Research Article

Active and Passive Immunization Protects against Lethal, Extreme Drug Resistant-Acinetobacter baumannii Infection

  • Guanpingshen Luo,

    Affiliation: Division of Infectious Diseases, Los Angeles Biomedical Research Institute at Harbor–University of California Los Angeles (UCLA) Medical Center, Torrance, California, United States of America

  • Lin Lin,

    Affiliations: Division of General Internal Medicine, Los Angeles Biomedical Research Institute at Harbor–University of California Los Angeles (UCLA) Medical Center, Torrance, California, United States of America, David Geffen School of Medicine at University of California Los Angeles (UCLA), Los Angeles, California, United States of America

  • Ashraf S. Ibrahim,

    Affiliations: Division of Infectious Diseases, Los Angeles Biomedical Research Institute at Harbor–University of California Los Angeles (UCLA) Medical Center, Torrance, California, United States of America, David Geffen School of Medicine at University of California Los Angeles (UCLA), Los Angeles, California, United States of America

  • Beverlie Baquir,

    Affiliation: Division of General Internal Medicine, Los Angeles Biomedical Research Institute at Harbor–University of California Los Angeles (UCLA) Medical Center, Torrance, California, United States of America

  • Paul Pantapalangkoor,

    Affiliation: Division of General Internal Medicine, Los Angeles Biomedical Research Institute at Harbor–University of California Los Angeles (UCLA) Medical Center, Torrance, California, United States of America

  • Robert A. Bonomo,

    Affiliation: Departments of Medicine, Pharmacology, and Molecular Biology and Microbiology, Louis Stokes Cleveland Department of Veterans Affairs Medical Center, Case Western Reserve University, Cleveland, Ohio, United States of America

  • Yohei Doi,

    Affiliation: Division of Infectious Diseases, University of Pittsburgh Medical Center, Pittsburgh, Pennsylvania, United States of America

  • Mark D. Adams,

    Affiliation: Department of Genetics and Center for Proteomics and Bioinformatics, Case Western Reserve University, Cleveland, Ohio, United States of America

  • Thomas A. Russo,

    Affiliation: Veterans Administration Western New York Healthcare System, Division of Infectious Diseases, State University of New York, Buffalo, New York, United States of America

  • Brad Spellberg mail

    Affiliations: Division of General Internal Medicine, Los Angeles Biomedical Research Institute at Harbor–University of California Los Angeles (UCLA) Medical Center, Torrance, California, United States of America, David Geffen School of Medicine at University of California Los Angeles (UCLA), Los Angeles, California, United States of America

  • Published: January 10, 2012
  • DOI: 10.1371/journal.pone.0029446


Extreme-drug-resistant (XDR) Acinetobacter baumannii is a rapidly emerging pathogen causing infections with unacceptably high mortality rates due to inadequate available treatment. New methods to prevent and treat such infections are a critical unmet medical need. To conduct a rational vaccine discovery program, OmpA was identified as the primary target of humoral immune response after intravenous infection by A. baumannii in mice. OmpA was >99% conserved at the amino acid level across clinical isolates harvested between 1951 and 2009 from cerebrospinal fluid, blood, lung, and wound infections, including carbapenem-resistant isolates, and was ≥89% conserved among other sequenced strains, but had minimal homology to the human proteome. Vaccination of diabetic mice with recombinant OmpA (rOmpA) with aluminum hydroxide adjuvant markedly improved survival and reduced tissue bacterial burden in mice infected intravenously. Vaccination induced high titers of anti-OmpA antibodies, the levels of which correlated with survival in mice. Passive transfer with immune sera recapitulated protection. Immune sera did not enhance complement-mediated killing but did enhance opsonophagocytic killing of A. baumannii. These results define active and passive immunization strategies to prevent and treat highly lethal, XDR A. baumannii infections.


