- Research article
- Open Access
Modulation of bacterial outer membrane vesicle production by envelope structure and content
© Schwechheimer et al.; licensee BioMed Central. 2014
- Received: 27 August 2014
- Accepted: 11 December 2014
- Published: 21 December 2014
Vesiculation is a ubiquitous secretion process of Gram-negative bacteria, where outer membrane vesicles (OMVs) are small spherical particles on the order of 50 to 250 nm composed of outer membrane (OM) and lumenal periplasmic content. Vesicle functions have been elucidated in some detail, showing their importance in virulence factor secretion, bacterial survival, and biofilm formation in pathogenesis. Furthermore, OMVs serve as an envelope stress response, protecting the secreting bacteria from internal protein misfolding stress, as well as external envelope stressors. Despite their important functional roles very little is known about the regulation and mechanism of vesicle production. Based on the envelope architecture and prior characterization of the hypervesiculation phenotypes for mutants lacking the lipoprotein, Lpp, which is involved in the covalent OM-peptidoglycan (PG) crosslinks, it is expected that an inverse relationship exists between OMV production and PG-crosslinked Lpp.
In this study, we found that subtle modifications of PG remodeling and crosslinking modulate OMV production, inversely correlating with bound Lpp levels. However, this inverse relationship was not found in strains in which OMV production is driven by an increase in “periplasmic pressure” resulting from the accumulation of protein, PG fragments, or lipopolysaccharide. In addition, the characterization of an nlpA deletion in backgrounds lacking either Lpp- or OmpA-mediated envelope crosslinks demonstrated a novel role for NlpA in envelope architecture.
From this work, we conclude that OMV production can be driven by distinct Lpp concentration-dependent and Lpp concentration-independent pathways.
- Outer Membrane
- Outer Membrane Protein
- Periplasmic Protein
- Outer Membrane Vesicle
- Envelope Material
Outer membrane vesicles (OMVs) bud from the outer membrane (OM) of Gram-negative bacteria -. These spherical particles are composed of outer membrane entrapping lumenal periplasmic content  and have a diameter of around 50 to 250 nm, as visualized by electron and atomic force microscopy ,. Predominately, studies of OMV function have centered around topics related to pathogenesis, such as their role in the dissemination of virulence factors and genetic material, as well as degradation enzymes (proteases, hydrolases and lipases) which allow protection of an ecological niche and acquisition of nutrients in addition to the nucleation of biofilms ,-. OMV production is also an envelope stress response and a reduction in vesiculation under stressful conditions is harmful to the bacterial cells -. Our understanding of the mechanism and regulation of OMV production, however, remains extremely fragmented.
The Gram-negative envelope consists of a cytoplasmic or inner membrane (IM) and the OM, separated by the periplasmic space which contains the peptidoglycan (PG) sacculus . The OM of Gram-negative bacteria is asymmetric with the inner leaflet composed of phospholipids and the outer leaflet composed of lipopolysaccharide (LPS) -. The PG is a highly dynamic polymer, especially during cell growth and growth phase transitions . For envelope stability, the OM is tethered to the PG sacculus via an abundant OM lipoprotein, Lpp, by covalent crosslinking -.
It has been long-appreciated that the OM must dissociate from the underlying PG for an OMV bud to form ,. Indeed, the complete loss of envelope stabilizing factors leads to extremely high OMV production, although this is accompanied by a loss of membrane integrity and cellular leakage ,,. Since wild-type (WT) bacteria in normal and in inducing conditions, along with numerous hypervesiculation mutants, produce OMVs without compromising envelope stability ,,,-, a more moderate and regulated modulation of envelope structure must be present that can yield OMVs.
We hypothesized that alterations in the PG structure underlying the OM could be a means by which cells may modulate OMV production in either direction. This idea is strengthened by data demonstrating that the deletion of the amidase autolysin in Porphyromonas gingivalis, an enzyme that cleaves PG amide bonds, led to an increase in OMV production . The opposite effect, however, that increased crosslinking leads to hypovesiculation, has never been observed.
The IM lipoprotein, NlpA is one of very few envelope components that have been characterized and found to have a dominant effect on OMV production. It was previously established that the loss of NlpA caused decreased OMV production in an otherwise WT strain ,, and suppressed the protein accumulation-driven hypervesiculation phenotype of the ΔdegP mutant, which lacks the periplasmic protease/chaperone DegP .
In this study, we analyzed the effect on OMV production of mutations that alter PG structure and Lpp crosslinking. We were also curious whether bound Lpp levels dictate vesiculation levels for bacteria under inducing conditions, particularly those involving build-up of material in the periplasm. We investigated bound Lpp levels for mutants in which periplasmic misfolded protein, PG fragments, or LPS accumulation led to upregulated OMV production. Finally, we investigated the genetic interactions between nlpA and genes encoding envelope modifying and stabilizing proteins.
OMV production and Lpp crosslinking changes inversely with altered PG structure
Next, we examined the Lpp crosslinking levels of the ΔmepAΔdacBΔpbpG strain. We used an immunoblotting assay that allows us to distinguish between the PG crosslinked form of Lpp, and the OM lipid-anchored but uncrosslinked form of Lpp (historically referred to as the ‘bound’ and the ‘free’ form, respectively). As expected, we found an inverse relationship between OMV production and bound Lpp (Figure 1B). The amount of free Lpp was comparable to WT (Figure 1C), suggesting that the observed decrease is not a result of an overall decrease in Lpp.
We also investigated the L,D-transpeptidase ΔynhGΔycbB double mutant, which contains the common D-Alanine (D-Ala)-Diaminopimelic acid (DAP) peptide crosslinks but lacks the minor DAP-DAP crosslinks . We were especially interested in this strain in light of its relationship to Lpp crosslinking, since it had been shown that DAP-DAP muropeptides are enriched in covalently crosslinked Lpp . Interestingly, the loss of DAP-DAP crosslinks correlated with a strong hypovesiculation phenotype, ~ 60% lower than WT (Figure 1D). When examining the Lpp crosslinking levels of this mutant we found a significant increase in covalently attached Lpp (by ~ 2.6 fold, Figure 1E), whereas the concentration of free Lpp resembled WT levels (Figure 1C). It should be noted that this was the first strain in which we observed an increase in bound Lpp, demonstrating that bound Lpp levels can have a dynamic range in both directions. Taken together, these data suggest that the modulation of PG structure can alter the levels of OMV production in either direction via an inverse relationship to PG-Lpp crosslinking.
The inverse relationship between Lpp crosslinks and OMV production does not hold for mutants that accumulate periplasmic protein
Accumulation of PG fragments correlates with increased OMV production without altering Lpp crosslinking
We further examined vesiculation and envelope crosslinking in another case where envelope products accumulate in the periplasm. The ΔampG mutant lacks the IM permease AmpG, and this mutant is impaired in transporting muropeptides from the periplasm to the cytoplasm for PG recycling . We utilized the ΔampGΔamiD double mutant which also lacks the amidase AmiD, causing large PG fragments to accumulate in the periplasm because they are also too large to fit through the porins . When we examined OMV production, we determined that the ΔampGΔamiD mutant exhibited ~ 14-fold increased OMV production with respect to WT (Figure 2C). These data supported the hypothesis that periplasmic accumulation of PG fragments caused their subsequent shedding into the medium via OMVs. Direct verification and quantitation of PG fragments in the OMVs is extremely challenging, technically, and therefore was not able to be determined in the scope of this study. To investigate the state of the envelope for this strain, free and crosslinked Lpp levels were measured. No difference in the levels of bound or free Lpp were found for the ΔampGΔamiD mutant and the WT strain (Figure 2A and B). In sum, a mutant in which PG fragments accumulate in the periplasm hypervesiculates without exhibiting altered total levels of Lpp crosslinking, similar to the effect when protein accumulation drives vesiculation.
LPS accumulation also leads to hypervesiculation without modulating bound Lpp concentration
We next reasoned that accumulation of LPS fragments could generate a similar effect to induce OMV production as either the accumulation of PG fragments or periplasmic protein. Data published recently indicate that individual mutations that alter the sugar core structure of LPS (ΔrfaC, ΔrfaG, and ΔrfaP) lead to periplasmic LPS accumulation due to the disruption of LPS maturation in the envelope of the cell . Additional evidence further supports the concept of periplasmic LPS accumulation: rfaC and rfaG mutant strains contain an increased amount of LPS in comparison to WT ,, and furthermore increasing LPS production leads to abnormal structures in the periplasm, implying that LPS overproduction results in a reduction of proper, OM-localized LPS, but not a reduction in the overall amount of LPS in the envelope .
Next, we determined the amount of covalently crosslinked Lpp in these LPS mutants in order to see if these inversely correlated with the OMV phenotypes. Covalent Lpp crosslinking was unchanged with respect to WT for ΔrfaC; ΔrfaG and ΔrfaP exhibited a slight reduction, albeit not statistically significant (Figure 3C). In control experiments, the amount of free Lpp in the strains was also not significantly different from WT (Figure 3D). These results support the hypothesis that OMV production in these LPS mutants is predominantly driven by accumulated material rather than a decrease in overall covalent Lpp crosslinking.
To test our model that the accumulation of mislocalized envelope lipid in the cell leads to its secretion via OMVs, we assessed whether OMVs produced by these LPS mutants were enriched in lipid. We quantified the lipids in OMVs using a lipophilic dye (FM4-64) that becomes fluorescent upon membrane intercalation. These values were then divided by the quantity of OMPs in the OMVs from each of the strains. The results show a four-fold increase in the lipid to OMP ratio for ΔrfaC OMVs, a 15-fold increase for ΔrfaG, and a 29-fold increase for ΔrfaP OMVs, with respect to the WT OMV control, confirming lipid accumulation in the OMVs of ΔrfaC, ΔrfaG, and ΔrfaP (Figure 3E). These data strongly support the idea that accumulated lipid, LPS, is in the secreted OMVs.
A complex role for NlpA in envelope architecture
To further investigate the envelope architecture of periplasmic accumulation-induced hypervesiculating mutants, we tested the effect of deleting nlpA in those strains. The loss of the IM lipoprotein, NlpA, decreases OMV production in an otherwise WT strain , and suppresses the hypervesiculation phenotypes of the protein-accumulating, ΔdegP mutant . Interestingly, however, the ΔnlpA mutation was not epistatic to ΔampGΔamiD, and the ΔnlpAΔrfaP double mutant still produced a significantly increased amount of OMVs (Figures 2C and 3F). These data suggested that membrane architecture differs for hypervesiculating strains containing different accumulated periplasmic products.
We also examined whether the loss of nlpA showed genetic interactions with other envelope stabilizing factors. Previous genetic and crosslinking studies have shown that there is an interaction between Lpp and OmpA ,,, an OM β-barrel protein with a periplasmic PG-interaction domain ,. A deletion in ompA, which encodes OmpA, resulted in ~26-fold hypervesiculation (Figure 4C), consistent with the phenotypes of the ΔompA Salmonella and Vibrio cholerae mutants ,. We tested if the nlpA deletion was epistatic to ΔompA. Similar to the results for the triple L,D-transpeptidase mutant, the ΔnlpA mutation also exacerbated the ΔompA hypervesiculation phenotypes in both overnight (Figure 4C) and log phase cultures (Figure 4D). Together, these data support a complex role for NlpA, depending on envelope conditions. Specifically, NlpA is critical to the ability to increase OMVs in conditions of protein, but not PG fragment and lipid accumulation, and the loss of NlpA increases hypervesiculation when levels of envelope stabilizing factors are decreased.
Fine-tuning of OMV production through PG biosynthesis and structure
The level of Lpp crosslinking was investigated for mutants with moderate PG structure effects that also exhibited increased and decreased levels of vesiculation. Here we report that the triple endopeptidase deletion mutant hypervesiculates and exhibits a decrease in covalent Lpp crosslinking (Figure 1B). This hypervesiculation phenotype was notably consistent with the previous P. gingivalis endopeptidase mutant . The opposite situation was found with the loss of the genes responsible for the minor DAP-DAP PG crosslinks (ΔynhGΔycbB). In this mutant, OMV production is lower than WT (Figure 1D), with a concomitant increase in bound Lpp (Figure 1E). These data support a model in which PG dynamics directly modulate the number of covalent envelope crosslinks and, thereby, indirectly modulate OMV production (Figure 5A).
The increase in bound Lpp for the ΔynhGΔycbB strain was particularly interesting in light of a previous report which showed that PG-Lpp crosslinks are enriched at sites of DAP-DAP crosslinks . We hypothesize that either DAP-DAP crosslinks could serve as “location markers” for crosslinking of Lpp and that in the absence of these markers, Lpp crosslinking to the PG is more random and more distributed across the PG sacculus, or alternatively, that the residues typically involved in the DAP-DAP crosslinks may be utilized for Lpp crosslinking in this mutant.
OMV production relieves stress caused by the accumulation of diverse, potentially harmful products in the envelope
Here we demonstrate that the accumulation of periplasmic PG fragments and LPS leads to an increase in OMV production. These data are consistent with the previously described role of OMVs in relieving protein-mediated envelope stress induced by a σE-stimulating model misfolded polypeptide and the lack of the DegP protease ,. In addition, we detected increased ratios of lipid:protein in LPS mutant strain OMVs, which indicates accumulated LPS cargo enrichment in OMVs. Similarly, the σE-stimulating model misfolded polypeptide was enriched in OMVs, and misfolded DegP substrates were present in OMVs purified from the DegP protease-deficient strain ,. PG in OMVs from PG accumulating strains could not be detected due to technical limitations, however it should be mentioned that the ΔampGΔamiD mutant strain releases large PG fragments into the cell-free medium , and since these are too large to diffuse through the OM porins, this observation is consistent with their secretion via OMVs.
We have previously found that vesiculation enhances survival in cases of periplasmic protein accumulation , and can now extend this model to include the shedding of LPS via OMVs. Very recently, YciM was identified as a negative regulator of LPS biosynthesis, and an excess of LPS was confirmed to be responsible for the death of yciM mutants . Interestingly, they report that suppressor mutations include those that either downregulate LPS biosynthesis via other routes, or they are part of a group of genes that is involved in OM assembly or organization (lpp, rfaP, ybcN, galU). Notably, all the mutants from the second group hypervesiculate (A. Kulp, A. Manning, B. Sun, T. Ai, D. Rodriguez, A. Schmidt, and M. Kuehn, unpublished data) ,.
These results further establish the general and important role OMV production plays in bacterial well-being, but we considered why bacteria do not simply expand their periplasm to accomodate the excess material without the concomitant loss of “macromolecular energy” that results from OMV release. In fact, it has been shown that the eukaryotic endoplasmic reticulum membrane expands to adapt to an increase in misfolded protein . The answer is straightforward when considering the bacterial envelope architecture: The OM and PG are connected by Lpp, a finite covalent crosslink. With such a constraint, either the concentration of misfolded/mislocalized envelope material could increase, the level of crosslinks could decrease, or the membrane could bulge out. High concentrations of material could become toxic to the proper function of the envelope cells ,, therefore this is not a viable option. Unlike the situation for PG structural mutants, overall bound Lpp levels do not change under conditions of periplasmic accumulation, suggesting more localized changes in the envelope architecture were responsible for OMV generation (see model, Figure 5B). Apparently, the trapped periplasmic material cannot prevent the formation of bound Lpp, but instead pushes the OM outward, either by taking advantage of “nanoterritories” of OM containing locally decreased levels of bound Lpp, or by displacing bound Lpp to sites on the periphery of the outwardly bulging OM. Subsequent spontaneous membrane fusion events, could then result in OMV budding and release.
The contribution of NlpA to envelope architecture
The data demonstrating that the loss of nlpA increased OMV production in strains that were also missing the envelope stabilizing factors, bound Lpp and OmpA, (Figure 4) led us to hypothesize a structural role of the IM lipid-anchored protein, NlpA, within the envelope that depended on these other factors: NlpA could provide an IM-based scaffolding site to stabilize the sites of Lpp- and OmpA-based envelope crosslinks as depicted in our working model (Figure 5C). This is supported by the observations that NlpA is most critical during stationary phase , at a time when Lpp-PG crosslinking has been shown to increase . But, if NlpA helps to stabilize crosslinks, why would the ΔnlpA strain then have a hypovesiculation phenotype? We propose that other factors in the envelope that depend on bound Lpp or OmpA are overcompensating for the loss of nlpA in this mutant, creating a more tightly crosslinked envelope. Interestingly, the undervesiculation phenotype of the ΔnlpA strain is manifested in stationary phase, whereas the phenotypes presented in this work are already present in log phase, suggesting that the factor in the ΔnlpA strain that can (over)compensate for NlpA only appears late in the cell cycle. Notably, vesiculation levels did not change when nlpA was deleted in mutants that directly affect PG components (ΔampGΔamiD and ΔnlpI) (Figure 2C and Schwechheimer et al, ). Further work is necessary to fully elucidate the accessory role of NlpA in the envelope and in OMV biogenesis.
Implications for regulated OMV production by WT bacteria
In sum, these data reveal that OMV levels are not solely dictated by Lpp crosslinking; at least two mechanisms can alter OMV budding, one dependent on and the other independent of overall levels of Lpp crosslinking. Our results help us to understand how WT bacteria might regulate OMV levels in different situations and times in their life cycle. In the first, cells could use localized or cell-cycle (temporal) modulation of the PG structure by modifying the equilibrium between PG synthesis and degradation to affect overall bound Lpp and, consequently, OMV levels. In the other, bulk deposition of envelope material within the periplasm, as a result of a localized secretion apparatus or a stress response, could allow outward bulging of the OM and ultimately OMV release at areas with locally-reduced amounts of bound Lpp or by relocating bound Lpp. As a complex entity whose integrity must be preserved for the viability of the cell, the envelope is modulated by numerous other factors, such as OmpA and NlpA, which contribute in specific ways to the modulation of the envelope architecture. Although many of the envelope components studied here are conserved amongst other Gram-negative bacterial species, further investigation is required to understand whether these principles regarding the modulation of OMV production are also conserved in other species.
Growth conditions and reagents
Strains used in this study
rrnB3 ΔlacZ4787 hsdR514 Δ(araBAD)567Δ(rhaBAD)568 rph-1
WT of Keio collection (Baba et al. 2006 )
Keio collection single mutants
BW25113 with indicated single mutations: ΔnlpA::Kan, ΔdegP::Kan, ΔrfaC::Kan, ΔrfaG::Kan, ΔrfaP::Kan
(Baba et al. 2006 )
BW25113 ΔycfS, ΔybiS, ΔerfK::Kan
(Schwechheimer et al. 2013 )
BW25113 ΔampG, ΔamiD::Kan
BW25113 ΔampG, ΔnlpA, ΔamiD::Kan
BW25113 ΔpbpG, ΔdacB, ΔmepA::Kan
BW25113 ΔynhG, ΔycbB::Kan
BW25113 ΔycfS, ΔybiS, ΔerfK, ΔnlpA::Kan
BW25113 ΔnlpA, ΔompA::Kan
OMV purification and quantitation
Media (250 mL) was inoculated (1:250 dilution) from 37°C overnight cultures, and the bacterial cultures grown to an OD600 ~ 0.4 (for log phase) or grown overnight at 37°C (~16 h). Cells were pelleted with the Beckman Avanti J-25 centrifuge (JLA-10.500 rotor, 10 000 g, 10 min, 4°C) and the resulting supernatants filtered [low protein binding Durapore membrane, 0.45 μm polyvinylidene fluoride, Millipore]. Filtrates were centrifuged again with the Beckman Avanti J-25 centrifuge (JLA-16.250 rotor, 38 400 g, 3 h, 4°C) followed by another step of centrifugation with the Beckman Optima TLX Ultracentrifuge if the pellets were not visible. In these cases, most of the supernatant was poured off, and the region where pelleted material should be was “resuspended” in the residual supernatant and re-pelleted (TLA 100.3 rotor, 41 000 g, 1 h, 4°C). Pellets were resuspended in Dulbecco’s phosphate buffered saline with added salt (0.2 M NaCl) (DPBSS), and filter-sterilized through 0.45 μm Ultra-free spin filters (Millipore). A portion of the filtrate was plated on LB agar and incubated at 37°C overnight to verify that the suspensions were free of bacteria.
To quantitate OMV yield, OMV preparations were boiled for 6 min in 2× Laemelli buffer, separated by 15% SDS-PAGE, and stained with SYPRO Ruby Red (Molecular Probes) overnight in the dark. Prior to and after staining, the gel was fixed for 1 h in a solution of 10% MeOH and 7% acetic acid. Ruby-stained proteins were detected under UV light (Additional file 1: Figure S2 shows representative gels samples). E. coli Omps F/C and A were quantified by densitometry (NIH Image J software). The OMP density values were divided by the OD600 of the original culture to calculate OMV production and this value was divided by the OMV production of the WT or untreated control strain to determine relative fold OMV production. Measurements of OMV yield using FM4-64 was as described previously .
PG purification, digestion and quantitation of covalently crosslinked Lpp
Unless otherwise indicated, media (500 mL) was inoculated (1:250 dilution) from overnight 37°C bacterial cultures and cultures grown at 37°C until they reached OD600 ~ 0.4. PG was isolated from broth cultures based on the protocol by Lam et al. . Briefly, cells were pelleted and resuspended in PBS after which the ice-cold suspensions were dropped in an equal volume of vigorously stirring, boiling 10% SDS. Samples were boiled for 4 h and then incubated at 37°C, continuously shaking, overnight. The following day, the PG was pelleted with the Beckman Optima TLX Ultracentrifuge (TLA 100.3 rotor, 80 000 g, 15 min, 30°C), resuspended in 1% SDS followed by another 2 h of boiling. PG was washed four times with deionized water and finally resuspended in equal volumes of deionized water.
Equal fractions of the purified sacculi were digested with 15 mg/mL chicken egg lysozyme (Sigma-Aldrich) in 10 mM Tris–HCl, pH 8, at room temperature for 2 days. Lysozyme digested PG was separated by 15% SDS-PAGE and Lpp was detected by immunoblotting and quantified by densitometry (NIH Image J software). The Lpp density values were divided by the OD600 of the original culture to calculate the amount of Lpp that was covalently crosslinked to PG, and this value was divided by the PG-crosslinked Lpp of the WT strain to determine relative fold of bound Lpp. We chose to use cell density as the denominator for these experiments rather than the traditional total PG, since this calculation rather provides insights into the budding dynamics of the OM.
Quantitation of free Lpp
This method was adapted from Cowles et al. . A 5 ml culture was grown overnight (~16 hrs) in LB at 37°C. 1 ml of this culture was spun down in a microfuge (10 000 g, 4 min, room temperature), resuspended in 50 μl 1% SDS in PBS and 50 μl 2× Laemelli buffer. Samples were boiled for 10 min and separated by 15% SDS-PAGE. Free Lpp was detected by immunoblotting and quantified by densitometry (NIH Image J software). The free Lpp density values were divided by the OD600 of the original culture to calculate the amount of free Lpp, and this value was divided by the free Lpp of the WT control strain to determine relative fold of free Lpp.
Periplasmic protein content
Periplasm was isolated and quantified after overnight growth (37°C, 16–18 h) using a previously published protocol .
FM4-64 lipid analysis of OMVs
To determine the lipid to OMPs ratio within OMVs, one portion of the purified WT, ΔrfaC, ΔrfaG, and ΔrfaP OMVs were incubated with FM4-64 (Invitrogen), 3.3 g/ml in phosphate-buffered saline (PBS) for 10 min at 37°C. FM4-64 incubated in PBS was used as a negative control. The fluorescence signal was measured with a Molecular Devices SpectraMAX GeminiXS fluorometer (excitation: 506 nm, emission: 750 nm). To determine the OMPs concentration, a second portion of OMVs was treated as explained above under OMV purification and quantitation. Lastly the lipid value was divided by the OMP value and normalized to the WT strain.
Parameters used for the T-test are equal variance due to the comparison of identical experimental repetitions or unequal variance due to different experimental repetitions and a two-tail distribution. For direct sample size comparison, the paired T-test was used, and for fold comparison, the unpaired. The T-test value of ≤ 0.05 was considered statistically significant; if the value was lower than 0.05, the significance value is given under the corresponding data. The number of times each experiment was repeated (n) is stated in the figure legends.
This work was supported by NIH grant R01GM099471. We are grateful for the generous contributions of Tom Silhavy (Lpp antibody) and the National BioResource Project (NIG, Japan) for the E.coli Keio Collection.
- Berleman J, Auer M: The role of bacterial outer membrane vesicles for intra- and interspecies delivery. Environ Microbiol. 2013, 15 (2): 347-354. 10.1111/1462-2920.12048.View ArticlePubMedGoogle Scholar
- Deatherage BL, Cookson BT: Membrane vesicle release in bacteria, eukaryotes, and archaea: a conserved yet underappreciated aspect of microbial life. Infect Immun. 2012, 80 (6): 1948-1957. 10.1128/IAI.06014-11.PubMed CentralView ArticlePubMedGoogle Scholar
- Kulp A, Kuehn MJ: Biological functions and biogenesis of secreted bacterial outer membrane vesicles. Annu Rev Microbiol. 2010, 64: 163-184. 10.1146/annurev.micro.091208.073413.PubMed CentralView ArticlePubMedGoogle Scholar
- Schwechheimer C, Sullivan CJ, Kuehn MJ: Envelope control of outer membrane vesicle production in Gram-negative bacteria. Biochemistry. 2013, 52 (18): 3031-3040. 10.1021/bi400164t.PubMed CentralView ArticlePubMedGoogle Scholar
- Beveridge TJ: Structures of gram-negative cell walls and their derived membrane vesicles. J Bacteriol. 1999, 181 (16): 4725-4733.PubMed CentralPubMedGoogle Scholar
- MacDonald IA, Kuehn MJ: Offense and defense: microbial membrane vesicles play both ways. Res Microbiol. 2013, 163 (9–10): 607-618.Google Scholar
- Ellis TN, Kuehn MJ: Virulence and immunomodulatory roles of bacterial outer membrane vesicles. Microbiol Mol Biol Rev. 2010, 74 (1): 81-94. 10.1128/MMBR.00031-09.PubMed CentralView ArticlePubMedGoogle Scholar
- Schooling SR, Beveridge TJ: Membrane vesicles: an overlooked component of the matrices of biofilms. J Bacteriol. 2006, 188 (16): 5945-5957. 10.1128/JB.00257-06.PubMed CentralView ArticlePubMedGoogle Scholar
- Yonezawa H, Osaki T, Kurata S, Fukuda M, Kawakami H, Ochiai K, Hanawa T, Kamiya S: Outer membrane vesicles of Helicobacter pylori TK1402 are involved in biofilm formation. BMC Microbiol. 2009, 9: 197-10.1186/1471-2180-9-197.PubMed CentralView ArticlePubMedGoogle Scholar
- McMahon KJ, Castelli ME, Vescovi EG, Feldman MF: Biogenesis of outer membrane vesicles in Serratia marcescens is thermoregulated and can be induced by activation of the Rcs phosphorelay system. J Bacteriol. 2012, 194 (12): 3241-3249. 10.1128/JB.00016-12.PubMed CentralView ArticlePubMedGoogle Scholar
- Maredia R, Devineni N, Lentz P, Dallo SF, Yu J, Guentzel N, Chambers J, Arulanandam B, Haskins WE, Weitao T: Vesiculation from Pseudomonas aeruginosa under SOS. Sci World J. 2012, 2012: 402919-10.1100/2012/402919.View ArticleGoogle Scholar
- McBroom AJ, Kuehn MJ: Release of outer membrane vesicles by Gram-negative bacteria is a novel envelope stress response. Mol Microbiol. 2007, 63 (2): 545-558. 10.1111/j.1365-2958.2006.05522.x.PubMed CentralView ArticlePubMedGoogle Scholar
- Manning AJ, Kuehn MJ: Contribution of bacterial outer membrane vesicles to innate bacterial defense. BMC Microbiol. 2011, 11: 258-10.1186/1471-2180-11-258.PubMed CentralView ArticlePubMedGoogle Scholar
- Manning AJ, Kuehn MJ: Functional advantages conferred by extracellular prokaryotic membrane vesicles. J Mol Microbiol Biotechnol. 2013, 23 (1–2): 131-141. 10.1159/000346548.PubMed CentralView ArticlePubMedGoogle Scholar
- Schwechheimer C, Kuehn MJ: Synthetic effect between envelope stress and lack of outer membrane vesicle production in Escherichia coli. J Bacteriol. 2013, 195 (18): 4161-4173. 10.1128/JB.02192-12.PubMed CentralView ArticlePubMedGoogle Scholar
- Tashiro Y, Sakai R, Toyofuku M, Sawada I, Nakajima-Kambe T, Uchiyama H, Nomura N: Outer membrane machinery and alginate synthesis regulators control membrane vesicle production in Pseudomonas aeruginosa. J Bacteriol. 2009, 191 (24): 7509-7519. 10.1128/JB.00722-09.PubMed CentralView ArticlePubMedGoogle Scholar
- Macdonald IA, Kuehn MJ: Stress-induced outer membrane vesicle production by Pseudomonas aeruginosa. J Bacteriol. 2013, 195 (13): 2971-2981. 10.1128/JB.02267-12.PubMed CentralView ArticlePubMedGoogle Scholar
- Silhavy TJ, Kahne D, Walker S: The bacterial cell envelope. Cold Spring Harb Perspect Biol. 2010, 2 (5): a000414-10.1101/cshperspect.a000414.PubMed CentralView ArticlePubMedGoogle Scholar
- Galloway SM, Raetz CR: A mutant of Escherichia coli defective in the first step of endotoxin biosynthesis. J Biol Chem. 1990, 265 (11): 6394-6402.PubMedGoogle Scholar
- Raetz CR: Biochemistry of endotoxins. Annu Rev Biochem. 1990, 59: 129-170. 10.1146/annurev.bi.59.070190.001021.View ArticlePubMedGoogle Scholar
- Raetz CR, Whitfield C: Lipopolysaccharide endotoxins. Annu Rev Biochem. 2002, 71: 635-700. 10.1146/annurev.biochem.71.110601.135414.PubMed CentralView ArticlePubMedGoogle Scholar
- Vollmer W, Bertsche U: Murein (peptidoglycan) structure, architecture and biosynthesis in Escherichia coli. Biochim Biophys Acta. 2008, 1778 (9): 1714-1734. 10.1016/j.bbamem.2007.06.007.View ArticlePubMedGoogle Scholar
- Cascales E, Bernadac A, Gavioli M, Lazzaroni JC, Lloubes R: Pal lipoprotein of Escherichia coli plays a major role in outer membrane integrity. J Bacteriol. 2002, 184 (3): 754-759. 10.1128/JB.184.3.754-759.2002.PubMed CentralView ArticlePubMedGoogle Scholar
- Braun V: Covalent lipoprotein from the outer membrane of Escherichia coli. Biochim Biophys Acta. 1975, 415 (3): 335-377. 10.1016/0304-4157(75)90013-1.View ArticlePubMedGoogle Scholar
- Braun V, Rehn K: Chemical characterization, spatial distribution and function of a lipoprotein (murein-lipoprotein) of the E. coli cell wall: the specific effect of trypsin on the membrane structure. Eur J Biochem. 1969, 10 (3): 426-438. 10.1111/j.1432-1033.1969.tb00707.x.View ArticlePubMedGoogle Scholar
- Wang Y: The function of OmpA in Escherichia coli. Biochem Biophys Res Commun. 2002, 292 (2): 396-401. 10.1006/bbrc.2002.6657.View ArticlePubMedGoogle Scholar
- Mashburn-Warren LM, Whiteley M: Special delivery: vesicle trafficking in prokaryotes. Mol Microbiol. 2006, 61 (4): 839-846. 10.1111/j.1365-2958.2006.05272.x.View ArticlePubMedGoogle Scholar
- Hoekstra D, van der Laan JW, de Leij L, Witholt B: Release of outer membrane fragments from normally growing Escherichia coli. Biochim Biophys Acta. 1976, 455 (3): 889-899. 10.1016/0005-2736(76)90058-4.View ArticlePubMedGoogle Scholar
- Deatherage BL, Lara JC, Bergsbaken T, Rassoulian Barrett SL, Lara S, Cookson BT: Biogenesis of bacterial membrane vesicles. Mol Microbiol. 2009, 72 (6): 1395-1407. 10.1111/j.1365-2958.2009.06731.x.PubMed CentralView ArticlePubMedGoogle Scholar
- Sonntag I, Schwarz H, Hirota Y, Henning U: Cell envelope and shape of Escherichia coli: multiple mutants missing the outer membrane lipoprotein and other major outer membrane proteins. J Bacteriol. 1978, 136 (1): 280-285.PubMed CentralPubMedGoogle Scholar
- McBroom AJ, Johnson AP, Vemulapalli S, Kuehn MJ: Outer membrane vesicle production by Escherichia coli is independent of membrane instability. J Bacteriol. 2006, 188 (15): 5385-5392. 10.1128/JB.00498-06.PubMed CentralView ArticlePubMedGoogle Scholar
- Fulsundar S, Harms K, Flaten GE, Johnsen PJ, Chopade BA, Nielsen KM: Gene transfer potential of outer membrane vesicles of Acinetobacter baylyi and effects of stress on vesiculation. Appl Environ Microbiol. 2014, 80 (11): 3469-3483. 10.1128/AEM.04248-13.PubMed CentralView ArticlePubMedGoogle Scholar
- Henry R, Lo M, Khoo C, Zhang H, Boysen RI, Picardeau M, Murray GL, Bulach DM, Adler B: Precipitation of iron on the surface of Leptospira interrogans is associated with mutation of the stress response metalloprotease HtpX. Appl Environ Microbiol. 2013, 79 (15): 4653-4660. 10.1128/AEM.01097-13.PubMed CentralView ArticlePubMedGoogle Scholar
- Hayashi J, Hamada N, Kuramitsu HK: The autolysin of Porphyromonas gingivalis is involved in outer membrane vesicle release. FEMS Microbiol Lett. 2002, 216 (2): 217-222. 10.1111/j.1574-6968.2002.tb11438.x.View ArticlePubMedGoogle Scholar
- Magnet S, Dubost L, Marie A, Arthur M, Gutmann L: Identification of the L, D-transpeptidases for peptidoglycan cross-linking in Escherichia coli. J Bacteriol. 2008, 190 (13): 4782-4785. 10.1128/JB.00025-08.PubMed CentralView ArticlePubMedGoogle Scholar
- Glauner B, Holtje JV, Schwarz U: The composition of the murein of Escherichia coli. J Biol Chem. 1988, 263 (21): 10088-10095.PubMedGoogle Scholar
- Jacobs C, Huang LJ, Bartowsky E, Normark S, Park JT: Bacterial cell wall recycling provides cytosolic muropeptides as effectors for beta-lactamase induction. EMBO J. 1994, 13 (19): 4684-4694.PubMed CentralPubMedGoogle Scholar
- Uehara T, Park JT: An anhydro-N-acetylmuramyl-L-alanine amidase with broad specificity tethered to the outer membrane of Escherichia coli. J Bacteriol. 2007, 189 (15): 5634-5641. 10.1128/JB.00446-07.PubMed CentralView ArticlePubMedGoogle Scholar
- Lima S, Guo MS, Chaba R, Gross CA, Sauer RT: Dual molecular signals mediate the bacterial response to outer-membrane stress. Science. 2013, 340 (6134): 837-841. 10.1126/science.1235358.PubMed CentralView ArticlePubMedGoogle Scholar
- Gmeiner J, Schlecht S: Molecular organization of the outer membrane of Salmonella typhimurium. Eur J Biochem. 1979, 93 (3): 609-620. 10.1111/j.1432-1033.1979.tb12861.x.View ArticlePubMedGoogle Scholar
- Klein G, Kobylak N, Lindner B, Stupak A, Raina S: Assembly of lipopolysaccharide in Escherichia coli requires the essential LapB heat shock protein. J Biol Chem. 2014, 289 (21): 14829-14853. 10.1074/jbc.M113.539494.PubMed CentralView ArticlePubMedGoogle Scholar
- Ogura T, Inoue K, Tatsuta T, Suzaki T, Karata K, Young K, Su LH, Fierke CA, Jackman JE, Raetz CR, Coleman J, Tomoyasu T, Matsuzawa H: Balanced biosynthesis of major membrane components through regulated degradation of the committed enzyme of lipid A biosynthesis by the AAA protease FtsH (HflB) in Escherichia coli. Mol Microbiol. 1999, 31 (3): 833-844. 10.1046/j.1365-2958.1999.01221.x.View ArticlePubMedGoogle Scholar
- Magnet S, Bellais S, Dubost L, Fourgeaud M, Mainardi JL, Petit-Frere S, Marie A, Mengin-Lecreulx D, Arthur M, Gutmann L: Identification of the L, D-transpeptidases responsible for attachment of the Braun lipoprotein to Escherichia coli peptidoglycan. J Bacteriol. 2007, 189 (10): 3927-3931. 10.1128/JB.00084-07.PubMed CentralView ArticlePubMedGoogle Scholar
- Pautsch A, Schulz GE: Structure of the outer membrane protein A transmembrane domain. Nat Struct Biol. 1998, 5 (11): 1013-1017. 10.1038/2983.View ArticlePubMedGoogle Scholar
- Choi DS, Yamada H, Mizuno T, Mizushima S: Trimeric structure and localization of the major lipoprotein in the cell surface of Escherichia coli. J Biol Chem. 1986, 261 (19): 8953-8957.PubMedGoogle Scholar
- Smith SG, Mahon V, Lambert MA, Fagan RP: A molecular Swiss army knife: OmpA structure, function and expression. FEMS Microbiol Lett. 2007, 273 (1): 1-11. 10.1111/j.1574-6968.2007.00778.x.View ArticlePubMedGoogle Scholar
- Moon DC, Choi CH, Lee JH, Choi CW, Kim HY, Park JS, Kim SI, Lee JC: Acinetobacter baumannii outer membrane protein A modulates the biogenesis of outer membrane vesicles. J Microbiol. 2012, 50 (1): 155-160. 10.1007/s12275-012-1589-4.View ArticlePubMedGoogle Scholar
- Valeru SP, Shanan S, Alossimi H, Saeed A, Sandstrom G, Abd H: Lack of outer membrane protein A enhances the release of outer membrane vesicles and survival of vibrio cholerae and suppresses viability of Acanthamoeba castellanii. Int J Microbiol. 2014, 2014: 610190-10.1155/2014/610190.PubMed CentralView ArticlePubMedGoogle Scholar
- Mahalakshmi S, Sunayana MR, Saisree L, Reddy M: yciM is an essential gene required for regulation of lipopolysaccharide synthesis in Escherichia coli. Mol Microbiol. 2013, 91 (1): 145-157. 10.1111/mmi.12452.View ArticlePubMedGoogle Scholar
- Schwechheimer C, Sullivan CJ, Kuehn MJ: Envelope control of outer membrane vesicle production in gram-negative bacteria. Biochemistry 2013, 52(18):3031–3040Google Scholar
- Sriburi R, Jackowski S, Mori K, Brewer JW: XBP1: a link between the unfolded protein response, lipid biosynthesis, and biogenesis of the endoplasmic reticulum. J Cell Biol. 2004, 167 (1): 35-41. 10.1083/jcb.200406136.PubMed CentralView ArticlePubMedGoogle Scholar
- Strauch KL, Johnson K, Beckwith J: Characterization of degP, a gene required for proteolysis in the cell envelope and essential for growth of Escherichia coli at high temperature. J Bacteriol. 1989, 171 (5): 2689-2696.PubMed CentralPubMedGoogle Scholar
- Baba T, Ara T, Hasegawa M, Takai Y, Okumura Y, Baba M, Datsenko KA, Tomita M, Wanner BL, Mori H: Construction of Escherichia coli K-12 in-frame, single-gene knockout mutants: the Keio collection. Mol Syst Biol. 2006, 2: 2006 0008-10.1038/msb4100050.PubMed CentralView ArticlePubMedGoogle Scholar
- Cherepanov PP, Wackernagel W: Gene disruption in Escherichia coli: TcR and KmR cassettes with the option of Flp-catalyzed excision of the antibiotic-resistance determinant. Gene. 1995, 158 (1): 9-14. 10.1016/0378-1119(95)00193-A.View ArticlePubMedGoogle Scholar
- Silhavy TJ, Berman ML, Enquist LW, Cold Spring Harbor Laboratory: Experiments With Gene Fusions. 1984, Cold Spring Harbor Laboratory, Cold Spring Harbor, N.YGoogle Scholar
- Lam H, Oh DC, Cava F, Takacs CN, Clardy J, de Pedro MA, Waldor MK: D-amino acids govern stationary phase cell wall remodeling in bacteria. Science. 2009, 325 (5947): 1552-1555. 10.1126/science.1178123.PubMed CentralView ArticlePubMedGoogle Scholar
- Cowles CE, Li Y, Semmelhack MF, Cristea IM, Silhavy TJ: The free and bound forms of Lpp occupy distinct subcellular locations in Escherichia coli. Mol Microbiol. 2011, 79 (5): 1168-1181. 10.1111/j.1365-2958.2011.07539.x.PubMed CentralView ArticlePubMedGoogle Scholar
- Schwechheimer C, Rodriguez DL, Kuehn MJ: NlpI-mediated modulation of outer membrane vesicle production through peptidoglycan dynamics in E.coli. MicrobiologyOpen, In press.,Google Scholar
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