The strains evaluated in this study consisted of 204 C. sakazakii, 12 C. turicensis, nine C. malonaticus, three C. dublinensis, and one strain each for C. muytjensii, C. universalis, and C. condimenti, which were obtained from the FDA laboratory culture collection. All these isolates were confirmed as Cronobacter species according to the proposed classification scheme as suggested by Iversen et al. (2008) and Joseph et al. (2012) using a Gram-negative card analyzed with the Vitek-2 Compact instrument (BioMerieux, Hazelwood, MO) and its version 5.03 software. Nine phylogenetically-related species representative of Salmonella enterica serovar Typhimurium, Klebsiella pneumoniae, Citrobacter freundii, Siccibacter turicensis, Franconibacter helveticus (two strains), and Franconibacter pulveris (two strains) were also included. All of the Cronobacter strains possessed the zinc metalloprotease (zpx) gene, a genus-specific target we previously reported (Kothary et al., 2007; Stephan et al., 2014). The species identity of the isolates was also confirmed using the species-specific rpoB PCR assays as described by Stoop et al. (2009) and Lehner et al. (2012) and the cgcA species-specific PCR assay as described by Carter et al. (2013). These 231 strains used in the study were isolated from clinical, food, or environmental sources and from diverse geographical locations and have been previously described by Franco et al., Yan et al., and Jarvis et al (Mullane et al., 2008; Franco et al., 2011; Jarvis et al., 2011, 2013; Yan et al., 2015a). The isolates were also subjected to RepF1B plasmidotyping (Franco et al., 2011) and molecular serogrouping (Mullane et al., 2008; Jarvis et al., 2011, 2013), the results of which further corroborated results of the rpoB- and cgcA- based PCR species identification assays.

Frozen bacterial cultures were stored at −80°C in Trypticase soy broth (BBL, Becton Dickinson, Franklin Lakes, NJ) supplemented with 1% NaCl (TSBS) and 50% glycerol. For propagation, frozen cultures were rapidly thawed and sub-cultured onto plates containing Trypticase soy agar (TSA, BBL) supplemented with 1% NaCl (TSAS) or Luria Bertani (LB) agar (LBA, BBL), and the plates were incubated for 16–18 h at 37°C.

Using a modification of the procedure described by Kwon et al. (2009) for the isolation of OMVs from Acinetobacter baumannii, OMVs were obtained from C. sakazakii strain BAA-894, C. malonaticus strain LMG23826^T and C. turicensis strain LMG23827^T by culturing these bacterial strains on TSAS and incubating the plates at 37°C for 18 h. The stationary phase grown cells were harvested in saline using a sterile plastic spreader, and the OMVs were isolated by differential centrifugation. Briefly, the cells and cellular debris were removed by centrifugation (10,000 × g for 15 min at 4°C), and OMVs contained in the resultant supernatant were further concentrated by ultracentrifugation at 150,000 × g for 3 h at 4°C. The pellets were suspended in 500 μl 20 mM Tris-HCl buffer (pH 8.0) and qualitatively assessed by electron microscopy and SDS-PAGE. Aside for the occasional flagellum, the OMVs observed in these preparations were similar to those observed in the original whole cell preparations.

Whole cell and the isolated OMV preparations were negatively stained and examined by electron microscopy. Whole cell suspensions were prepared in 0.5% sodium phosphotungstate (pH 6.8) and OMV suspensions were diluted 1:2 in 20 μl of a 1% (wt/vol) sodium phosphotungstate (pH 6.8) staining solution (final concentration was 0.5% sodium phosphotungstic acid). A single drop (containing approximately 15 μl) of the whole cell or OMV stained suspensions was then placed onto the surface of a 300 mesh, 0.25% Formvar-coated, carbon-coated copper grid (Electron Microscopy Sciences, Hatfield, PA). After drying for 1 min, excess fluid was removed from the grid surface with filter paper, and specimens were allowed to air dry before being examined in a JEOL 1011 transmission electron microscope (JEOL USA, Inc., Peabody, MA) operating at an accelerating voltage of 80 kV. Images were recorded using a Gatan model 785 side-mounted, ES1000W Erlangshen CCD camera using Digital Micrograph™ of the Gatan Microscopy Suite software version (Gatan, Inc., Pleasanton, CA).

SDS-PAGE was performed on OMV preparations (containing approximately 2.5–5 mg/ml protein) using 8–25% gradient gels in the PhastSystem (GE Healthcare, Piscataway, NJ). Molecular weights of the reduced and denatured OMV proteins from the three Cronobacter spp. were estimated by using the relative mobility method (Weber et al., 1972). Western blotting of OMV protein samples separated by SDS-PAGE was carried out by electro-blotting onto a Problott (Applied Biosystems, Foster City, CA) membrane in a transfer buffer (10 mM of 3-[cyclohexylamino]-1-propane sulfonic acid containing 10% methanol, pH 11).

The N-terminal amino acid sequences of the excised Coomassie blue-stained OMV protein bands from Western blots were determined by classical Edman degradation reactions using a Shimadzu PPSQ-33A Protein Sequencer (Columbia, MD). Computations for protein homology and identity analyses were performed using NCBI BLAST analysis.

Strains were grown overnight at 37°C in 5 ml of TSBS on an Innova shaker incubator (Eppendorf North America, Hauppauge, NY) at 160 rpm. Genomic DNA was purified from 2 ml of the culture using a robotic QIAcube workstation with its automated Qiagen DNeasy chemistry (Qiagen, Germantown, MD) following the manufacturer's recommendations. Typically, 5–15 μg of purified genomic DNA was recovered in a final elution volume of 200 μl. For PCR analysis, 1–2 μl of the genomic preparations were used as DNA templates. For microarray analysis, the purified DNA was further concentrated using an Amicon Ultracel-30 membrane filter (30,000 molecular weight cutoff, 0.5 ml, Millipore Corp. Billerica, MA) to a final volume of approximately 10–25 μl.

PCR primers specifically targeting the groEL, ompA, ompC, ompX, mipA genes, the conjugative plasmid transfer protein gene, and an outermembrane (OM) autotransporter protein gene(s) were designed by using NCBI Primer-BLAST software (Ye et al., 2012). PCR primer names, sequences, amplicon sizes, and gene target names are shown in Table 1. The primers used for the PCR amplification were synthesized by Integrated DNA Technologies (Coralville, IA). All PCR reactions were carried out using the GoTaq® Green Master Mix (Promega Corp., Madison, WI), which consisted of a 25 μl reaction mix having 1 unit of GoTaq Hotstart DNA polymerase, 1.5 mM MgCl₂, and 200 μM of each dNTP. Primers were added at 1 μM concentration each along with 1 μl of the genomic DNA (containing approximately 50 ng DNA/25 μl reaction) that served as a template. In all PCR reactions, the polymerase was activated by using a 3 min. incubation step at 94°C, followed by 25 cycles of denaturation at 94°C for 30 s and annealing and extension steps according to the PCR reaction parameters as described in Table 1. For each reaction, a final extension step of 5 min. at the cycle extension temperature was included.

The microarray used in this study is an Affymetrix MyGeneChip Custom Array (Affymetrix design number:FDACRONOa520845F) and was developed utilizing the whole genome sequences and 18 plasmids of 15 Cronobacter strains as previously described (Tall et al., 2015; Yan et al., 2015b).

Genomic DNA was fragmented by incubating at 37°C for 1 min. in a 20 μl reaction containing 1 × One-Phor-All Plus Buffer (GE Healthcare) and 0.01 units DNase I (GE Healthcare) as previously described (Jackson et al., 2011), and further modified by Tall et al. (2015). The fragmented DNA was heat-inactivated at 99°C for 15 min, and was 3′-end labeled by adding 4 μl of 5 × terminal transferase buffer (Promega), 1 μl 1 mM biotin-11-ddATP (PerkinElmer NEL508), and 2 μl (60 units) of terminal transferase enzyme (Promega). The labeling was carried out for 4 h at 37°C followed by heat inactivation at 98°C for 1 min.

Hybridizations were performed according to the Affymetrix GeneChip Expression Analysis Technical Manual for a 49-format array (Affymetrix, 2014). Following hybridization, wash and stain procedures were carried out on an Affymetrix FS-450 fluidics station using the mini_prok2v1_450 fluidics script (Affymetrix, 2014). Reagents for washing and staining were prepared according to the GeneChip® Expression Analysis Technical Manual (Affymetrix, 2014). The following modifications were made to the wash and stain procedure: Streptavidin solution mix (vial 1) was replaced with SAPE solution mix (Life Technologies, Grand Island, NY). Arrays were scanned using Affymetrix GeneChip® Scanner 3000 running on AGCC software.

For each OMV gene represented on the microarray, probe set intensities were summarized using the Robust MultiArray Averaging (RMA) function in the Affymetrix package of R-Bioconductor as previously described (Bolstad et al., 2003). Briefly, RMA summarization of probe level data was carried out by performing three individual treatments on all of the experimental data (CEL file) in succession. Firstly, probe specific correction of the perfect matched (PM) probes was done using a model based on the observed intensities being the sum of signal and noise. Secondly, quantile normalization was performed on the corrected PM probe intensities. Finally, a median polishing algorithm was used to summarize the background-corrected, normalized probe intensities to generate a final probe set value.

The closed genomes of C. sakazakii ATCC BAA-894 (BioProject Accession PRJNA12720), C. turicensis z3032 (BioProject Accession PRJEA39965) and the draft genome for C. malonaticus LMG 23826 (BioProject Accession PRJNA89099) were used as references to develop PCR primers for the OMP gene PCR analysis. The accession numbers of the Cronobacter strains used to develop the phylogenetic analysis of ompA can be found in Supplemental Table 1.

The generation of the first transmission electron photomicrograph of a bacterial cell is credited to Helmut Ruska, the brother of Nobel laureate Ernst Ruska (Knott and Genoud, 2013), who won the prize in 1986 for his work in electron optics, including the design of the first electron microscope. Though transmission electron microscopes were commercially available as early as 1939, it was not until the 1960s when researchers began to notice the presence of OMVs expressed by a variety of pathogenic Gram-negative bacteria including Vibrio cholerae, E. coli, and Bacteroides fragilis (Bladen and Waters, 1963; Bayer and Anderson, 1965; Chatterjee and Das, 1967; Knox et al., 1996; Kolling and Matthews, 1999; Chatterjee and Chaudhuri, 2011; Avila-Calderón et al., 2015; Kim et al., 2015). OMVs are thought to play several physiological and pathogenic functions in bacteria-bacteria and bacteria-host cell interactions however, as suggested by Schwechheimer and Kuehn they are not limited to just these roles (Schwechheimer and Kuehn, 2015). For example, Schwechheimer and Kuehn (2015) suggest that OMVs play functional roles in bacterial interactions with their environment(s), contributing to survival, nutrient acquisition, and ecological niche protection, including structural support in multispecies environments such as biofilms. TEM analysis of sodium phosphotungstate negatively-stained Cronobacter whole cell preparations showed an abundance of OMVs, and numerous OMVs were observed in these preparations, specifically as they cascaded off of each cell's surface onto the surface of the support grid (Figures 1A,B) or being pinched off of cell-associated membranous tendrils (Figure 1C). Occasionally, sheared and entrapped flagella were also seen in the OMV preparations. TEM evaluation of cells of all seven Cronobacter species produced similar OMVs (data not shown). Results of TEM analysis of partially isolated OMVs preparations from C. sakazakii strain BAA-894 (Figure 2) also demonstrates that the OMVs in these preparations were structurally similar to those observed in the negatively stained whole cell preparations. According to Mashburn-Warren and Whiteley, three main models for the expression and release of OMVs from the Gram-negative bacterial cell surface have been proposed (Mashburn-Warren and Whiteley, 2006). The first model posits that the OMVs originate from regions of the cell wall where there are no peptidoglycan-associated lipoproteins present (probably as a result of the outer membrane biosynthesis expanding faster than the underlying peptidoglycan layer). Then, these OMV-rich regions pinch off and are released from the cell surface. The second model proposes that the peptidoglycan fragments generated during normal cell wall turnover and/or repair are not efficiently transported back into the bacterial cytoplasm, thus leaving a region devoid of peptidoglycan. Turgor pressure resulting from a build-up of peptidoglycan within the periplasm would then cause blebbing of the outer membrane. The third model is thought to be specific to Pseudomonas aeruginosa where ionic interactions between Pseudomonas Quinolone Signal (PQS) and Mg²⁺ ions within the outer membrane enhances anionic repulsion between LPS molecules resulting in membrane blebbing (Mashburn-Warren et al., 2009). It was subsequently shown that PQS components are packaged within OMVs and these signaling components are thought to also be required for OMV formation (Mashburn-Warren et al., 2009). Though it is not known how OMVs are released from the Cronobacter cell surface, the vesicles observed in Figures 1, 2 could have been produced by mechanisms described in any of the proposed models. Schwechheimer and Kuehn (2015) have discussed in much greater detail the various models of OMV biogenesis, and various OMV structural components and their roles in the production of OMVs.