Antibiotic resistance is recognized as one of the greatest threats to human health on the planet [1], [2], [3], [4], [5]. In the last decade, Acinetobacter baumannii has emerged as one of the most common and highly antibiotic-resistant pathogens in the United States (US) and throughout the world [6], [7], [8]. Indeed, 50–70% of A. baumannii clinical isolates are now extensively drug resistant (XDR; i.e. resistant to carbapenems and all other antibiotics except colistin or tigecycline), reflecting a >15-fold increase in just the past 10 years [9], [10], [11], [12], [13]. Infections caused by XDR A. baumannii are associated with prolonged hospitalization, tremendous health care costs, and high rates of death despite treatment [6], [8], [12], [14], [15], [16], [17]. Even more concerning is the increasing resistance of A. baumannii to both colistin and tigecycline [8], [15], [18], [19], [20]. Such pan-drug resistant (PDR) A. baumannii infections are resistant to every FDA approved antibiotic, and are hence untreatable.

Since risk factors for A. baumannii infections are understood [21], [22], [23], [24], [25], vaccination of acutely at-risk patients is a promising method to prevent such infections, and antibody-based immunotherapy has promise to improve outcomes from infection. To identify a lead antigenic target for active and passive immunization against A. baumannii, a rational screening mechanism was used to identify a candidate vaccine. OmpA was found to be a predominant target of humoral immunity during sublethal A. baumannii infection in mice. Recombinant OmpA was an effective vaccine immunogen, protecting mice against lethal infection, and also induced protective antibodies when administered as passive immunization against lethal A. baumannii infection.


Specific anti-A. baumannii antibodies are generated during infection in mice

As a basis for identifying lead antigenic candidates for vaccine development, the humoral immune response to surface proteins from A. baumannii was determined after natural infection. Individually marked Balb/c mice were bled via tail-vein nicking to determine baseline, pre-immune anti-A. baumannii cell membrane protein antibody titers. Mice were then infected via the tail-vein with survivable inocula (106) of six clinical isolates of A. baumannii, five of which were carbapenem resistant (Table 1 and Table S1). Two weeks post-infection, paired immune sera were obtained from the mice. ELISA of paired pre-immune vs. immune sera confirmed that mice infected with all of the strains generated substantial increases (10–100-fold) in anti-A. baumannii cell membrane protein IgG-antibody titers by 2 weeks post-infection (Figure 1).


Figure 1. A. baumannii infection induces specific humoral immune response.

Ten mice were infected with ATCC 17978 (top) and 2 mice each were infected with clinical isolates from Harbor-UCLA Medical Center (HUMC) (bottom). Paired pre-immune & immune serum IgG anti-A. baumannii cell membrane protein titers are shown. M1 = mouse 1; M2 = mouse 2.


Table 1. Bacterial Strains.*


Having demonstrated a specific humoral immune response to the organism, the immunodominant antigenic target of that response was sought. A. baumannii cell membrane protein preparations from all six strains used to infect mice were separated by two dimensional gel electrophoresis and stained by western blot using paired pre-immune and immune sera from the above infected mice. The two dimensional gels demonstrated effective separation by size and isoelectric focusing (IEF) of membrane proteins from all six clinical isolates (Figure 2A). In all cases, post-immune serum identified a limited number of unique spots not recognized by pre-immune serum (Figure 2B).


Figure 2. A. baumannii infection induces specific anti-rOmpA antibody response.

(A) Membrane protein preparations from A. baumanni clinical strains (ATCC 17978 & HUMC1, 4, 5, 6, & 12) were run on 2 D gels stained with Coomassie Blue. (B) Western blots of those 2D gels were stained with paired sera obtained from mice before infection (pre-serum) and after recovery from non-lethal iv infection (post-serum) with A. baumannii. 2D gels were run at least twice for all strains, and representative figures are shown. Spots uniquely identified by post-immune serum were seen at conserved locations. Spots selected for protein identification by MALDI-TOF analysis are marked with white arrows—these all contained OmpA.


The same three spots (Figure 2B) were selected for identification by MALDI-TOF analysis across blots from three different A. baumannii isolates representing different strain types (Table 1). The protein found in all spots was identified by matrix assisted laser desorption/ionization-time of flight (MALDI-TOF) analysis as OmpA, which is known to be a predominant component of the outer cell membrane of A. baumannii [47]. Anti-OmpA antibody titers were determined in paired pre-immune vs. immune sera from mice infected with A. baumannii. As for total anti-A. baumannii antibodies, anti-rOmpA IgG titers increased in most mice infected with A. baumanniii (Figure 3), confirming that OmpA is a target of adaptive humoral immunity post-infection.


Figure 3. Anti-OmpA IgG antibodies were generated after infection with multiple strains of A. baumannii.

Ten mice were infected with ATCC 17978 (top) and 2 mice each were infected with HUMC clinical isolates (bottom). Paired pre-immune & immune serum IgG anti-rOmpA cell membrane protein titers are shown.


OmpA as a potential vaccine antigen

Ideal antigens for vaccine development should be conserved across clinical isolates and should not be homologous to the human proteome. The ompA gene was sequenced in the six clinical isolates used for infection. The predicted protein sequence had 99% identity across all clinical isolates (Figure 4), which were harvested 58 years apart (1951 to 2009) from varied clinical sources (cerebrospinal fluid, lung, blood, wound; Table 1). Alignment against 14 other sequences from A. baumannii in PubMed revealed 89% identity across all sequences (Figure S1). In contrast, PubMed BLAST search of the human proteome using the ATCC 17978 OmpA sequence revealed only 7 sequences with minimal homology (E values ranging 0.53 to 6.2). Thus OmpA is conserved across a broad array of clinical isolates of A. baumannii but shares minimal homology with human proteins.


Figure 4. OmpA was highly conserved across clinical isolates of A. baumannii.

The OmpA gene was sequenced from each strain and the predicted amino acid sequences demonstrated >99% identity.


To determine in vivo efficacy, a lethal infectious model was desired. However, A. baumannii bacteremia spontaneously clears in mice unless a host defect is present [39]. Similarly, in our initial pilot experiments, a lethal iv infectious inoculum could not be identified in normal Balb/c mice, unless inocula were so high that they induced overwhelming infection resulting in death within 24 h (e.g., ≥109 bacilli). While neutropenia has been used to make mice susceptible to lethal infection caused by A. baumannii [39], [40], [41], neutropenia is a rare clinical risk factor for patients with A. baumannii infections [12], [21], [22], [23], [42], [43], [44], [45]. Thus an alternative means to immunocompromise mice was sought. By multivariate analysis, diabetes mellitus has been shown to be a risk factor for acquisition of and worse outcomes from A. baumannii infection [23], [24], [46], so a diabetic mouse model of mucormycosis [28] was adapted for in vivo study of A. baumannii infections. In pilot studies, an inoculum of 2 to 3×107 of strain HUMC1 was found to cause lethal iv infection in diabetic Balb/c mice (data not shown).

rOmpA was expressed in E. coli and purified by nickel-agarose binding to a His tag. In the initial experiment, retired breeder (>6 months old) mice were vaccinated and boosted with rOmpA in 0.1% aluminum hydroxide (Al(OH)3). Diabetes was induced after the boost and two weeks later, diabetic mice were infected via the tail-vein with A. baumannii HUMC1. Vaccinated mice had significant improvements in survival compared to adjuvant control mice (Figure 5A). The experiment was repeated using juvenile mice and again the vaccine improved survival compared to adjuvant control mice (Figure 5B).


Figure 5. Vaccination with rOmpA protected mice from lethal A. baumannii infection in a disseminated sepsis model.

A) Survival of retired breeder (>6 mo) diabetic Balb/c mice vaccinated with 3 µg of rOmpA plus aluminum hydroxide (AlOH3) adjuvant, or with adjuvant alone (n = 6 adjuvant control and 8 vaccinated) and infected with 2×107 A. baumannii HUMC1. B) Survival of juvenile (8–10 weeks, n = 18 mice per group) diabetic Balb/c mice vaccinated with 3 µg of rOmpA plus adjuvant or adjuvant alone and infected with 2×107 A. baumannii HUMC1. C) Tissue bacterial burden in vaccinated (3 µg) or control diabetic mice (n = 10 control and 13 vaccinated) infected with 107 A. baumannii HUMC1. Median and interquartile ranges are shown. * p<0.05 vs. adjuvant control.


To determine the impact of vaccination on bacterial burden, juvenile mice were vaccinated, made diabetic, and infected as above. On day 2 post-infection (the day the control mice were predicted to die based on the previous experiment), mice were euthanized and organs harvested to determine tissue bacterial burden. Vaccination reduced by approximately 10-fold the tissue bacterial burden in all organs evaluated except for the lungs, which had a non-significant (p = 0.08) 3-fold reduction in bacterial burden (p<0.01 bacterial burden in vaccinated vs. control mice for all other organs) (Figure 5C).

Antibodies in vaccine-mediated protection

The relationship between antibody titers and survival in vaccinated mice was evaluated. In two separate experiments, mice were vaccinated with rOmpA plus adjuvant or adjuvant alone, boosted, and antibody titers were determined pre-infection. Vaccination with 3 µg of rOmpA induced marked increases in anti-rOmpA IgG antibody titers compared to control mice (median [range] titers = 204,800 [102,400–409,600] for vaccinated vs. 800 [800–2,000] for adjuvant control mice, p<0.0001). Vaccination again protected mice from lethal infection (note slightly lower inoculum for these experiments, 1.4×107 and 1.6×107 for the repeat experiments, vs. 2×107 and 2.4×107 in the previous survival experiments) (Figure 6A). Antibody titers correlated with survival (Figure 6B) when analyzing both vaccinated and control mice combined (p<0.0001, rho = 0.5) or just analyzing vaccinated mice without control mice (p = 0.001, rho = 0.6 by Spearman Rank test). An IgG titer threshold of ≥204,800 was maximally accurate at distinguishing survivors from non-survivors when analyzing both vaccinated and control mice (96%) or when analyzing just vaccinated mice (85%).


Figure 6. Anti-rOmpA antibody titers correlated with survival in infected mice.

A) Survival of juvenile diabetic Balb/c mice vaccinated with 3 µg of rOmpA plus adjuvant or adjuvant alone (n = 20 mice per group from 2 experiments) and infected with 1.4 or 1.6×107 A. baumannii HUMC1 in the sequential experiments. The experiments were terminated at 28 days with all remaining mice appearing clinically well. B) Antibody titers of individual vaccinated (n = 26) and control (n = 28) mice vs. day of death.


To confirm the activity of immune antibodies, serum was harvested from donor vaccinated or control mice (rOmpA titers = 1:409,600 from vaccinated vs. 1:3,200 from control sera). Diabetic mice were treated ip with 0.5 ml of immune or control serum and infected 2 hours later with A. baumannii HUMC1. Mice treated with immune serum had markedly enhanced survival vs. mice treated with control serum (Fig. 7A). To define the mechanism of antibody-induced protection, A. baumannii was cultured in the presence of immune vs. non-immune serum. A. baumannii numbers doubled or tripled relative to growth controls (absent serum) after 1 hour culture in both immune and non-immune sera at both 10% and 40% (data not shown), excluding complement-mediated killing as a mechanism of protection. Immune serum also did not reduce CFUs relative to control serum (Fig. 7B). However, immune serum did enhance opsonophagocytic killing of A. baumannii (Fig. 7B).


Figure 7. Passive immunization with immune serum from rOmpA-vaccinated mice protected recipient mice from lethal infection.

A) Survival of juvenile diabetic Balb/c mice (n = 10 per group) treated ip with immune (from OmpA vaccinated donor mice) or non-immune (from adjuvant treated donor mice) serum 2 hours before tail-vein infection with 2×107 A. baumannii HUMC1. The experiments were terminated at 28 days with all remaining mice appearing clinically well. *p = <0.0001 vs. non-immune serum. B) Opsonophagocytic killing of A. baumannii HUMC1 by immune (from OmpA vaccinated mice) or control (from adjuvant treated mice) serum incubated without or with RAW 247.6 macrophages. Median and interquartile killing is shown, normalized to the control serum. Results are from 8 to 12 samples per group, from 3 separate experiments. *p<0.05 vs. all other groups.



Over the past decade A. baumannii has emerged to become one of the most antibiotic-resistant causes of infections all over the world. It is critical that new strategies are developed to prevent and treat such infections. Therefore, a rational discovery program was undertaken to identify a candidate antigen for an A. baumannii-targeted vaccine. Antigen discovery was based on identification of the immunodominant targets from A. baumannii membrane protein preparations following systemic infection. rOmpA was identified as a promising candidate for active and passive immunization based on humoral immunodominance during infection in mice. OmpA was highly conserved across multiple clinical isolates, and shared minimal homology with the human proteome. Substantial efficacy was seen in lethal murine models in immunocompromised, diabetic mice when administered with Al(OH)3 adjuvant.

Individual mouse antibody titers correlated with survival and immune serum was effective during passive immunization. It has been previously reported that A. baumannii can be resistant to complement-mediated killing [48], [49], however the complement resistance in A. baumannii appears to be strain dependent [50]. In a previous study, complement susceptible strains were reported to decrease in quantity by 5 to 10-fold after 1 hour of incubation in serum, whereas resistant strains increased during that hour by a similar amount [50]. In the current study, the A. baumannii strains tested doubled or tripled after 1 hour of culture in the presence of serum (immune and non-immune), ruling out a direct complement-mediated effect. Hence, antibodies to OmpA did not overcome the innate resistance of the organism to complement-mediated killing. However, immune serum from vaccinated mice did enhance opsonophagocytic killing of the organism. Collectively, these results confirm that enhanced uptake and killing of A. baumannii by antibody-based opsonophagocytosis lead to more effective clearance of A. baumannii from tissue. Thus, phagocytic killing of A. baumannii can be enhanced by antibodies targeting OmpA.

A. baumannii OmpA has been found to have a variety of interesting biological properties in in vitro model systems. For example, OmpA has been shown to bind to eukaryotic cells, translocate to the nucleus, and induce cell death [47], [51]. Furthermore, OmpA binding to Factor H may be responsible for the resistance of A. baumannii to complement-mediated killing [48], [49]. However, as mentioned, in the current study antibodies targeting OmpA did not overcome serum resistance of the organism. Rather, anti-OmpA antibodies enhanced opsonophagocytic killing of the organism.

Recently, a whole cell, killed A. baumannii vaccine was described which protected mice from infection [52]. The investigators prepared crude cell membrane protein preparations and found that the immunologically active components of the whole cell vaccine were found in the cell membrane [53]. The crude membrane preparation contained at least 61 separate proteins, and the resulting mixture protected mice from lethal A. baumannii infection. These results underscore the potential for A. baumannii vaccines to be effective, and are complementary to the current study, which defines one antigen as a promising lead candidate to develop a recombinant protein based vaccine, as opposed to a crude cell membrane extract. In contrast to the previous study, which found that antibodies were raised against numerous antigens when a crude membrane preparation was used to immunize mice [53], the current study defined humoral immune response after iv infection with viable, pathogenic organisms, rather than immunization with membrane protein preparations. While OmpA was identified as a predominant protein target of humoral immunity after iv infection, the current results cannot exclude a broader immune response to other proteins as well.

In summary, rOmpA is a promising candidate for active and passive immunization to prevent XDR/PDR A. baumannii infections. Efficacy has been established at feasible doses with a translatable adjuvant. Use of the vaccine elucidated opsonophagocytic antibodies as the mechanism of adaptive host defense that protected against A. baumannii infection. Anti-OmpA antibody titer was identified as a surrogate marker of protection. These results underscore the translational potential of rOmpA as a target for active and passive immunization against this highly antibiotic-resistant, rapidly emerging pathogen.

Materials and Methods

Organism and mouse strains

Six clinical isolates of A. baumannii were used (Table 1 and Table S1). Five of the strains were resistant to all antibiotics except for colistin. Strain typing was performed by multi-locus sequence typing as previously described [26], [27]. Balb/c mice were used for all experiments. For some experiments, retired breeder mice (>6 mo old) were used, whereas for other experiments juvenile (6–10 weeks old) Balb/c mice were used. Diabetes was induced by intraperitoneal injection of 200 mg/kg streptozotocin in 0.2 ml citrate buffer 10 days prior to infection. Glycosuria and ketonuria were confirmed in all mice 7 days after streptozotocin treatment, as previously described [28].

Cell Membrane Preparations, Western Blots, 2 Dimensional Gel Imaging, and Protein Identification

A. baumannii cell membrane preparations were produced by a modification of a standard, published method [29], [30]. In brief, A. baumannii strains were grown overnight at 37°C with shaking in tryptic soy broth (TSB). The bacteria were passaged to mid-log-growth at 37°C with shaking, washed, and the resultant pellet was resuspended in disintegration buffer (7.8 g/L NaH2PO4, 7.1 g/L Na2HPO4, 0.247 g/L MgSO4 7.H2O+protease inhibitor mix (GE Healthcare, USA)+nuclease mix (GE Healthcare, USA)) and sonicated on ice for 3 periods of 5 min. The unbroken cells were separated by centrifugation at 1,500 g. The supernatant was centrifuged for 30 min at 4°C at 4,500 rpm and was passed through a 0.45 µM filter (Milipore, USA) to remove cell debris. An equal volume of ice-cold 0.1 M sodium carbonate (pH 11) was added to the resulting supernatant and the mixture was stirred slowly overnight, on ice. The carbonate treated membrane proteins were collected by ultracentrifugation at 100,000 g for 45 min at 4°C, and the membranes were re-suspended in 500 µl H2O. Finally, the protein extract was processed with a 2-DE Cleanup Kit (Bio-Rad, USA).

Two dimensional SDS/10%-PAGE gels of A. baumannii cell membrane preparations were used to separate proteins by size and isoelectric focusing (IEF), as described by Pitarch et al [31], [32]. For isoelectric focusing (IEF), the Bio-Rad-PROTEIN IEF system was used (Bio-Rad, USA) with 4–7 pH gradient strips (ReadyStrip IPG strips, Bio-Rad, USA). Proteins were solubilized in 8 M urea, 2% (w/v) CHAPS, 40 mM DTT and 0.5% (v/v) corresponding rehydrated buffer (Bio-Rad, USA). The strips were rehydrated overnight and underwent electrophoresis at 250 V for 20 min, 4000 V for 2 h, and 4,000 V for 10,000 V-h, all at room temperature. Prior to the second dimension (SDS-PAGE), the focused IPG strips were equilibrated with buffer I and II for 10 min (ReadyPrep 2-D Starter Kit, Bio-Rad, USA). The proteins were separated on 8–16% Criterion Pre-cast Gel (Bio-Rad, USA) and transferred to immune-Blot PVDF membranes (Bio-Rad, USA). Membranes were treated with Western Blocking Reagent (Roche) overnight and probed with pre-immune or immune A. baumannii infected-mice serum. Membranes were washed and incubated with secondary, HRP-conjugated goat anti-mouse IgG (Santa Cruz Biotech, USA). After incubation with SuperSignal West Dura Extended Duration Substrate (Pierce, USA), signals were detected using a CCD camera.

Protein spots of interest were excised and sent to the UCLA W. M. Keck Proteomic Center for identification on a Thermo LTQ-Orbitrap XL mass spectrometer (San Jose, CA) equipped with an Eksigent (Dublin, CA) NanoLiquid chromatography-1D plus system and an Eksigent autosampler. Proteins within the spots were in-gel tryptic digested as described by Shevchenko et al. [33], [34]. The eluted peptides were loaded onto a CVC Microtech (Fontana, CA ) 35 mm length, 100 µm ID C18 pre-Trap column and washed for 10 min with 100% Buffer A (2% acetonitrile containing 0.1% formic acid) at a flow rate of 5 µl/min. The peptides were separated on a 15 cm New Objective ProteoPep IntegraFrit column (Woburn, MA) using a flow rate of 300 nl/min. The following elution gradient was used: 0–15 min 0–30% Buffer B (98% acetonitrile containing 0.1% formic acid), 15–20 min 30–80% Buffer B and 20–22 min 80% Buffer B. The column was then re-equilibrated for 13 min with Buffer A. The eluting analytes were sprayed in positive mode into the LTQ-Orbitrap MS using electrospray ionization voltage of 2300 V, capillary voltage of 45 V, tube lens of 130 V, and capillary temperature of 200°C. Information dependent acquisition was performed where the 6 most intense ions were selected in the m/z range of 300–1600 using a 60 K resolution FTMS scan and subjecting them to MS-MS using broadband collision induced disassociation of normalized collision energy of 35 and LTQ detection. Peaks were excluded from further MS-MS for a period of 60 sec.

The resulting MS/MS spectra was searched against the Acinetobacter baumannii strain ATCC 17978 database (​/main.php?spid=Abau_ATCC17978) using the Matrix Science MASCOT Daemon search engine (Boston, MA). The following search parameters were used: peptide tolerance: ±10 ppm, MS/MS tolerance ±0.3 Da, maximum missed cleavages: 2, fixed modifications: carboxymethyl (C) and variable modifications: deamidization (ND) and oxidation (M). Proteins identified within a particular included those with a minimum of two unique peptides that are ranked as number 1 and with an ion scores with a p<0.05.

rOmpA Production and Immunization

His-tagged rOmpA (amino acids 2 to 347) was produced in an Escherichia coli pQE-32 expression system (Qiagen) as previous described [35], [36]. Briefly, ompA was amplified from A. baumannii 17978 genomic DNA with primers OmpA-F CATCACCATGGGATCCTTGTTGCTGCTCCATTAGCT and OmpA-R CTAATTAAGCTTGGCTGCAGTTATTGAGCTGCTGCAGGA and cloned into QE-32 by using In-Fusion 2.0 Dry-Down PCR Cloning Kit, per the manufacturer's instructions (Clontech Laboratories). The 6X-His tagged protein was purified over a Ni-agarose affinity column according to the manufacturer instructions (Qiagen). Endotoxin was removed from rOmpA by using Detoxin Gel Endotoxin Removing Columns (Norgen Biotek, Canada), and the endotoxin level was determined with Limulus Amebocyte Lysate endochrome (Charles River) per manufacturer's instruction. Using this procedure, endotoxin was reduced to 1 to 4 EU per 3 µg dose used for vaccination. Mice were immunized by subcutaneous injection of 3 µg of rOmpA in 0.1% Al(OH)3 (Alhydrogel, Brenntag Biosector, Frederikssund, Denmark) in phosphate buffered saline (PBS). Control mice received adjuvant alone on the same schedule. Mice were immunized 5 weeks prior to infection and again 2 weeks prior to infection. Four days after the boost (10 days prior to infection), mice were rendered diabetic as described above.

Mouse model of infection

A. baumannii strains were grown overnight at 37°C with shaking in TSB broth. The bacteria were passaged to mid-log-growth at 37°C with shaking. Cells were washed twice with PBS and resuspended at the appropriate concentration for infection. The final concentration was confirmed by quantitative culturing of the inocula. Mice were infected iv via the tail-vein with sublethal (106) or lethal (targeted 2×107) inocula in PBS. All animal work was conducted after approval by the Institutional Animal Use and Care Committee at the Los Angeles Biomedical Research Institute (project 012447), in compliance with the recommendations in the Guide for the Care and Use of Laboratory Animals of the National Institutes of Health.

Two days after infection (the day on which control mice were anticipated to begin dying), organs were harvested and homogenized in sterile PBS. Homogenized organs from individually marked mice were quantitatively cultured to determine tissue bacterial burden.


A previously published ELISA assay [37], [38] was adapted for detection of antibodies against A. baumannii cell membrane preparations and rOmpA. In brief, ELISA plates were coated with 100 µl per well of 5 µg/ml of rOmpA or cell membrane preparation. Coated wells were blocked with bovine serum albumin, incubated with mouse sera, washed, and stained with goat anti-mouse secondary antibody conjugated with horseradish peroxidase. Wells were washed again and incubated with o-phenylenediamine substrate with H2O2. The color was allowed to develop for 20 min after which the reaction was terminated by adding equal volume of 3N HCl and the optical density (OD) was determined at 490 nm in a microtiter plate reader. Negative control wells received an irrelevant isotype control monoclonal antibody rather than mouse serum. The ELISA titer was taken as the reciprocal of the last serum dilution with an OD reading≥(mean OD of negative control samples+(standard deviation * 2)).

Complement and Opsonophagocysis Assays

A. baumannii HUMC1 was cultured overnight in tryptic soy broth (TSB) at 37°C, passaged to mid-log growth, rinsed, and aliquoted into 96 well microtiter plates. For complement studies, 10% or 40% non-immune or immune sera were added to the wells for 1 hour. Well contents were quantitatively cultured at baseline and again at 1 h. The opsonophagocytic kill assay was based on a modification of a previously used method [25][26]. Murine RAW 264.7 macrophage cells (American Type Culture Collection, Rockville, MD) were cultured at 37°C in 5% CO2 in RPMI 1640 (Irvine Scientific, Santa Ana, CA) with 10% fetal bovine serum (FBS), 1% penicillin, streptomycin, and glutamine (Gemini BioProducts), and 50 µM β-mercaptoethanol (Sigma-Aldrich, St. Louis, MO). RAW 274.7 cells were activated by 3 days of exposure to 100 nM PMA (Sigma-Aldrich). Activated RAW 264.7 macrophages were harvested after scraping with BD Falcon cell scrapers (Fischer Scientific) and added to the microtiter wells at a 20:1 ratio of macrophages to bacteria. After a 1 hour incubation with gentle shaking, aliquots from the wells were quantitatively plated in tryptic soy agar (TSA). Colony forming units (CFU) of individual tubes were normalized to the average CFUs in tubes with control serum, and percent killing was calculated as 1−(CFUs from the individual tube/average CFU in tubes with control serum).


Survival was compared by the non-parametric Log Rank test. Antibody titers and bacterial burden were compared with the Wilcoxon Rank Sum test for unpaired comparisons or the Wilcoxon Signed Rank test for paired comparisons, as appropriate. Multiple comparisons were corrected by the Tukey non-parametric test. Correlations were determined by the Spearman Rank test. All statistics were run using Kyplot. Differences were considered significant if the p value was <0.05.

Supporting Information

Figure S1.

Homology of rOmpA to A. baumannii strains. OmpA is >99% homologous at the amino acid level across the six clinical isolates of A. baumannii used in the current study, including carbapenem-susceptible and carbapenem-resistant strains. C) 14 additional with sequences in Pubmed Genbank.



Table S1.

Susceptibility Testing for Strains Studied.




The authors would like to extend sincere appreciation to Melissa Sondej at the UCLA Molecular Instrumentation Center for assistance with the proteomics results. Results presented in part at the 98th Annual Meeting of the American Association of Immunologists.

Author Contributions

Conceived and designed the experiments: LL BS. Performed the experiments: GL LL ASI BB PP YD MDA. Analyzed the data: RAB MDA TAR BS. Contributed reagents/materials/analysis tools: RAB MDA TAR BS. Wrote the paper: GL LL ASI RAB YD MDA TAR BS.


  1. 1. Walker B, Barrett S, Polasky S, Galaz V, Folke C, et al. (2009) Environment. Looming global-scale failures and missing institutions. Science 325: 1345–1346.
  2. 2. Smolinski MS, Hamburg MA, Lederberg J, editors. (2003) Microbial Threats to Health: Emergence, Detection, and Response. Washington D.C.: The Institute of Medicine. 367 p.
  3. 3. Infectious Diseases Society of America (2004) Bad Bugs, No Drugs. 35 p. A White Paper. Alexandria, VA.
  4. 4. Choffnes ER, Relman DA, Mack A (2010) for the Forum on Microbial Threats, Institute of Medicine of the National Academies. Antibiotic resistance: implications for global health and novel intervention strategies. Washington D.C.: The National Academies Press.
  5. 5. Spellberg B, Blaser M, Guidos R, Boucher HW, Bradley JS, et al. (2011) for the Infectious Diseases Society of America. Position Paper: Combating Antimicrobial Resistance. Clin Infect Dis 52(S5): S397–428.
  6. 6. Perez F, Hujer AM, Hujer KM, Decker BK, Rather PN, et al. (2007) Global challenge of multidrug-resistant Acinetobacter baumannii. Antimicrob Agents Chemother 51: 3471–3484.
  7. 7. Higgins PG, Dammhayn C, Hackel M, Seifert H (2010) Global spread of carbapenem-resistant Acinetobacter baumannii. J Antimicrob Chemother 65: 233–238.
  8. 8. Doi Y, Husain S, Potoski BA, McCurry KR, Paterson DL (2009) Extensively drug-resistant Acinetobacter baumannii. Emerg Infect Dis 15: 980–982.
  9. 9. Rosenthal VD, Maki DG, Jamulitrat S, Medeiros EA, Todi SK, et al. (2010) International Nosocomial Infection Control Consortium (INICC) report, data summary for 2003–2008, issued June 2009. Am J Infect Control 38: 95–104 e102.
  10. 10. Hoffmann MS, