes L. pneumophila survival at low temperatures and is critical for infection of at least four genera of amoebae (13,15). In mammalian hosts, T2S contributes to both intracellular infection of macrophages and the destruction of lung tissue. L. pneumophila lsp mutants that lack T2S have an ~10-fold reduction in intracellular growth in both U937 cells, a human macrophage-like cell line, and murine macrophages obtained from A/J mice (16,18). Data from our laboratory have also shown that this reduction in CFU is not due to an entry defect or increased degradation through the phagosome-lysosome pathway but is instead due to a replication defect in LCVs at 4 to 12 h postentry (19).

During intracellular infection of macrophages, L. pneumophila triggers the production of cytokines (20). As is often the case with bacterial infections, this process is initiated in part by the recognition of pathogen-associated molecular patterns (PAMPs) by host surface or endosomal Toll-like receptors (TLRs), cytosolic nucleotide binding oligomerization domain (NOD)-like receptors (NLRs), retinoic acid-inducible protein I (RIG-I)-like receptors (RLRs), and inflammasomes (21,23). Upon PAMP recognition, signal transduction events activate the nuclear factor kappa B (NF-κB) and mitogen-activated protein kinase (MAPK) pathways, causing the transcriptional activators NF-κB and activator protein 1 (AP-1) to induce cytokine gene transcription (23). For the most part, the pathways with which L. pneumophila interacts upon infection were discovered through studies in mice, using either infection of mice lacking the relevant innate immune pathway or in vitro infections of bone marrow-derived (BMD) macrophages obtained from these knockout mice (22, 24). However, a difference in the interactions of L. pneumophila with the innate immune system in human cells versus murine cells, i.e., the role of NAIP5 in restricting L. pneumophila growth in murine cells but not in human cells, has been reported (25, 26).

Interestingly, human U937 macrophages infected with L. pneumophila lsp mutants that lack T2S (but not a complemented lsp mutant) produce higher levels of cytokines than do U937 cells infected with the wild-type (WT) strain (16). We also observed that lsp mutant-infected macrophages contain elevated levels of cytokine (e.g., interleukin-6 [IL-6]) mRNAs (16). The increase in the levels of cytokines seen with the T2S mutant was not a result of there being modestly fewer CFU in the mutant monolayers, since fewer CFU, whether of the WT or the lsp mutant, result in lower, not higher, cytokine levels. Also, when a nonreplicating dotA T4S mutant, which is delivered to the degradative lysosomal pathway, was examined, lower, rather than higher, levels of cytokines were seen (16). Finally, as noted above, the lspF mutant is not trafficked to the phagolysosome in either human or murine macrophages (19). Based on these data, we posited that L. pneumophila T2S dampens host signal transduction and cytokine gene transcription. Here, we show, among other things, that T2S limits signaling through the MyD88-TLR2 pathway, affecting both NF-κB and MAPK activation. Interestingly, the dampening effect of T2S was not observed in murine macrophages, indicating that PAMP recognition is more distinct between human and mice than previously reported.

RESULTS

T2S dampens the cytokine response of multiple types of human macrophages but not murine macrophages.

We previously demonstrated that L. pneumophila T2S mutants triggered more cytokine production following infection of U937 cells than did the parental WT strain 130b (16). To validate these results, we assessed the effect of T2S on IL-6 production by the human macrophage-like cell line THP-1 as well as peripheral blood mononuclear cells (PBMCs) obtained from human volunteers. As is the case for U937 cells, THP-1 cells and PBMCs are widely utilized for studying the interaction between L. pneumophila and macrophages (27,31). For both of these host cells, infection with an lspF mutant that lacks T2S resulted in levels of IL-6 that were significantly higher than those obtained following infection with WT strain 130b (Fig. 1A and andB).B). Furthermore, the magnitudes of the effect of T2S were comparable across the macrophage types, ranging from ~3-fold for THP1 cells and PBMCs to ~5-fold for U937 cells (Fig. 1C). As we previously observed when infecting U937 cells (16, 18), the T2S mutant displayed modestly impaired growth in THP-1 cells and PBMCs (see Fig. S1 in the supplemental material). However, the increases in cytokine levels observed after infection with the lspF mutant were unlikely to have been a manifestation of there being fewer CFU in the monolayer, since fewer legionellae typically result in lower, not higher, cytokine levels (16). Taken together, these data suggested that the T2S system of L. pneumophila is able to dampen the cytokine output of multiple types of human macrophage-like cells.

FIG 1
IL-6 output from various types of macrophages infected with L. pneumophila WT and T2S mutant strains. (A to D) THP-1 cells (A), PBMCs (B), U937 cells (C), and A/J BMD macrophages (D) were either not infected or infected with WT strain 130b or lspF mutant ...

To determine if the influence of T2S on cytokine production extends beyond human cell types, we performed infection assays using BMD macrophages obtained from A/J mice. Interestingly, infection with the mutant lacking T2S resulted in less, not more, IL-6 in murine macrophages (Fig. 1D). Thus, the dampening effect of L. pneumophila T2S on cytokine expression is not manifest in all species' macrophages and may be specific to human host cells.

Since all of our assessments of secreted cytokines had been done at 24, 48, or 72 h postinoculation (Fig. 1A to toC)C) (16), we tested whether the dampening effect of T2S can be detected early in the intracellular infection process. To this end, we amplified the number of infected macrophages by increasing the dose of inoculating bacteria such that the ratio of legionellae to host cells was 10 rather than 0.5. Since U937 cells gave the most robust IL-6 response overall (compare Fig. 1C to toAA and andB),B), we did this experiment, as well as subsequent ones, utilizing this macrophage type. When the supernatants of infected U937 cells were then sampled at 4 h postinoculation, we again observed significantly more IL-6 expression following infection with the lspF mutant than following infection with WT strain 130b (Fig. 1E). These data suggested that the dampening effect of T2S on the cytokine response begins during the initial rounds of infection within the macrophage monolayer.

The differences in cytokine levels that we observed could be explained by either a natural dampening of the macrophage's innate immune response by the T2S system of WT bacteria or an artificial hyperactivation of innate immunity by the lspF mutant as a result of possible increased lysis. The finding that the higher cytokine levels associated with mutant strains are not evident in all species of macrophages suggested that they are not an unspecific by-product of the lspF mutation. The finding that the lspF mutant does not traffic more readily to the phagolysosome than the WT further suggests that it is not subject to greater degradation (19). Nonetheless, to determine if the lspF mutant undergoes increased lysis upon infection of human macrophages, we infected U937 cells with WT and mutant bacteria expressing cell-associated green fluorescent protein (GFP) and then assayed levels of GFP released from bacteria. We observed similar levels of GFP when we compared the lysates obtained from WT-infected cells to those obtained from mutant-infected cells (see Fig. S2 in the supplemental material), indicating that the T2S mutant does not undergo more lysis. Additional support for this conclusion comes from the fact that some but not all innate immune pathways are affected by the loss of T2S (see below). Thus, we concluded that the T2S system actively diminishes the expression of IL-6 by human macrophages infected with L. pneumophila.

T2S decreases stimulation of the MAPK and NF-κB pathways.

Given that NF-κB and AP-1 are transcription factors that regulate the activation and secretion of proinflammatory cytokines, we hypothesized that T2S inhibits signaling through one or both of these innate immunity pathways. Thus, U937 cells were infected with WT strain 130b or the lspF mutant and examined for levels of phosphorylated p38, stress-activated protein kinase (SAPK)/Jun amino-terminal kinase (JNK), and extracellular signal-regulated kinase 1/2 (ERK1/2), three adaptors within the MAPK pathway that are activated during L. pneumophila infection of murine and human macrophages (32,34). In all three cases, WT infection resulted in increased levels of phosphorylated proteins relative to those of the uninfected control (see Fig. S3A to S3C in the supplemental material). Compatible with our hypothesis, levels of phosphorylated p38 and SAPK/JNK were significantly higher during infection with mutant bacteria than during infection with the WT (Fig. 2A and andB).B). In contrast, the levels of phosphorylated ERK1/2 were higher in WT-infected cells (Fig. 2C). This net effect suggested that signaling directed at the AP-1 transcription factor is negatively affected by the T2S system. Hence, components of the AP-1 transcription factor, i.e., c-Jun and activating transcription factor 2 (ATF2), were also examined for their phosphorylation status. As expected, WT infection resulted in increased levels of the activated AP-1 components relative to those of the uninfected control (Fig. S3D and S3E). Moreover, both c-Jun and ATF2 had decreased levels of phosphorylation during strain 130b infection versus lspF mutant infection (Fig. 2D and andE),E), implying decreased AP-1 activation during WT infection. Together, these data indicated that signaling through the MAPK pathway is dampened by the L. pneumophila T2S system.

FIG 2
Activation levels of proteins in the MAPK and NF-κB pathways induced by infection of U937 cells with L. pneumophila WT and T2S mutant strains. U937 cells were infected with either WT strain 130b or lspF mutant strain NU275, and at 4 h postinoculation, ...

A second facet of innate immunity that controls cytokine transcription and is triggered by L. pneumophila infection in murine and human cells is signaling through NF-κB (32, 33, 35,39). Thus, we assessed levels of IκBα, the inhibitor of NF-κB that keeps the transcription factor sequestered in the cytoplasm of the cell. WT-infected cells displayed decreased IκBα levels relative to those of the uninfected control (see Fig. S3F in the supplemental material). Increased levels of IκBα were detected in U937 cells infected with WT strain 130b compared to cells infected with the lspF mutant (Fig. 2F), indicating that T2S limits the levels of NF-κB in the nuclei of L. pneumophila-infected macrophages. In sum, the dampening of both the MAPK and NF-κB pathways would explain, at least in part, why cytokine levels are lower in WT-infected cells than in T2S mutant-infected cells.

NLR and RLR signaling is necessary for optimal IL-6 secretion during L. pneumophila infection of human macrophages but is not required for the dampening effect of T2S on cytokine production.

The noninflammasome NLRs NOD1 and NOD2 are stimulated during L. pneumophila infection. This has been shown in the context of lung infection of knockout mice and infected BMD macrophages obtained from knockout mice as well as a human epithelial cell line (33, 40,43). The activation of the MAPK and NF-κB pathways is in part dependent upon NOD signaling, which is contingent upon RIP2 (44, 45). Thus, in order to assess the impact of NOD signaling on L. pneumophila infection of human macrophages as well as T2S-mediated dampening, we made a stable RIP2 knockdown U937 cell line with a 72% decrease in the protein level, as shown by immunoblotting (Fig. 3A). We infected these cells, along with control cells expressing a nontargeting short hairpin RNA (shRNA) (“scramble”) plasmid, with WT strain 130b as well as the T2S lspF mutant and then checked for both bacterial growth and IL-6 secretion. While a previous study reported an increase in WT L. pneumophila growth in the lungs of NLR-deficient mice (41), we did not find any impact of the NLR pathway on the intracellular CFU of either WT or T2S mutant bacteria (see Fig. S4A in the supplemental material). Knockdown of RIP2, however, resulted in a decrease in IL-6 production following 24 h of WT infection (Fig. 3B, top), showing, for the first time, that RIP2 is necessary for optimal cytokine stimulation during L. pneumophila infection of human macrophages. However, the ratio of cytokine output of WT-infected cells to that of T2S-mutant infected cells did not change as a result of the knockdown (Fig. 3B, bottom, for values normalized to the scramble controls; see also Fig. S5A for absolute values), indicating that the NLR pathway is not required for the T2S-dependent dampening of the cytokine response.

FIG 3
Effect of RIP2 depletion on cytokine production triggered by L. pneumophila WT and lspF mutant strains in macrophages. (A) Lysates obtained from U937 cells containing either an shRNA targeting RIP2 or a nontargeting scramble shRNA were subjected to immunoblot ...

In addition to triggering NLRs, L. pneumophila stimulates the RLR pathway, which is also linked to the type I interferon (IFN) response. This is based on studies using BMD macrophages from knockout mice and knockdown of RLR pathway adaptors in human epithelial cells (46,52). In order to judge the influence of RLR signaling on L. pneumophila infection of human macrophages as well as T2S-mediated dampening of innate immunity, we examined infected U937 cells that were knocked down for receptors and adaptors in the RLR pathway. Three stable knockdown cell lines were created with a 91% decrease for RIG-I, a 98% decrease for MDA-5, or a 52% decrease for MAVS (Fig. 4A). These knockdown cells were normal for WT and T2S mutant growth (see Fig. S4B to S4D in the supplemental material). Since L. pneumophila-infected U937 cells did not exhibit an induction of IFN-β transcripts or the secretion of detectable levels of IFN-β (data not shown), we surmised that the type I interferon response is not germane to the effect that we are studying, and therefore, we continued to use IL-6 as our marker for cytokine output. While the knockdown of the receptors RIG-I and MDA-5 did not alter cytokine signaling following WT infection (Fig. 4B and andC,C, top), the knockdown of the downstream adaptor MAVS decreased the IL-6 output from WT-infected cells (Fig. 4D, top), demonstrating, for the first time, the importance of MAVS in cytokine signaling by L. pneumophila-infected human macrophages. However, the knockdown of RIG-I and MDA5 and their adaptor MAVS did not decrease the ratio of the IL-6 output from mutant-infected cells to that from WT-infected cells (Fig. 4B to toD,D, bottom, for values normalized to the scramble control; see also Fig. S5B to S5D for absolute values). The ratio for MAVS knockdown macrophages actually increased, perhaps because the T2S system secretes a PAMP or secretes an enzyme that generates a PAMP that stimulates this pathway. Overall, this data set indicates that the RLR pathway is not required for the T2S-dependent dampening of IL-6.

FIG 4
Effect of RIG-I, MDA-5, or MAVS depletion on cytokine production triggered by L. pneumophila WT and lspF mutant strains in macrophages. (A) Lysates obtained from U937 cells containing either an shRNA targeting RIG-I, MDA5, or MAVS or a nontargeting scramble ...

The inflammasome in human macrophages is not required for the dampening effect of T2S on cytokine production.

During L. pneumophila infection of murine macrophages, activation of the inflammasome occurs through NAIP5/NLRC4, triggered by flagellin, as well as through an apoptosis-associated speck-like protein containing a CARD (ASC)-dependent pathway, resulting in the production of cytokines via an IL-1 autocrine loop (22, 23, 53,56). Humans lack the NAIP5 allele present in murine cells (57); however, the canonical ASC-dependent inflammasome is still activated upon L. pneumophila infection of human macrophages (58). Furthermore, it has been shown, via gene knockdown in human macrophages, that noncanonical inflammasome activation occurs through caspase-4, which serves as an intracellular lipopolysaccharide (LPS) receptor (59). In order to ascertain the role of the ASC-dependent inflammasome and caspase-4 in the dampening effect of the L. pneumophila T2S system, we created two stable U937 knockdown cells lines with a 73% decrease of both ASC and caspase-4 levels (Fig. 5A). The growth of WT and T2S mutant L. pneumophila bacteria in U937 cells was unaffected by the gene knockdowns (see Fig. S4E and S4F in the supplemental material). The knockdown of either the ASC or caspase-4 pathway decreased IL-6 production following WT infection (Fig. 5B and andC,C, top). This agrees with data from previous studies that showed that both ASC and caspase-4 are stimulated during L. pneumophila infection of human macrophages (59, 60), although our data are the first documentation of the role of ASC and caspase-4 in IL-6 secretion. The knockdown of ASC or caspase-4 did not decrease the ratio of the IL-6 output from mutant-infected cells to that from WT-infected cells (Fig. 5B and andC,C, bottom, and Fig. S5E and S5F). If anything, the ratio between the T2S mutant and the WT increased when either protein was knocked down, suggesting that a PAMP released by or generated as a result of the T2S system stimulates the ASC or caspase-4 pathway. Nonetheless, given that no decrease in the ratio of IL-6 stimulation from T2S mutant- versus WT-infected cells was seen, we concluded that the dampening effect of the T2S system does not require ASC- or caspase-4-mediated inflammasome responses.

FIG 5
Effect of ASC and caspase-4 depletion on cytokine production triggered by L. pneumophila WT and lspF mutant strains in macrophages. (A) Lysates obtained from U937 cells containing either an shRNA targeting ASC or caspase-4 or a nontargeting scramble shRNA ...

PKR is necessary for optimal IL-6 secretion during L. pneumophila infection of human macrophages; however, cytokine dampening by T2S is independent of PKR.

Double-stranded RNA (dsRNA)-dependent protein kinase receptor (PKR) is an intracellular RNA receptor that can stimulate proinflammatory cytokines. This protein has been implicated mainly in the host response to viral infection (61); however, it also plays a role in the immune response to bacterial products (62). One study using a PKR inhibitor showed that blocking of the PKR pathway in murine BMD macrophages does not affect the activation of the MAPK pathway during L. pneumophila infection (63); however, to our knowledge, PKR has not been studied in relation to L. pneumophila infection of human macrophages. In order to test the impact of this understudied pathway in a human model, we created a stable PKR knockdown in the U937 cell line with a 55% decrease in protein expression (Fig. 6A). The loss of PKR decreased the secretion of IL-6 following WT infection (Fig. 6B, top), indicating that PKR is involved in optimal cytokine secretion in response to L. pneumophila infection of human macrophages. However, PKR knockdown did not decrease the difference in IL-6 stimulation between WT-infected and T2S mutant-infected macrophages (Fig. 6B, bottom; see also Fig. S5G in the supplemental material). The loss of PKR also did not affect the levels of WT or T2S mutant growth during intracellular infection (Fig. S4G).

FIG 6
Effect of PKR depletion on cytokine production triggered by L. pneumophila WT and lspF mutant strains in macrophages. (A) Lysates obtained from U937 cells containing either an shRNA targeting PKR or a nontargeting scramble shRNA were subjected to immunoblot ...

Cytokine dampening by T2S is mediated through the immune adaptor MyD88.

Previous studies used knockout mice and BMD macrophages from these knockout mice to demonstrate that during intracellular infection, L. pneumophila stimulates TLRs, including both cell surface TLR2 (via the recognition of lipoprotein and LPS) and TLR5 (flagellin) and intracellular TLR9 (CpG oligodeoxynucleotide) (64,69). In order to test, for the first time, the importance of these pathways in human macrophages, we started out by generating a stable knockdown of MyD88 with a 76% decrease in protein expression (Fig. 7A). MyD88 is the adaptor for all the TLRs known to be important for L. pneumophila infection (22). While the loss of MyD88 did not appear to impact IL-6 secretion during WT infection (Fig. 7B, top), it resulted in a decrease in the ratios of IL-6 levels stimulated in T2S mutant infection to those in WT infection by 59% and 49% at the 48-h and 72-h time points, respectively (Fig. 7B, bottom; see also Fig. S5H in the supplemental material). In order to confirm that this decrease in the IL-6 secretion ratio was a result of the decrease in the level of MyD88 and not an unintended off-target effect of the V2LHS_152058 shRNA plasmid (Table 1), we used shRNA plasmid V2LHS_152059 to generate a second independent MyD88 knockdown cell line. This cell line displayed a 54% decrease in protein levels (Fig. S6A). Importantly, infection of this cell line also showed a decrease in the difference in the IL-6 output from mutant- versus WT-infected cells (Fig. S6B), validating that MyD88-mediated signaling is dampened by T2S and suggesting that there is an effect on an upstream TLR(s).

FIG 7
Effect of MyD88 or TBK1 depletion on cytokine production triggered by L. pneumophila WT and lspF mutant strains in macrophages. (A) Lysates obtained from U937 cells containing either an shRNA targeting MyD88 or TBK1 or a nontargeting scramble shRNA were ...
TABLE 1
Plasmids used for gene silencing in U937 cells

In order to obtain further support for the role of MyD88 in dampening, we knocked down TANK binding kinase 1 (TBK1), a second, downstream adaptor in the TLR signaling pathway, among other immune-signaling pathways (70,72). When the protein level of TBK1 was decreased by 87% in a stable knockdown in U937 cells (Fig. 7A), there was a substantial drop in IL-6 levels upon WT infection (Fig. 7C, top), formally documenting the role of TBK1 in human macrophage infection. The finding that the knockdown of TBK1 had a greater effect than did the knockdown of MyD88 (compare Fig. 7B and andC)C) is likely due to the fact that TBK1 is also an adaptor for the RLR pathway as well as many intracellular RNA/DNA receptors (70). Importantly, similarly to our observation with the knockdown of MyD88, the knockdown of TBK1 led to a decrease in the difference between the IL-6 outputs of T2S mutant- and WT-infected macrophages, specifically showing a 44% decrease at 48 h postinfection (Fig. 7C, bottom; see also Fig. S5I in the supplemental material). The loss of MyD88 and TBK1 did not influence the growth of the WT or the T2S mutant in U937 monolayers (Fig. S4H and S4I). Overall, these data indicate that T2S-mediated dampening occurs through both MyD88 and TBK1, further suggesting an effect on the upstream TLRs known to be involved in L. pneumophila infection (i.e., TLR2, TLR5, and/or TLR9).

T2S-mediated dampening of the cytokine response is facilitated through TLR2.

In order to begin to determine which TLR(s) is involved in T2S-mediated dampening, we generated a knockdown of TLR2 reducing protein expression by 86% (Fig. 8A). As expected, the gene knockdown reduced the responsiveness of macrophages to purified palmitoyl-3-Cys-Ser-(Lys)4 (Pam3CSK4), a known agonist for TLR2 (see Fig. S7 in the supplemental material). This TLR2 knockdown did not lead to a decrease in the IL-6 output during WT infection of U937 cells and in fact led to an increase in the early cytokine output (Fig. 8B, top). However, more significantly, it led to a decrease in the difference in IL-6 outputs from T2S mutant-infected compared to WT-infected macrophages, with decreases of 49% at 48 h and 60% at 72 h (Fig. 8B, bottom, and Fig. S5J). Indeed, the effect of the TLR2 knockdown was equivalent to that seen with the MyD88 knockdown. The TLR2 knockdown, along with the MyD88 knockdown, also led to a decrease in the difference in IL-8 outputs from T2S mutant-infected compared to WT-infected macrophages at 48 h or 72 h (Fig. S8). Together, these data indicate that the TLR2 pathway is dampened by the T2S system of L. pneumophila.

FIG 8
Effect of TLR2, TLR9, or TRIF depletion on cytokine production triggered by infection of macrophages with L. pneumophila WT and lspF mutant strains. (A) Lysates obtained from U937 cells containing either an shRNA targeting TLR2, TLR9, or TRIF or a nontargeting ...

To assess if any of the other TLRs linked to L. pneumophila infection were involved in T2S-mediated dampening, we next knocked down TLR9, leading to a 63% decrease in protein expression (Fig. 8A). This knockdown did not lead to a decrease in IL-6 stimulation during WT infection (Fig. 8C, top), nor did it lead to a decrease in the difference in IL-6 outputs from T2S mutant- compared to WT-infected macrophages (Fig. 8C, bottom; see also Fig. S5K in the supplemental material), indicating that TLR9 signaling is not dampened by T2S. We next turned our attention to TLR5 but were unable to knock down this TLR in U937 cells. However, since TLR5 is the receptor for the L. pneumophila PAMP flagellin (68), we generated an L. pneumophila flaA lspF mutant that lacks the T2S system as well as flagellin and then tested its ability to trigger cytokine production. The flaA lspF double mutant elicited IL-6 secretion at the same level as that of the lspF mutant (Fig. S9), indicating that flagellin is not required for the observed effect of T2S, and therefore, TLR5 is unlikely to be involved in cytokine dampening.

As an additional step toward investigating the possible involvement of other TLRs in cytokine dampening, we knocked down TIR domain-containing adaptor inducing interferon beta (TRIF). The TRIF protein is a downstream adaptor for TLR3 and TLR4. Although TLR3 and TLR4 have not been implicated in signaling during L. pneumophila infection of murine cells (66, 73), we considered this a first approach to look at the involvement of these two TLRs in L. pneumophila infection of human macrophages. The knockdown of TRIF led to an 81% decrease in the protein level (Fig. 8A) and resulted in a decrease in IL-6 stimulation at the 24-h time point following WT infection (Fig. 8D, top), indicating, for the first time, that TRIF is necessary for optimal IL-6 secretion in human macrophage infection. However, the ratio of IL-6 secreted during T2S mutant infection to that secreted during WT infection remained the same between scramble and knockdown cells (Fig. 8D, bottom; see also Fig. S5L in the supplemental material), indicating that TRIF is not required for T2S-dependent dampening during L. pneumophila infection of human macrophages. TRIF was also unimportant for the intracellular growth of the WT and the T2S mutant (Fig. S4J). Overall, our data set indicates that L. pneumophila dampens the MyD88- and TBK1-dependent TLR2 pathway in a T2S-dependent manner, leading to a reduction in cytokine levels produced by infected human macrophages.

DISCUSSION

Building upon our previous work (16), we have now demonstrated that L. pneumophila T2S dampens the cytokine response of three types of human macrophage-like cells, including cells obtained from human volunteers. Therefore, we strongly suspect that this effect of T2S has implications for human disease caused by L. pneumophila. Our new immunoblot data indicate that the previously observed effect of T2S on cytokine gene transcription (16) is due, at least partly, to a dampening of the macrophage's MAPK and NF-κB pathways. Although it is possible that proteins secreted via T2S act directly on components of the MAPK and NF-κB pathways, as has been documented following exposure to various pathogens (21, 74,76), we focused this study on discerning whether T2S diminishes the upstream event of PAMP recognition. By generating a set of human knockdown cell lines, we determined that the NLR, RLR, TRIF, and PKR pathways as well as ASC- and caspase-4-dependent inflammasomes are not required for the T2S dampening effect. However, utilizing a similar experimental approach, we gained evidence for T2S acting on the MyD88-dependent TLR2 pathway. Based on the current literature, this pathway is involved in recognizing L. pneumophila LPS (66, 67) as well as a peptidoglycan-associated lipoprotein (77); however, there is still the possibility that there is an as-yet-unidentified PAMP recognized by TLR2. Further support for the L. pneumophila T2S system acting upon the TLR2 pathway is the fact that the dampening effect of T2S, although clearly evident in human macrophages, was not manifest for infected murine macrophages. Indeed, the TLR2 pathway in human cells can be different from that in murine cells. Although human TLR2 and murine TLR2 share 84% amino acid similarity in their intracellular domains, they are only 65% similar in their extracellular domains, and thus, the two TLRs differ in their abilities to recognize ligands. For example, while human TLR2 discriminates between the tripalmitoylated peptide P3CSK4 and the trilauroylated lipopeptide Lau3CSK4 (both of which are synthetic analogs of microbial lipopeptides), responding only to the former, murine TLR2 responds to both of these lipopeptide ligands (78). To our knowledge, the connection between L. pneumophila T2S and the manipulation of innate immunity that we have documented is a novel illustration of the functional importance of a T2S system.

The dampening effect of T2S on the TLR2 pathway in human macrophages could be occurring at a number of levels. In the simplest scenario, a T2S-dependent effector(s) could limit the host recognition of the TLR2 agonists (e.g., LPS and/or lipopeptides) that are present on or released by the bacterium. As a first possible explanation, T2S might be secreting an effector(s) that limits the levels of LPS and lipopeptides or alters their conformation in some way such that they are no longer recognized by human TLR2. It has been theorized that L. pneumophila LPS is recognized by TLR2 because it contains long fatty acid chains in its lipid A and because it has a ketone group on the penultimate carbon of one of these fatty acid chains (67). Thus, a secreted effector that either cleaves or otherwise changes the fatty acids in the LPS could be one explanation for how T2S decreases signaling through TLR2. Based on our in silico analysis of the L. pneumophila genome, there are multiple putative lipases predicted to be secreted by T2S that could be involved in processing and deacylating LPS (12), analogous to lipases from other bacteria (79,83). As a second means by which T2S could diminish PAMP recognition by TLR2, it is possible that a protein effector secreted into the LCV impedes the translocation of LPS and/or lipopeptides out of the LCV and into the macrophage cytoplasm and perhaps ultimately into the extracellular milieu. Although historically, TLR2 has been named a surface TLR, recent findings have challenged this idea and demonstrated intracellular TLR2 colocalizing with its ligand (84, 85). As a final way in which T2S might impede the TLR2 pathway, it is conceivable that a secreted bacterial protein traffics out of the LCV and obstructs recognition by blocking, cleaving, or otherwise altering the host receptor or a downstream adaptor such as MyD88. Although TLR5 and TLR9 also signal through MyD88, the fact that we see a dampening of only the TLR2 pathway could be because there is more stimulation of TLR2 than of TLR5 and TLR9 during L. pneumophila infection. Compatible with the possibility of an effector directly targeting the host receptor or adaptor, there is already an example of a T2S-dependent substrate occurring in the cytosol of infected macrophages (86), although this particular effector, the ProA metalloprotease, is not required for the dampening of cytokine gene transcription (16). Thus, we posit the existence of a novel T2S-dependent effector that impedes the functioning of the TLR2 pathway.

Although the dampening effect of T2S on the cytokine output is evident 24, 48, and 72 h after infection of U937 cells (16), the impact of the knockdown of MyD88, TBK1, or TLR2 on the ratio of the amount of IL-6 from mutant infections relative to that from WT infections, although evident at 48 and/or 72 h, was not seen at 24 h (Fig. 7 and and8).8). This suggests that the dampening effect of T2S is not due solely to an effect on the MyD88-TLR2 signaling pathway. Even at 48 and 72 h, the contribution of MyD88-TLR2 was not the full explanation, as knockdowns resulted in 50 to 60% reductions of T2S-mediated dampening (Fig. 7B and and8B).8B). Taken together, the T2S-dampening effect at earlier time points (e.g., 4 to 24 h) might mainly involve a pathway(s) that is yet to be defined, but at later times (e.g., 48 and 72 h), it is primarily (but not entirely) due to the action on MyD88-TLR2. It is also formally possible that the T2S-dampening effect, particularly at the earlier time points, involves one of the known signaling pathways that we have examined here (i.e., the NLR, RLR, TRIF, and PKR pathways and ASC- and caspase-4-dependent inflammasomes) but that the level of inhibition of any one pathway is low, such that the single-gene knockdowns that we performed did not show an effect. Thus, the identification of the additional target(s) of T2S might require the simultaneous knockdown of multiple signaling pathways.

The dampening effect of T2S on TBK1 also suggests that L. pneumophila T2S could limit another PAMP recognition pathway(s), in addition to TLR signaling. In recent years, a number of TBK1-utilizing pathways have been discovered and shown to be involved mostly in the recognition of viral or bacterial nucleic acid that is present in the cytoplasm of infected cells. These pathways include the cGAS (cyclic GMP-AMP synthase) pathway, the MRE11 (meiotic recombination 11 homolog A) pathway, and the DAI (DNA-dependent activator of IFN regulatory factors) pathway (87, 88). Whereas DAI is not required for the expression of IFN-β triggered by L. pneumophila infection of a human lung epithelial cell line (47), cGAS is active during L. pneumophila infection of BMD murine macrophages (89). Thus, it is possible that one or more of these TBK1-dependent pathways are also inhibited by T2S during L. pneumophila infection of human macrophages.

The decrease of the cytokine response by the T2S system has implications for understanding Legionella pathogenesis. In addition to IL-6 and IL-8, which served as the readouts in this study, we previously observed that the T2S system is able to decrease the levels of human tumor necrosis factor alpha (TNF-α) and IL-1β in supernatants of infected macrophages (16). Since these various proinflammatory cytokines fulfill a number of important roles in host defense, including increasing vasodilation, recruiting and activating leukocytes, triggering the release of acute-phase proteins, and activating complement and opsonization (16), we hypothesize that the dampening effect of T2S on TLR2 signaling contributes to the ability of L. pneumophila to grow in the human lung and cause pneumonia. Previously, we also determined that the T2S-dependent CelA endoglucanase, ChiA chitinase, LapA and LapB aminopeptidases, LipA and LipB lipases, Map phosphatase, PlaA lysophospholipase A, PlaC glycerophospholipid:cholesterol acyltransferase, PlcA and PlcB phospholipases C, and SrnA RNase are not required for the dampening of the cytokine output, and the ProA metalloprotease, although able to directly degrade cytokines, does not affect the levels of cytokine gene transcripts (16). Our proteomic and in silico analyses indicate that the L. pneumophila T2S system exports between 25 and 60 proteins, including several putative lipolytic enzymes and a number of novel proteins (12, 13, 15). Thus, future studies will be directed toward, among other things, identifying which T2S-dependent effector(s) is responsible for impeding immune signaling and then determining its molecular mode of action. We suspect that the observations made here by studying L. pneumophila T2S will have implications for other pathogens that grow in or otherwise target macrophages.

While the initial impetus for this study was the investigation of the dampening effect of T2S on cytokine production by human macrophages, the generation of cell lines deficient in individual immune pathways led to substantial new information regarding innate immune pathways that operate during (WT) L. pneumophila infection. Our data set documented, for the first time, a variety of pathways as being important for optimal cytokine stimulation during L. pneumophila infection of macrophages, including the intracellular RNA receptor PKR, the TLR adaptor TRIF, and the RNA/DNA sensor adaptor TBK1. We also demonstrated that many of the signaling pathways known to be involved in L. pneumophila infection of murine cells are also operative during infection of human cells, including the noninflammasome NLR pathway through the adaptor RIP2, the RLR pathway through the adaptor MAVS, and the inflammasome through ASC and caspase-4. Finally, the dampening effect of T2S was not seen in murine macrophages, demonstrating that PAMP recognition is more distinct between human and mice than previously reported.

MATERIALS AND METHODS

Bacterial strains, bacteriological media, and chemicals.

L. pneumophila strain 130b (ATCC BAA-74, also known as AA100) is a clinical isolate that served as our WT and parental strain for mutants (90). Both mutant strain NU275, which lacks a functional lspF gene that encodes an inner membrane component of the T2S apparatus, and mutant strain NU347, which lacks a functional flaA gene encoding flagellin, were described previously (18, 91). A mutant lacking both flaA and lspF (NU430) was obtained by introducing pGlspF::Km (18) into NU347 by transformation (91) and then selecting for the acquisition of kanamycin resistance. In order to help monitor the behavior of L. pneumophila in macrophages, we utilized previously reported L. pneumophila WT and T2S mutant strains with a GFP-expressing plasmid introduced (19). Legionellae were routinely cultured at 37°C in buffered yeast extract (BYE) broth or on buffered charcoal yeast extract (BCYE) agar, which, when appropriate, contained gentamicin or kanamycin (92). Unless noted otherwise, chemicals were purchased from Sigma-Aldrich (St. Louis, MO). Catalog numbers are indicated when there is more than one version of a reagent available from the vendor.

Macrophage lines and intracellular infection assays.

In order to assess L. pneumophila growth within macrophages as well as the effects of bacterial infection on host cell function, we utilized a human U937 cell line (ATCC CRL-1593.2), a human THP-1 cell line (ATCC TIB 202), and BMD macrophages obtained from 6- to 8-week-old female A/J mice (Jackson Laboratory, Bar Harbor, ME) (16, 27, 93). The preparation of the different macrophages was done as previously described, with the exception of THP-1 cells, which were differentiated by incubation for 24 h in RPMI medium (catalog number 10-040-CV; Corning Mediatech, Inc., Manassas, VA) containing 10% fetal bovine serum (Atlanta Biologicals, Lawrenceville, GA) and 100 ng/ml phorbol myristate acetate (catalog number P8139; Sigma) and at a concentration of 1 × 106 cells/well in a 24-well tissue culture plate (94). For our infection analysis, we also used PBMCs, which had been obtained from healthy human volunteers, as previously described (95). To this end, phosphate-buffered saline (PBS) containing 7.5 U heparin/ml (catalog number H3149; Sigma) was added at three times the volume of the buffy coat (obtained from C. Gunderson and H. Seifert, Northwestern University), and the resulting suspension was centrifuged at 500 × g for 10 min. The cell pellet was resuspended in 0.3 mM EDTA in PBS, and the suspension was then centrifuged at 100 × g for 10 min. After washing of the pellet in this manner two more times, the mononuclear fraction was suspended in RPMI medium containing 15% human serum (catalog number H6914; Sigma), and the cell suspension was then added to tissue culture-treated, 24-well polystyrene plates (Falcon, Corning, NY) and incubated overnight at 37°C. To enrich for the adherent mononuclear cell population, as described previously (28, 96,98), the newly formed monolayers were washed three times to exclude nonadherent cells from the plate, and RPMI medium containing 15% human serum was then added back. The adherent mononuclear cells were then allowed to differentiate in human serum-containing medium for an additional 6 days, as previously described (96, 98).

In order to assess the role of innate immune pathways during infection, we generated a series of stable U937 knockdown cell lines. The generation of these cell lines was done as previously described (19). Briefly, silencing was achieved by transduction with a vesicular stomatitis virus glycoprotein (VSV-G)-pseudotyped lentivirus that encodes an shRNA molecule targeting the gene of interest. Table 1 lists plasmids used for gene silencing and their sources. As a control, a nontargeting shRNA plasmid (scramble) was introduced into U937 cells, and the scramble cell line that was obtained was used to compare results from cell lines carrying a target shRNA plasmid. When experiments utilized cell lines carrying shRNA plasmids from GE Healthcare (Table 1), scramble control cells were generated by using plasmid RHS4346 (GE Healthcare, Chalfont, UK). For experiments where cell lines carrying shRNA plasmids from Sigma were used (Table 1), the scramble plasmid SHC016 (Sigma-Aldrich, St. Louis, MO) was utilized. In an attempt to knock down TLR5, we utilized shRNA plasmids V2LHS_171357 and V2LHS_171361 from GE Healthcare and shRNA plasmids TRCN0000430395, TRCN0000431479, TRCN0000056956, TRCN0000056954, and TRCN0000056953 from Sigma-Aldrich, but we were ultimately unable to reduce TLR5 protein levels with these shRNA plasmids.

Monolayers containing 0.25 × 106 to 1 × 106 macrophages were inoculated with bacteria at a multiplicity of infection (MOI) of 0.5 (for WT and knockdown U937 cells, THP-1 cells, and PBMCs) or an MOI of 1 (for murine BMD macrophages), incubated for 2 h to allow bacterial entry, and then washed three times with RPMI medium to remove any remaining extracellular legionellae (16). At 0, 24, 48, and 72 h postinoculation, the infected monolayers were lysed, and dilutions were plated onto BCYE agar in order to determine the number of intracellular CFU (16). In order to examine the effect of L. pneumophila on cytokine production, macrophages were infected with WT and mutant bacteria as noted above, and after 24, 48, or 72 h of incubation, the amount of IL-6 or IL-8 in cell-free culture supernatants was measured by using Ready-Set-Go enzyme-linked immunosorbent assay (ELISA) kits (EBioscience, San Diego, CA), as described previously (16). However, to judge IL-6 levels after 4 h of infection, inoculation of U937 cells was done by employing an MOI of 10 in order to increase the number of infected macrophages within the monolayer. To measure IFN-β levels in culture supernatants, we utilized an IFN-β ELISA kit (catalog number 41410-1; R&D Systems, Minneapolis, MN). In order to assess the phenotype of our TLR2 knockdown cells, we stimulated scramble or knockdown cells with 50 ng/ml the purified TLR2 ligand Pam3CSK4 (catalog number tlrl-pms; InvivoGen, San Diego, CA) for 24 h and then collected supernatants and assessed IL-6 secretion using the Ready-Set-Go IL-6 ELISA kit.

Immunoblot analysis of macrophage gene knockdown and of the MAPK and NF-κB pathways in infected macrophages.

Immunoblot analyses were used both to confirm the knockdown of target proteins in gene knockdown in stable U937 cell lines and to check the activation status of adaptors important in the MAPK and NF-κB pathways. For confirmation of the knockdown, U937 cell monolayers were prepared as usual (16), after which protein levels of shRNA targets were probed. For analysis of the activation of MAPK and NF-κB pathways, U937 cell monolayers were either left uninfected or inoculated with L. pneumophila at an MOI of 50, and at 4 h postinoculation, the phosphorylation of proteins involved in immune signaling was determined (99). For both assays, at the indicated time points, the tissue culture medium was removed from the wells containing the monolayers, the wells were washed with PBS, and 100 μl of 4°C radioimmunoprecipitation assay (RIPA) buffer (50 mM Tris [pH 7.4], 150 mM NaCl, 2 mM EDTA, 0.2% Triton X-100, 0.3% NP-40 alternative, 25 mM NaF, 0.1 mM Na orthovanadate, 0.25% Na deoxycholate) that contained a protease inhibitor (RIPA-PI) was then added. To prepare a stock solution of RIPA-PI, one tablet of a protease inhibitor (catalog number 04693124001; Roche, Penzberg, Germany) was dissolved in 10 ml of RIPA buffer. U937 cells were resuspended in RIPA-PI by using a cell scraper (catalog number 353085; Fisher Scientific, Pittsburgh, PA), and after the addition of 1 μl of phenylmethylsulfonyl fluoride, the cell suspension was incubated for 10 min on ice. Lysis of the infected cells was completed by passing the sample through a 22-gauge syringe (catalog number 305156; BD Biosciences, San Jose, CA) five times. Next, the lysate was centrifuged at 16,300 × g for 15 min at 4°C in order to remove cellular debris and bacteria. The resulting supernatant containing soluble host proteins was subjected to SDS-polyacrylamide (8 to 12%) gel electrophoresis, and separated proteins were then transferred onto a polyvinylidene difluoride (PVDF) membrane (catalog number 88518; Thermo Scientific, Waltham, MA) (99). Next, the blots were incubated for 12 h at 4°C in 5% bovine serum albumin (BSA) (catalog number A4503; Sigma) for the detection of phosphorylated SAPK/JNK (p-SAPK/JNK), p-ERK1/2, and p-ATF2 or in 5% nonfat dry milk (i.e., blotting-grade blocker from Bio-Rad) for probing for p-c-Jun, p-p38, IκBα, TLR2, TLR9, ASC, TBK1, RIP2, MyD88, RIG-I, MAVS, MDA-5, PKR, caspase-4, TRIF, glyceraldehyde-3-phosphate dehydrogenase (GAPDH), and H3. For the most part, primary antibodies were added at a concentration of 1:1,000 in Tris-buffered saline containing 5% Tween 20 (catalog number P1379; Sigma) (TBS-T) and 5% BSA and incubated at 4°C for 12 h. However, for the detection of H3 and GAPDH, the primary antibodies were diluted in TBS-T containing 5% nonfat dry milk at concentrations of 1:2,000, and 1:4,000, respectively, and for TLR9, incubation was done for 1 h. All primary antibodies were purchased from Cell Signaling Technology (Danvers, MA), with the exception of anti-GAPDH antiserum, which was obtained from Santa Cruz Biotechnology (Dallas, TX). After a series of washes, the blots were incubated with secondary antibody solutions for 1 h at room temperature. An anti-rabbit immunoglobulin G (IgG)-horseradish peroxidase (HRP) conjugate (Cell Signaling) diluted 1:1,000 was used for the detection of all primary antibodies, except for those directed against TLR9, H3, and GAPDH. In the case of H3 and TLR9 detection, the anti-rabbit IgG-HRP conjugate was used at a 1:2,000 dilution, and for the detection of GAPDH, an anti-mouse IgG-HRP conjugate (Cell Signaling) was used at a 1:3,000 dilution. The detection reagents used were ECL (Amersham, Buckinghamshire, UK) for the GAPDH and H3 blots and ECL prime (Amersham) for all other blots, and Amersham Hyperfilm was used to develop the images of the blots (19). Image Lab software (Bio-Rad) was used to quantify the detection signals generated on the immunoblots.

Immunoblot assessment of bacterial lysis within infected macrophages.

U937 cell monolayers were inoculated with GFP-expressing L. pneumophila strains at an MOI of 50, as noted above, and at 4 h postinoculation, the amount of GFP released into the soluble fraction in infected macrophages was determined by immunoblot analysis. At 4 h, the culture medium was removed from the wells and replaced with 1 ml of fresh medium containing 0.1% saponin in order to lyse the infected U937 cells (but not the intact bacteria contained within them) (100). After dislodging the macrophages from the plate with a cell scraper, the sample was centrifuged in a microcentrifuge tube at 16,300 × g for 10 min at 4°C. The pellet containing intact bacteria and large cellular debris was resuspended and lysed in Laemmli buffer (101). Soluble proteins within the supernatant were isolated and concentrated, as previously described (102), and then reconstituted in Laemmli buffer. Cellular and soluble fractions were subjected to SDS-polyacrylamide gel electrophoresis, and the separated proteins were transferred to a PVDF membrane. After incubation of the membranes for 12 h at 4°C in TBS-T containing 5% nonfat dry milk, the membranes were treated with anti-GFP antibody (catalog number 2956s; Cell Signaling) at a dilution of 1:1,000 in TBS-T containing 5% nonfat dry milk for 12 h at 4°C. Following washes, the blots were incubated with an anti-rabbit IgG-horseradish conjugate at a dilution of 1:1,000 in TBS-T containing 5% dry milk for 1 h at room temperature, and they were then developed by using ECL Prime and analyzed as noted above.

Quantitative reverse transcription-PCR.

At 24 h postinoculation, RNA was purified from infected U937 cells by using the RNeasy minikit (Qiagen, Hilden, Germany). cDNA was made by using the iScript cDNA synthesis kit (Bio-Rad, Hercules, CA). The cDNA was amplified by PCR using primers specific for IFN-β and GAPDH (Hs02621180_s1 and Hs00266705_g1) (Applied Bioscience, Carlsbad, CA), an ABI 7500 thermal cycler (Applied Biosystems, Foster City, CA), and TaqMan probes (Applied Biosystems). As described previously (16), GAPDH served as a control gene for analysis of changes in cycle threshold values; fold induction above the uninfected control was ascertained based on changes in the cycle threshold values.

Supplementary Material

Supplemental material:

ACKNOWLEDGMENTS

We thank past and present members of the Cianciotto laboratory for their helpful advice and Richard White in particular for his assistance in providing a protocol for generating knockdown macrophages. We also acknowledge Carl Gunderson in the Seifert laboratory for providing buffy coat from anonymous human volunteers and Christian Stehlik and his laboratory for their technical guidance.

This work was funded by NIH grant AI043987 awarded to N.P.C.

Footnotes

Supplemental material for this article may be found at https://doi.org/10.1128/IAI.00897-16.

REFERENCES

1. Cianciotto NP, Hilbi H, Buchrieser C 2013. Legionnaires' disease, p 147–217. In Rosenberg E, DeLong EF, Lory S, Stackebrandt E, Thompson F (ed), The prokaryotes: human microbiology, 4th ed Springer, New York, NY.
2. Cunha BA, Burillo A, Bouza E 2016. Legionnaires' disease. Lancet 387:376–385. doi:.10.1016/S0140-6736(15)60078-2 [PubMed] [Cross Ref]
3. Dooling KL, Toews KA, Hicks LA, Garrison LE, Bachaus B, Zansky S, Carpenter LR, Schaffner B, Parker E, Petit S, Thomas A, Thomas S, Mansmann R, Morin C, White B, Langley GE 2015. Active bacterial core surveillance for legionellosis—United States, 2011-2013. MMWR Morb Mortal Wkly Rep 64:1190–1193. doi:.10.15585/mmwr.mm6442a2 [PubMed] [Cross Ref]
4. Mercante JW, Winchell JM 2015. Current and emerging Legionella diagnostics for laboratory and outbreak investigations. Clin Microbiol Rev 28:95–133. doi:.10.1128/CMR.00029-14 [PMC free article] [PubMed] [Cross Ref]
5. Parr A, Whitney EA, Berkelman RL 2015. Legionellosis on the rise: a review of guidelines for prevention in the United States. J Public Health Manag Pract 21:E17–E26. doi:.10.1097/PHH.0000000000000123 [PMC free article] [PubMed] [Cross Ref]
6. van Heijnsbergen E, Schalk JA, Euser SM, Brandsema PS, den Boer JW, de Roda Husman AM 2015. Confirmed and potential sources of Legionella reviewed. Environ Sci Technol 49:4797–4815. doi:.10.1021/acs.est.5b00142 [PubMed] [Cross Ref]
7. Finsel I, Hilbi H 2015. Formation of a pathogen vacuole according to Legionella pneumophila: how to kill one bird with many stones. Cell Microbiol 17:935–950. doi:.10.1111/cmi.12450 [PubMed] [Cross Ref]
8. Prashar A, Terebiznik MR 2015. Legionella pneumophila: homeward bound away from the phagosome. Curr Opin Microbiol 23:86–93. doi:.10.1016/j.mib.2014.11.008 [PubMed] [Cross Ref]
9. Cianciotto NP. 2013. Type II secretion and Legionella virulence. Curr Top Microbiol Immunol 376:81–102. doi:.10.1007/82_2013_339 [PubMed] [Cross Ref]
10. Kubori T, Nagai H 2016. The type IVB secretion system: an enigmatic chimera. Curr Opin Microbiol 29:22–29. doi:.10.1016/j.mib.2015.10.001 [PubMed] [Cross Ref]
11. Nivaskumar M, Francetic O 2014. Type II secretion system: a magic beanstalk or a protein escalator. Biochim Biophys Acta 1843:1568–1577. doi:.10.1016/j.bbamcr.2013.12.020 [PubMed] [Cross Ref]
12. DebRoy S, Dao J, Soderberg M, Rossier O, Cianciotto NP 2006. Legionella pneumophila type II secretome reveals unique exoproteins and a chitinase that promotes bacterial persistence in the lung. Proc Natl Acad Sci U S A 103:19146–19151. doi:.10.1073/pnas.0608279103 [PubMed] [Cross Ref]
13. Tyson JY, Pearce MM, Vargas P, Bagchi S, Mulhern BJ, Cianciotto NP 2013. Multiple Legionella pneumophila type II secretion substrates, including a novel protein, contribute to differential infection of amoebae Acanthamoeba castellanii, Hartmannella vermiformis, and Naegleria lovaniensis. Infect Immun 81:1399–1410. doi:.10.1128/IAI.00045-13 [PMC free article] [PubMed] [Cross Ref]
14. Söderberg MA, Dao J, Starkenburg S, Cianciotto NP 2008. Importance of type II secretion for Legionella pneumophila survival in tap water and amoebae at low temperature. Appl Environ Microbiol 74:5583–5588. doi:.10.1128/AEM.00067-08 [PMC free article] [PubMed] [Cross Ref]
15. Tyson JY, Vargas P, Cianciotto NP 2014. The novel Legionella pneumophila type II secretion substrate NttC contributes to infection of amoebae Hartmannella vermiformis and Willaertia magna. Microbiology 160:2732–2744. doi:.10.1099/mic.0.082750-0 [PMC free article] [PubMed] [Cross Ref]
16. McCoy-Simandle K, Stewart CR, Dao J, Debroy S, Rossier O, Bryce PJ, Cianciotto NP 2011. Legionella pneumophila type II secretion dampens the cytokine response of infected macrophages and epithelia. Infect Immun 79:1984–1997. doi:.10.1128/IAI.01077-10 [PMC free article] [PubMed] [Cross Ref]
17. Rossier O, Cianciotto NP 2001. Type II protein secretion is a subset of the PilD-dependent processes that facilitate intracellular infection by Legionella pneumophila. Infect Immun 69:2092–2098. doi:.10.1128/IAI.69.4.2092-2098.2001 [PMC free article] [PubMed] [Cross Ref]
18. Rossier O, Starkenburg S, Cianciotto NP 2004. Legionella pneumophila type II protein secretion promotes virulence in the A/J mouse model of Legionnaires' disease pneumonia. Infect Immun 72:310–321. doi:.10.1128/IAI.72.1.310-321.2004 [PMC free article] [PubMed] [Cross Ref]
19. White RC, Cianciotto NP 2016. Type II secretion is necessary for optimal association of the Legionella-containing vacuole with macrophage Rab1B but enhances intracellular replication mainly by Rab1B-independent mechanisms. Infect Immun 84:3313–3327. doi:.10.1128/IAI.00750-16 [PMC free article] [PubMed] [Cross Ref]
20. Newton HJ, Ang DK, van Driel IR, Hartland EL 2010. Molecular pathogenesis of infections caused by Legionella pneumophila. Clin Microbiol Rev 23:274–298. doi:.10.1128/CMR.00052-09 [PMC free article] [PubMed] [Cross Ref]
21. Asrat S, Davis KM, Isberg RR 2015. Modulation of the host innate immune and inflammatory response by translocated bacterial proteins. Cell Microbiol 17:785–795. doi:.10.1111/cmi.12445 [PMC free article] [PubMed] [Cross Ref]
22. Massis LM, Zamboni DS 2011. Innate immunity to Legionella pneumophila. Front Microbiol 2:109. doi:.10.3389/fmicb.2011.00109 [PMC free article] [PubMed] [Cross Ref]
23. Shin S. 2012. Innate immunity to intracellular pathogens: lessons learned from Legionella pneumophila. Adv Appl Microbiol 79:43–71. doi:.10.1016/B978-0-12-394318-7.00003-6 [PubMed] [Cross Ref]
24. Palusinska-Szysz M, Janczarek M 2010. Innate immunity to Legionella and Toll-like receptors—review. Folia Microbiol (Praha) 55:508–514. doi:.10.1007/s12223-010-0084-8 [PubMed] [Cross Ref]
25. Khweek AA, Amer A 2010. Replication of Legionella pneumophila in human cells: why are we susceptible? Front Microbiol 1:133. doi:.10.3389/fmicb.2010.00133 [PMC free article] [PubMed] [Cross Ref]
26. Franchi L, Nunez G 2011. A new twist in the regulation of Legionella replication through ASC and caspase-1. Front Microbiol 2:57. doi:.10.3389/fmicb.2011.00057 [PMC free article] [PubMed] [Cross Ref]
27. Naylor J, Cianciotto NP 2004. Cytochrome c maturation proteins are critical for in vivo growth of Legionella pneumophila. FEMS Microbiol Lett 241:249–256. doi:.10.1016/j.femsle.2004.10.028 [PubMed] [Cross Ref]
28. Horwitz MA, Silverstein SC 1980. Legionnaires' disease bacterium (Legionella pneumophila) multiplies intracellularly in human monocytes. J Clin Invest 66:441–450. doi:.10.1172/JCI109874 [PMC free article] [PubMed] [Cross Ref]
29. Lomma M, Dervins-Ravault D, Rolando M, Nora T, Newton HJ, Samson FM, Sahr T, Gomez-Valero L, Jules M, Hartland EL, Buchrieser C 2010. The Legionella pneumophila F-box protein Lpp2082 (AnkB) modulates ubiquitination of the host protein parvin B and promotes intracellular replication. Cell Microbiol 12:1272–1291. doi:.10.1111/j.1462-5822.2010.01467.x [PubMed] [Cross Ref]
30. Molmeret M, Zink SD, Han L, Abu-Zant A, Asari R, Bitar DM, Abu Kwaik Y 2004. Activation of caspase-3 by the Dot/Icm virulence system is essential for arrested biogenesis of the Legionella-containing phagosome. Cell Microbiol 6:33–48. doi:.10.1046/j.1462-5822.2003.00335.x [PubMed] [Cross Ref]
31. Vinzing M, Eitel J, Lippmann J, Hocke AC, Zahlten J, Slevogt H, N′Guessan PD, Gunther S, Schmeck B, Hippenstiel S, Flieger A, Suttorp N, Opitz B 2008. NAIP and Ipaf control Legionella pneumophila replication in human cells. J Immunol 180:6808–6815. doi:.10.4049/jimmunol.180.10.6808 [PubMed] [Cross Ref]
32. Losick VP, Isberg RR 2006. NF-kB translocation prevents host cell death after low-dose challenge by Legionella pneumophila. J Exp Med 203:2177–2189. doi:.10.1084/jem.20060766 [PMC free article] [PubMed] [Cross Ref]
33. Shin S, Case CL, Archer KA, Nogueira CV, Kobayashi KS, Flavell RA, Roy CR, Zamboni DS 2008. Type IV secretion-dependent activation of host MAP kinases induces an increased proinflammatory cytokine response to Legionella pneumophila. PLoS Pathog 4:e1000220. doi:.10.1371/journal.ppat.1000220 [PMC free article] [PubMed] [Cross Ref]
34. Welsh CT, Summersgill JT, Miller RD 2004. Increases in c-Jun N-terminal kinase/stress-activated protein kinase and p38 activity in monocyte-derived macrophages following the uptake of Legionella pneumophila. Infect Immun 72:1512–1518. doi:.10.1128/IAI.72.3.1512-1518.2004 [PMC free article] [PubMed] [Cross Ref]
35. Abu-Zant A, Jones S, Asare R, Suttles J, Price C, Graham J, Kwaik YA 2007. Anti-apoptotic signalling by the Dot/Icm secretion system of Legionella pneumophila. Cell Microbiol 9:246–264. doi:.10.1111/j.1462-5822.2006.00785.x [PubMed] [Cross Ref]
36. Bartfeld S, Engels C, Bauer B, Aurass P, Flieger A, Bruggemann H, Meyer TF 2009. Temporal resolution of two-tracked NF-kB activation by Legionella pneumophila. Cell Microbiol 11:1638–1651. doi:.10.1111/j.1462-5822.2009.01354.x [PubMed] [Cross Ref]
37. Ge J, Xu H, Li T, Zhou Y, Zhang Z, Li S, Liu L, Shao F 2009. A Legionella type IV effector activates the NF-kB pathway by phosphorylating the IkB family of inhibitors. Proc Natl Acad Sci U S A 106:13725–13730. doi:.10.1073/pnas.0907200106 [PubMed] [Cross Ref]
38. Losick VP, Haenssler E, Moy MY, Isberg RR 2010. LnaB: a Legionella pneumophila activator of NF-kB. Cell Microbiol 12:1083–1097. doi:.10.1111/j.1462-5822.2010.01452.x [PMC free article] [PubMed] [Cross Ref]
39. Simon S, Hilbi H 2015. Subversion of cell-autonomous immunity and cell migration by Legionella pneumophila effectors. Front Immunol 6:447. doi:.10.3389/fimmu.2015.00447 [PMC free article] [PubMed] [Cross Ref]
40. Archer KA, Ader F, Kobayashi KS, Flavell RA, Roy CR 2010. Cooperation between multiple microbial pattern recognition systems is important for host protection against the intracellular pathogen Legionella pneumophila. Infect Immun 78:2477–2487. doi:.10.1128/IAI.00243-10 [PMC free article] [PubMed] [Cross Ref]
41. Berrington WR, Iyer R, Wells RD, Smith KD, Skerrett SJ, Hawn TR 2010. NOD1 and NOD2 regulation of pulmonary innate immunity to Legionella pneumophila. Eur J Immunol 40:3519–3527. doi:.10.1002/eji.201040518 [PMC free article] [PubMed] [Cross Ref]
42. Frutuoso MS, Hori JI, Pereira MSF, Junior DSL, Sonego F, Kobayashi KS, Flavell RA, Cunha FQ, Zamboni DS 2010. The pattern recognition receptors Nod1 and Nod2 account for neutrophil recruitment to the lungs of mice infected with Legionella pneumophila. Microbes Infect 12:819–827. doi:.10.1016/j.micinf.2010.05.006 [PubMed] [Cross Ref]
43. Liu M, Conover GM, Isberg RR 2008. Legionella pneumophila EnhC is required for efficient replication in tumor necrosis factor a-stimulated macrophages. Cell Microbiol 10:1906–1923. doi:.10.1111/j.1462-5822.2008.01180.x [PMC free article] [PubMed] [Cross Ref]
44. Caruso R, Warner N, Inohara N, Nunez G 2014. NOD1 and NOD2: signaling, host defense, and inflammatory disease. Immunity 41:898–908. doi:.10.1016/j.immuni.2014.12.010 [PMC free article] [PubMed] [Cross Ref]
45. Motta V, Soares F, Sun T, Philpott DJ 2015. NOD-like receptors: versatile cytosolic sentinels. Physiol Rev 95:149–178. doi:.10.1152/physrev.00009.2014 [PubMed] [Cross Ref]
46. Chiu YH, Macmillan JB, Chen ZJ 2009. RNA polymerase III detects cytosolic DNA and induces type I interferons through the RIG-I pathway. Cell 138:576–591. doi:.10.1016/j.cell.2009.06.015 [PMC free article] [PubMed] [Cross Ref]
47. Lippmann J, Rothenburg S, Deigendesch N, Eitel J, Meixenberger K, van Laak V, Slevogt H, N′Guessan PD, Hippenstiel S, Chakraborty T, Flieger A, Suttorp N, Opitz B 2008. IFNb responses induced by intracellular bacteria or cytosolic DNA in different human cells do not require ZBP1 (DLM-1/DAI). Cell Microbiol 10:2579–2588. doi:.10.1111/j.1462-5822.2008.01232.x [PubMed] [Cross Ref]
48. McNab F, Mayer-Barber K, Sher A, Wack A, O'Garra A 2015. Type I interferons in infectious disease. Nat Rev Immunol 15:87–103. doi:.10.1038/nri3787 [PubMed] [Cross Ref]
49. Monroe KM, McWhirter SM, Vance RE 2009. Identification of host cytosolic sensors and bacterial factors regulating the type I interferon response to Legionella pneumophila. PLoS Pathog 5:e1000665. doi:.10.1371/journal.ppat.1000665 [PMC free article] [PubMed] [Cross Ref]
50. Opitz B, Vinzing M, van Laak V, Schmeck B, Heine G, Gunther S, Preissner R, Slevogt H, N′Guessan PD, Eitel J, Goldmann T, Flieger A, Suttorp N, Hippenstiel S 2006. Legionella pneumophila induced IFN-b in lung epithelial cells via IPS-1 and IRF3, which also control bacterial replication. J Biol Chem 281:36173–36179. doi:.10.1074/jbc.M604638200 [PubMed] [Cross Ref]
51. Plumlee CR, Lee C, Beg AA, Decker T, Shuman HA, Schindler C 2009. Interferons direct an effective innate response to Legionella pneumophila infection. J Biol Chem 284:30058–30066. doi:.10.1074/jbc.M109.018283 [PMC free article] [PubMed] [Cross Ref]
52. Stetson DB, Medzhitov R 2006. Recognition of cytosolic DNA activates an IRF3-dependent innate immune response. Immunity 24:93–103. doi:.10.1016/j.immuni.2005.12.003 [PubMed] [Cross Ref]
53. Case CL, Kohler LJ, Lima JB, Strowig T, de Zoete MR, Flavell RA, Zamboni DS, Roy CR 2013. Caspase-11 stimulates rapid flagellin-independent pyroptosis in response to Legionella pneumophila. Proc Natl Acad Sci U S A 110:1851–1856. doi:.10.1073/pnas.1211521110 [PubMed] [Cross Ref]
54. Case CL, Shin S, Roy CR 2009. Asc and Ipaf inflammasomes direct distinct pathways for caspase-1 activation in response to Legionella pneumophila. Infect Immun 77:1981–1991. doi:.10.1128/IAI.01382-08 [PMC free article] [PubMed] [Cross Ref]
55. Casson CN, Yu J, Reyes VM, Taschuk FO, Yadav A, Copenhaver AM, Nguyen HT, Collman RG, Shin S 2015. Human caspase-4 mediates noncanonical inflammasome activation against gram-negative bacterial pathogens. Proc Natl Acad Sci U S A 112:6688–6693. doi:.10.1073/pnas.1421699112 [PubMed] [Cross Ref]
56. Ge J, Gong YN, Xu Y, Shao F 2012. Preventing bacterial DNA release and absent in melanoma 2 inflammasome activation by a Legionella effector functioning in membrane trafficking. Proc Natl Acad Sci U S A 109:6193–6198. doi:.10.1073/pnas.1117490109 [PubMed] [Cross Ref]
57. Lage SL, Longo C, Branco LM, da Costa TB, Buzzo CDL, Bortoluci KR 2014. Emerging concepts about NAIP/NLRC4 inflammasomes. Front Immunol 5:309. doi:.10.3389/fimmu.2014.00309 [PMC free article] [PubMed] [Cross Ref]
58. Khare S, Dorfleutner A, Bryan NB, Yun C, Radian AD, de Almeida L, Rojanasakul Y, Stehlik C 2012. An NLRP7-containing inflammasome mediates recognition of microbial lipopeptides in human macrophages. Immunity 36:464–476. doi:.10.1016/j.immuni.2012.02.001 [PMC free article] [PubMed] [Cross Ref]
59. Shi J, Zhao Y, Wang Y, Gao W, Ding J, Li P, Hu L, Shao F 2014. Inflammatory caspases are innate immune receptors for intracellular LPS. Nature 514:187–192. doi:.10.1038/nature13683 [PubMed] [Cross Ref]
60. Bryan NB, Dorfleutner A, Rojanasakul Y, Stehlik C 2009. Activation of inflammasomes requires intracellular redistribution of the apoptotic speck-like protein containing a caspase recruitment domain. J Immunol 182:3173–3182. doi:.10.4049/jimmunol.0802367 [PMC free article] [PubMed] [Cross Ref]
61. Garcia MA, Meurs EF, Esteban M 2007. The dsRNA protein kinase PKR: virus and cell control. Biochimie 89:799–811. doi:.10.1016/j.biochi.2007.03.001 [PubMed] [Cross Ref]
62. Gray JS, Bae HK, Li JC, Lau AS, Pestka JJ 2008. Double-stranded RNA-activated protein kinase mediates induction of interleukin-8 expression by deoxynivalenol, Shiga toxin 1, and ricin in monocytes. Toxicol Sci 105:322–330. doi:.10.1093/toxsci/kfn128 [PMC free article] [PubMed] [Cross Ref]
63. Fontana MF, Shin S, Vance RE 2012. Activation of host mitogen-activated protein kinases by secreted Legionella pneumophila effectors that inhibit host protein translation. Infect Immun 80:3570–3575. doi:.10.1128/IAI.00557-12 [PMC free article] [PubMed] [Cross Ref]
64. Akamine M, Higa F, Arakaki N, Kawakami K, Takeda K, Akira S, Saito A 2005. Differential roles of Toll-like receptors 2 and 4 in in vitro responses of macrophages to Legionella pneumophila. Infect Immun 73:352–361. doi:.10.1128/IAI.73.1.352-361.2005 [PMC free article] [PubMed] [Cross Ref]
65. Archer KA, Alexopoulou L, Flavell RA, Roy CR 2009. Multiple MyD88-dependent responses contribute to pulmonary clearance of Legionella pneumophila. Cell Microbiol 11:21–36. doi:.10.1111/j.1462-5822.2008.01234.x [PMC free article] [PubMed] [Cross Ref]
66. Fuse ET, Tateda K, Kikuchi Y, Matsumoto T, Gondaira F, Azuma A, Kudoh S, Standiford TJ, Yamaguchi K 2007. Role of Toll-like receptor 2 in recognition of Legionella pneumophila in a murine pneumonia model. J Med Microbiol 56:305–312. doi:.10.1099/jmm.0.46913-0 [PubMed] [Cross Ref]
67. Girard R, Pedron T, Uematsu S, Balloy V, Chignard M, Akira S, Chaby R 2003. Lipopolysaccharides from Legionella and Rhizobium stimulate mouse bone marrow granulocytes via Toll-like receptor 2. J Cell Sci 116:293–302. doi:.10.1242/jcs.00212 [PubMed] [Cross Ref]
68. Hawn TR, Verbon A, Lettinga KD, Zhao LP, Li SS, Laws RJ, Skerrett SJ, Beutler B, Schroeder L, Nachman A, Ozinsky A, Smith KD, Aderem A 2003. A common dominant TLR5 stop codon polymorphism abolishes flagellin signaling and is associated with susceptibility to Legionnaires' disease. J Exp Med 198:1563–1572. doi:.10.1084/jem.20031220 [PMC free article] [PubMed] [Cross Ref]
69. Newton CA, Perkins I, Widen RH, Friedman H, Klein TW 2007. Role of Toll-like receptor 9 in Legionella pneumophila-induced interleukin-12 p40 production in bone marrow-derived dendritic cells and macrophages from permissive and nonpermissive mice. Infect Immun 75:146–151. doi:.10.1128/IAI.01011-06 [PMC free article] [PubMed] [Cross Ref]
70. Brubaker SW, Bonham KS, Zanoni I, Kagan JC 2015. Innate immune pattern recognition: a cell biological perspective. Annu Rev Immunol 33:257–290. doi:.10.1146/annurev-immunol-032414-112240 [PMC free article] [PubMed] [Cross Ref]
71. Wang JQ, Jeelall YS, Ferguson LL, Horikawa K 2014. Toll-like receptors and cancer: MYD88 mutation and inflammation. Front Immunol 5:367. doi:.10.3389/fimmu.2014.00367 [PMC free article] [PubMed] [Cross Ref]
72. Everts B, Amiel E, Huang SC, Smith AM, Chang CH, Lam WY, Redmann V, Freitas TC, Blagih J, van der Windt GJ, Artyomov MN, Jones RG, Pearce EL, Pearce EJ 2014. TLR-driven early glycolytic reprogramming via the kinases TBK1-IKK epsilon supports the anabolic demands of dendritic cell activation. Nat Immunol 15:323–332. doi:.10.1038/ni.2833 [PMC free article] [PubMed] [Cross Ref]
73. Lettinga KD, Florquin S, Speelman P, van Ketel R, van der Poll T, Verbon A 2002. Toll-like receptor 4 is not involved in host defense against pulmonary Legionella pneumophila infection in a mouse model. J Infect Dis 186:570–573. doi:.10.1086/341780 [PubMed] [Cross Ref]
74. Reddick LE, Alto NM 2014. Bacteria fighting back: how pathogens target and subvert the host innate immune system. Mol Cell 54:321–328. doi:.10.1016/j.molcel.2014.03.010 [PMC free article] [PubMed] [Cross Ref]
75. Regueiro V, Moranta D, Frank CG, Larrarte E, Margareto J, March C, Garmendia J, Bengoechea JA 2011. Klebsiella pneumoniae subverts the activation of inflammatory responses in a NOD1-dependent manner. Cell Microbiol 13:135–153. doi:.10.1111/j.1462-5822.2010.01526.x [PubMed] [Cross Ref]
76. Rosadini CV, Kagan JC 2015. Microbial strategies for antagonizing Toll-like-receptor signal transduction. Curr Opin Immunol 32:61–70. doi:.10.1016/j.coi.2014.12.011 [PMC free article] [PubMed] [Cross Ref]
77. Shim HK, Kim JY, Kim MJ, Sim HS, Park DW, Sohn JW, Kim MJ 2009. Legionella lipoprotein activates Toll-like receptor 2 and induces cytokine production and expression of costimulatory molecules in peritoneal macrophages. Exp Mol Med 41:687–694. doi:.10.3858/emm.2009.41.10.075 [PMC free article] [PubMed] [Cross Ref]
78. Grabiec A, Meng G, Fichte S, Bessler W, Wagner H, Kirschning CJ 2004. Human but not murine Toll-like receptor 2 discriminates between tri-palmitoylated and tri-lauroylated peptides. J Biol Chem 279:48004–48012. doi:.10.1074/jbc.M405311200 [PubMed] [Cross Ref]
79. Erwin AL, Mandrell RE, Munford RS 1991. Enzymatically deacylated Neisseria lipopolysaccharide (LPS) inhibits murine splenocyte mitogenesis induced by LPS. Infect Immun 59:1881–1887. [PMC free article] [PubMed]
80. Kawasaki K, Ernst RK, Miller SI 2004. Deacylation and palmitoylation of lipid A by Salmonellae outer membrane enzymes modulate host signaling through Toll-like receptor 4. J Endotoxin Res 10:439–444. doi:.10.1177/09680519040100061001 [PubMed] [Cross Ref]
81. Lu M, Zhang M, Takashima A, Weiss J, Apicella MA, Li XH, Yuan D, Munford RS 2005. Lipopolysaccharide deacylation by an endogenous lipase controls innate antibody responses to Gram-negative bacteria. Nat Immunol 6:989–994. doi:.10.1038/ni1246 [PubMed] [Cross Ref]
82. Shao B, Lu M, Katz SC, Varley AW, Hardwick J, Rogers TE, Ojogun N, Rockey DC, Dematteo RP, Munford RS 2007. A host lipase detoxifies bacterial lipopolysaccharides in the liver and spleen. J Biol Chem 282:13726–12735. doi:.10.1074/jbc.M609462200 [PubMed] [Cross Ref]
83. Trent MS, Pabich W, Raetz CR, Miller SI 2001. A PhoP/PhoQ-induced lipase (PagL) that catalyzes 3-O-deacylation of lipid A precursors in membranes of Salmonella typhimurium. J Biol Chem 276:9083–9092. doi:.10.1074/jbc.M010730200 [PubMed] [Cross Ref]
84. Marre ML, Petnicki-Ocwieja T, DeFrancesco AS, Darcy CT, Hu LT 2010. Human integrin alpha(3)beta(1) regulates TLR2 recognition of lipopeptides from endosomal compartments. PLoS One 5:e12871. doi:.10.1371/journal.pone.0012871 [PMC free article] [PubMed] [Cross Ref]
85. Petnicki-Ocwieja T, Kern A, Killpack TL, Bunnell SC, Hu LT 2015. Adaptor protein-3-mediated trafficking of TLR2 ligands controls specificity of inflammatory responses but not adaptor complex assembly. J Immunol 195:4331–4340. doi:.10.4049/jimmunol.1501268 [PMC free article] [PubMed] [Cross Ref]
86. Rechnitzer C, Williams A, Wright JB, Dowsett AB, Milman N, Fitzgeorge RB 1992. Demonstration of the intracellular production of tissue-destructive protease by Legionella pneumophila multiplying within guinea-pig and human alveolar macrophages. J Gen Microbiol 138:1671–1677. doi:.10.1099/00221287-138-8-1671 [PubMed] [Cross Ref]
87. Broz P, Monack DM 2013. Newly described pattern recognition receptors team up against intracellular pathogens. Nat Rev Immunol 13:551–565. doi:.10.1038/nri3479 [PubMed] [Cross Ref]
88. Tam JC, Jacques DA 2014. Intracellular immunity: finding the enemy within—how cells recognize and respond to intracellular pathogens. J Leukoc Biol 96:233–244. doi:.10.1189/jlb.4RI0214-090R [PMC free article] [PubMed] [Cross Ref]
89. Watson RO, Bell SL, MacDuff DA, Kimmey JM, Diner EJ, Olivas J, Vance RE, Stallings CL, Virgin HW, Cox JS 2015. The cytosolic sensor cGAS detects Mycobacterium tuberculosis DNA to induce type I interferons and activate autophagy. Cell Host Microbe 17:811–819. doi:.10.1016/j.chom.2015.05.004 [PMC free article] [PubMed] [Cross Ref]
90. Liles MR, Edelstein PH, Cianciotto NP 1999. The prepilin peptidase is required for protein secretion by and the virulence of the intracellular pathogen Legionella pneumophila. Mol Microbiol 31:959–970. doi:.10.1046/j.1365-2958.1999.01239.x [PubMed] [Cross Ref]
91. Stewart CR, Rossier O, Cianciotto NP 2009. Surface translocation by Legionella pneumophila: a form of sliding motility that is dependent upon type II protein secretion. J Bacteriol 191:1537–1546. doi:.10.1128/JB.01531-08 [PMC free article] [PubMed] [Cross Ref]
92. Edelstein PH. 1981. Improved semiselective medium for isolation of Legionella pneumophila from contaminated clinical and environmental specimens. J Clin Microbiol 14:298–303. [PMC free article] [PubMed]
93. Gunderson FF, Cianciotto NP 2013. The CRISPR-associated gene cas2 of Legionella pneumophila is required for intracellular infection of amoebae. mBio 4:e00074-13. doi:.10.1128/mBio.00074-13 [PMC free article] [PubMed] [Cross Ref]
94. Shi L, Hu LH, Li YR 2010. Autoimmune regulator regulates autophagy in THP-1 human monocytes. Front Med China 4:336–341. doi:.10.1007/s11684-010-0096-4 [PubMed] [Cross Ref]
95. Johnson WD Jr, Mei B, Cohn ZA 1977. The separation, long-term cultivation, and maturation of the human monocyte. J Exp Med 146:1613–1626. doi:.10.1084/jem.146.6.1613 [PMC free article] [PubMed] [Cross Ref]
96. Swanson MS, Isberg RR 1995. Association of Legionella pneumophila with the macrophage endoplasmic reticulum. Infect Immun 63:3609–3620. [PMC free article] [PubMed]
97. Gao LY, Harb OS, Kwaik YA 1998. Identification of macrophage-specific infectivity loci (mil) of Legionella pneumophila that are not required for infectivity of protozoa. Infect Immun 66:883–892. [PMC free article] [PubMed]
98. Polesky AH, Ross JT, Falkow S, Tompkins LS 2001. Identification of Legionella pneumophila genes important for infection of amoebas by signature-tagged mutagenesis. Infect Immun 69:977–987. doi:.10.1128/IAI.69.2.977-987.2001 [PMC free article] [PubMed] [Cross Ref]
99. Towbin H, Staehelin T, Gordon J 1979. Electrophoretic transfer of proteins from polyacrylamide gels to nitrocellulose sheets: procedure and some applications. Proc Natl Acad Sci U S A 76:4350–4354. doi:.10.1073/pnas.76.9.4350 [PubMed] [Cross Ref]
100. VanRheenen SM, Luo ZQ, O'Connor T, Isberg RR 2006. Members of a Legionella pneumophila family of proteins with ExoU (phospholipase A) active sites are translocated to target cells. Infect Immun 74:3597–3606. doi:.10.1128/IAI.02060-05 [PMC free article] [PubMed] [Cross Ref]
101. Sambrook J, Fritsch EF, Maniatis T 1989. Molecular cloning: a laboratory manual, 2nd ed Cold Spring Harbor Laboratory Press, Plainview, NY.
102. Wessel D, Flugge UI 1984. A method for the quantitative recovery of protein in dilute solution in the presence of detergents and lipids. Anal Biochem 138:141–143. doi:.10.1016/0003-2697(84)90782-6 [PubMed] [Cross Ref]

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