SDS-PAGE analysis of partially purified OMV preparations obtained from C. sakazakii, C. malonaticus, and C. turicensis (Figure 2) showed the presence of approximately 11 major protein bands, ranging in molecular weight (MW) from 18 to >100-kDa (Figure 3). The estimated MWs of these protein bands were 18, 25, 30, 30–35, 40 (three closely aligned protein bands), 50, 60, 100, and >100 kDa, and N-terminal amino acid sequencing and BLAST analysis (Table 2) identified these protein bands as OmpX, MipA, contaminating flagellin (Stephan et al., 2014, and 30–35 kDa), OmpA, OmpC, OmpE, OmpF, conjugative plasmid transfer protein (CTP), GroEL, an oligomer of OmpA, and an OM autotransporter protein (OMATP), respectively. The fact that known OMPs such as OmpA, C, E, F, and X were found associated with the isolated OMVs by SDS-PAGE and BLAST analysis strongly suggests that the isolation protocol used to obtain OMVs was successful in separating OMVs from cellular debris and other intracellular structures, except for the noted occasional entrapped flagella. Another interesting point can be made: many of the OMPs identified are OMPs which are related to the stress response. Schwechheimer and Kuehn address this in their review (Schwechheimer and Kuehn, 2015) where they suggest that OMV contents vary depending on the growth phase of the culture prior to OMV isolation. Because the cells used in the present study were more than likely at stationary phase of growth (overnight growth from a TSAS agar plate), OMVs shedding was maximized and their contents more reflective of cells growing under a stressful growth environment. This finding also explains why few cytoplasmic or cell membrane proteins were identified compared to OMPs reported in two previous studies reported by Alzahrani et al. (2015) and Ye et al. (2015). Though differences in protein abundance for C. sakazakii vs. that for C. malonaticus and C. turicensis were observed, collectively similar proteins were observed in the OMV preparations of each the three species. Other than the common flagellin and GroEL chaperonin proteins, the OMPs identified in the present study were not identified by Alzahrani et al. (2015). Quite possibly, the differences in types of OMV proteins could be ascribed to how the bacteria were grown in the two studies prior to isolation, i.e., stationary grown cells on TSAS used in this study vs. log phase grown cells in Brain Heart Infusion Broth or tryptic soy broth used by Alzahrani et al. and Ye et al., respectively (Alzahrani et al., 2015; Ye et al., 2015).

One of the three 40 kDa OMV protein bands and a 100 kDa protein band were identified as OmpA (Table 2). The first OMP described for Cronobacter was OmpA expressed by E. sakazakii strain 51329 (now C. muytjensii) by Mohan Nair and Venkitanarayanan (2006). BLAST analysis showed that each Cronobacter species possessed homologs of ompA (NCBI annotation identified the protein as encoding for an OmpA precursor protein). The 100 kDa protein possessed the same N-terminal amino acid sequence as the 40 kDa protein and these results suggest that the larger protein band represents an oligomer of the smaller protein band. Since the initial report by Mohan Nair and Venkitanarayanan (2006), ompA has also been shown to be a genus-specific PCR target and the protein shares homology with other porin-like OMPs common among the Enterobacteriaceae.

Similar to the OmpA, three additional proteins OmpC, OmpE, and OmpF also with MWs of 40 kDa were identified as porin-like proteins. Porin proteins span the outer membrane and act as a pore through which molecules can diffuse, and typically control the diffusion of small metabolites like sugars, ions, and amino acids, but some can also selectively transport a single group of molecules, or may be specific for one molecule (Klebba, 2005). For example, β-lactam and fluoroquinolone antibiotics must pass through porins to reach their targets in Gram-negative bacteria. Another OMP identified in the OMV preparations is OmpX with a MW of approximately 18-kDa. Vogt and Schulz (1999) described OmpX in E. coli as a member of a family of highly conserved bacterial proteins that promote bacterial adhesion to and entry into mammalian cells. Adherence factor functions have also been described for both OmpX and OmpA in Cronobacter. Recent reports (Mohan Nair and Venkitanarayanan, 2007; Kim and Loessner, 2008; Singamsetty et al., 2008; Kim et al., 2010) describing the invasion of Cronobacter into INT407 and Caco-2 cell lines have revealed that expression of OmpA, OmpX, and host actin filaments are required for invasion. In addition, Cronobacter invasion of HBMEC has been reported to require microtubules (Singamsetty et al., 2008). The findings reported here for OmpX and OmpA are similar to those reported by Ye et al. (2015).

A 30 kDa protein was identified as a membrane-bound lytic transglycosylase, MltA-interacting protein, which belongs to the OmpV family of OMPs and is thought to be primarily involved in cell wall/outer membrane biosynthesis (Table 2). MltA-interacting protein is encoded by the gene mipA which is a member of a family of genes that encode for several bacterial MltA-interacting proteins. MltA-interacting proteins are responsible for the enlargement of the stress-bearing peptidoglycan layer of bacteria, and their activity depends on the coordinated interaction of murein synthases and hydrolases, as well as its interaction with the membrane-bound lytic transglycosylase, MltA. MltA-interacting proteins are also known to bind to outer membrane-associated penicillin binding proteins, such as PBP1B, a bifunctional murein transglycosylase/transpeptidase. Voller et al. (1999) propose that MltA-interacting proteins attach to PBP1B to form a complex and in E. coli, represent the first step in reconstitution of the hypothetical murein-synthesizing holoenzyme; this complex is thought to be responsible for the controlled growth of the peptidoglycan layer. The presence of this protein within OMVs further supports the association of the cell wall biosynthesis hypothesis proposed by Mashburn-Warren and Whiteley (2006), Mashburn-Warren et al. (2009).

A 50 kDa protein was identified as a conjugative plasmid transfer protein (CTP) (Table 2). Conjugative transfer of bacterial plasmids is the most effective way of horizontal gene transfer, and it is therefore considered to be one of the major causes for the increase in the multidrug antibiotic resistance, with homologies now being assigned to type IV secretion systems. The most noted conjugative transfer protein is the P-type conjugative transfer protein, TrbG which is associated with the trb locus of Agrobacterium Ti plasmids. The TrbG-like protein is a lipoprotein homolog of the F-type TraK protein (which is believed to be an outer membrane pore-forming secretin), as well as the vir system-encoded VirB9 protein. The protein is hypothesized to oligomerize to form a ring-like structure similar to other secretins, and several additional observations support the hypothesis that TraK interacts with TraV and TraB to form a complex in E. coli that spans the cell envelope from the outer membrane (TraV) through the periplasm (TraK) to the inner membrane (TraB) (Harris et al., 2001). Dorward et al. (1989) proposed that OMVs can also facilitate genetic exchange between bacteria. Indeed, DNA contained in OMVs has been successfully transferred into other bacterial cells, even between cells of different species (Kahn et al., 1983). As proposed by Olsen and Amano (2015), this represents a bacterial DNA delivery system that is not yet well recognized and documented. The presence of this protein within these OMVs complements the fact that the conjugative plasmids such as pESA2, pSP291-2, and pCTU2 are present in some Cronobacter spp. and in particular, the three strains analyzed in this study.

An approximately 60-kDa protein was identified as GroEL (Table 2). Skjærven et al. (2015) suggest that GroEL plays an essential role in the control of cellular stress and as a molecular chaperon, and is found in a large number of bacteria. In addition to its stress response function, GroEL is thought to be required for the proper folding of many proteins i.e., assist in refolding of heat/stress-damaged proteins (Zeilstra-Ryalls et al., 1991). In order to function properly, GroEL requires a second protein, the lid-like co-chaperon protein complex GroES. Speculatively, the association of GroEL with OMVs may aid in the proper folding of other OMPs, such as OmpX and OmpA, for delivery to host tissues. The genes groES (mopA) and groEL (mopB) of E. coli form an operon which was first defined by mutations affecting the morphogenesis of several bacteriophages. For example, both of the groES/EL gene products have been shown to be essential for bacteriophage head and tail assemblies (Fayet et al., 1989). Furthermore, Frisk et al. (1989) showed using whole-cell enzyme-linked immunosorbent assay and immnuoelectron microscopy that the expression of GroEL in Haemophilus ducreyi was associated with the cell surface. The finding of GroEL associated Cronobacter spp. OMVs support these results and possibly identifies a new cellular location in Cronobacter other than the cytoplasm as suggested by Alzahrani et al. (2015).

Another large protein (>100 kDa) was identified as an OM autotransporter protein (OMATP). The secretion of proteins occurs in a number of different pathways in bacteria, and several secretion mechanisms have been ascribed to Gram-negative bacteria. The autotransporter secretion pathway (Lee and Schneewind, 2001) is a distinct secretion mechanism, in which an autotransporter protein moiety mediates the export of a protein through the outer membrane and the protein itself serves as the precursor of the secreted protein. Autotransporters have been implicated as important components/factors in mediating virulence mechanisms, such as the expression of adhesions used to colonize host cells, and actin-promoted bacterial mobility (Frisk et al., 1989). Autotransporters comprise three functional domains:(1) a N-terminal targeting domain (amino-terminal leader sequence) that functions as a signal peptide to mediate targeting to and translocation across the inner membrane; (2) a C-terminal translocation domain (carboxy-terminal) that forms a beta-barrel pore to allow for secretion (Henderson et al., 1998; Lee and Schneewind, 2001; Veiga et al., 2002); and (3) the secreted mature protein. The association of an autotransporter protein with the formation of OMVs supports the hypothesis that OMVs are another example of a bacterial secretion system. One of the most noted outer membrane protein autotransporter genes is icsA found on pWR100, the virulence plasmid of Shigella spp. This gene is responsible for the intracellular/intercellular bacterial movement by eliciting polar deposition of filamentous actin to bind to the bacterial cell surface in an actin-based motility (Bernardini et al., 1989). Thus, inside a host cell the nucleation and polymerization of actin molecules onto the Shigella cell surface by IcsA provides propulsion for intracellular movement and intercellular dissemination. However, little is known about the role and association of autotransporter proteins in Cronobacter pathogenesis.

PCR analysis was used to demonstrate OMP encoding gene prevalence and distribution among 240 Cronobacter and phylogenetically-related strains. We observed that all of the Cronobacter species possessed genes for OMATP, OmpA, OmpC, and GroEL (Table 3). In contrast, 3 of 12 C. dublinensis strains; 2 of 16 C. turicensis; and 10 of the 19 phylogenetically-related strains were PCR-negative for ompX, while all other Cronobacter strains were PCR-positive for this target. Within the 19 phylogenetically related strains, isolates that were PCR-negative for gene targets include 18 for OMATP gene, 16 for ompC, 16 for groEL, 17 for mipA, and 19 for ctp, suggesting that the primers used to detect these gene targets mostly detected Cronobacter-specific gene regions. Overall, these results suggest that genes for these OMPs appear to be conserved among Cronobacter species; however conservation of ompA, and ompX may be extended to other members of the Enterobacteriaceae. These findings also support the growing body of literature which reports that OMP porin proteins such as OmpA, OmpC, OmpF, OmpX and the chaperonin GroEL are well conserved among members of this large family of Gram-negative bacteria, and also supports the findings reported by Alzahrani et al. (2015) and Ye et al. (2015).

Recently, a novel pan genomic DNA microarray was developed to augment the development of next generation sequencing methods that can rapidly detect and characterize Cronobacter species and to be used as a highly discriminatory characterization and identification tool for the protection of public health in outbreaks or in source attribution investigations (Tall et al., 2015). Using this microarray, the presence of the OMP genes among 240 Cronobacter and phylogenetically-related species was determined. The microarray has 59 OMP alleles (probesets) representing all seven Cronobacter species. A summary of the hybridization results after the interrogation of these strains with 13 of these OMP gene probesets is shown in Table 4 and the presence/absence results demonstrate that particular alleles such as the OMATP gene from C. sakazakii and ompC and ompF from C. malonaticus captured on the microarray are more species-specific, while groEL and ompA alleles from C. turicensis and the ompC allele from C. muytjensii are highly conserved among all of the species. Nucleotide diversity of ompA sequences from 23 Cronobacter strains (representative of the 77 strains reported in this work) is shown in Figure 4 and different clusters of Cronobacter strains were observed. In most cases, there is a species-wise grouping of the ompA alleles as illustrated in the annotated tree. The diversity of C. sakazakii is demonstrated and emerging differences among some C. malonaticus, C. turicensis, and C. muytjensii strains were also noted. For example, the ompA allele of C. malonaticus strain CQ39 grouped with C. sakazakii strains instead of other C. malonaticus strains; and C. turicensis strain Md1s grouped with C. muytjensii strain GK1258. These two observations suggest that a wide nucleotide sequence divergence exists among ompA genes of various Cronobacter spp. This nucleotide sequence divergence was also captured by the microarray analysis and the results of the phylogenetic analysis using just the microarray OMP probesets is shown in Supplemental Figure 1. Interestingly, the Cronobacter and phylogenetically-related strains grouped as respective species into seven major clusters. For example C. sakazakii, C. malonaticus, C. turicensis, and C. univiersalis strains grouped into clusters 1–3, 4 and 6, 5, and 3, respectively. In contrast, C. dublinensis, C. muytjensii, and C. condimenti grouped as separate species clades within cluster 7. Lastly, the phylogenetically-related strains grouped as non-Cronobacter (labeled as nearest neighbors) species clades within clusters 1 and 7. This phylogenetic tree again agrees with similar phylogenetic analyses generated using whole genome sequence information (Grim et al., 2013; Stephan et al., 2014), and demonstrates the usefulness of the microarray to study the phylogenetic relationship of a specific set of alleles (Stephan et al., 2014; Tall et al., 2015; Yan et al., 2015b). In order to determine whether the various ompA genes translate into different proteins, the deduced 348 amino acid sequences of 10 ompA nucleotide sequences representing strains shown in Figure 4 were compared (Data not shown). Two interesting points can be made from this comparative sequence analysis: (1) A large cluster of 27 C. sakazakii strains of multiple serotypes (CsakO:2, CsakO:4, and ND), and sequence types (ST4, ST218, and ND) possessed an ompA gene similar in nucleotide and deduced protein sequence to that of Clonal Complex 4 C. sakazakii strains; and (2) several Cronobacter species possessed similar ompA genes; for example, C. sakazakii strain Md27g and C. malonaticus strain Md25g clustered together as did C. turicensis strain Md1s and C. muytjensii strains GK1258 and GK 1257. Comparing ompA gene sequences from subgroups of C. sakazakii and from Cronobacter species revealed nucleotide divergence at the intra- and inter-species levels. Any functional significance associated with these changes has to be elucidated further.

In summary, OMVs are released from both pathogenic and non-pathogenic Gram-negative bacterial cells by possibly several, yet unclear, mechanisms. In Cronobacter species, these vesicles are thought to be formed when the OM protrudes, and sometimes encapsulates both periplasmic and outer membrane bound components within their structures. Early on, these structures were thought to be artifacts but currently, OMVs are recognized as structures possessing very diverse functions. Foremost, OMVs can be regarded as a secretion system used by bacteria to communicate with host cells and other bacterial cells. Though the secretion of lipids, OMPs, and signaling molecules is achieved, the actual delivery system with these components is quite unique in that their contents are protected inside the lumen of the OMVs from the environment, and the intact OMVs can then be delivered directly to specific host cell receptors as suggested by Alzahrani et al. (2015). Many organisms use OMVs to secrete virulence factors. As such, bacteria may actively regulate their OMV contents to influence the host-pathogen interaction(s). For example, once Cronobacter gains entry into the systemic circulation either through the breakdown of the intestinal barrier via necrotizing enterocolitis or active adherence, invasion and translocation of enterocytes as suggested by Giri et al. (2012), OMVs may be released in abundant numbers and result in the delivery of OmpA and OmpX to target host cell receptors, such as the endothelial cells of the capillary bed making up the blood-brain-barrier (BBB). If there is an overwhelming abundant number of OMVs with associated components such as LPS and OMPs which are then presented to the host's immune system, a pro-inflammatory response may be stimulated which could lead to a fatal “cytokine storm.” Such immune responses have been previously described (Townsend S. M. et al., 2007; Mittal et al., 2009) and were shown to be inefficient in fighting intracellular infections. In order to determine whether LPS was associated with the OMVs, a preliminary experiment (data not shown) using a Pyrosate test kit for the detection of LPS (Associates of Cape Cod, Inc., MA) showed that LPS was present in the OMVs preparations. Speculatively, if a pro-inflammatory “cytokine storm” did occur (as suggested here by these preliminary results that LPS was associated with OMVs, and by evidence previously reported, Townsend S. M. et al., 2007; Mittal et al., 2009; Alzahrani et al., 2015) at the surface of endothelial cells within the capillary beds of the BBB in the presence of Cronobacter cells expressing OmpA and OmpX, alteration in the physiology and permeability of these cells could occur and lead to translocation (Giri et al., 2012) and bacterial invasion of the meninges. In addition, the infection may be further exacerbated by the interaction of the host's immune cells and Cronobacter, for example, the pathogen's survival and persistence within the phagocytic cells may further contibute to meningitis (Townsend S. M. et al., 2007; Mittal et al., 2009). The existence of Cronobacter and LPS components in PIF manufacturing environments (Townsend S. et al., 2007) is an excellent example of this intersection where man-made processes have selected for an organism's colonization and persisitence within this environment and the subsequent contamination of PIF products which are utlimately consumed by humans. It is this dynamic juncture where this bacterium, within its man-made environment, and its comtamination of a food product may contribute precisely to what King (2013) describes as the “triple threat” facing the overall health of humans as illustrated in the One Health Initiative. The global nature of our food supply further raises public health concerns about the risk of transporting microbes; i.e., microbes can move globally faster than their disease incubation periods, and the dangers to both human and animal health is increasing, with both food and water as potential vehicles for the dissemination of pathogens. Finally, the One Health approach is also proactive, preventive, and compliments nicely with the guidelines described in the Food Safety Modernization act of 2011 which will help to shift food safety attentions “upstream” to the ecological, animal, and environmental sources responsible for foodborne illnesses and, therefore, helps us to identify the most effective points for the initiation of food safety actions.

The authors declare that the research was conducted in the absence of any commercial or financial relationships that could be construed as a potential conflict of interest.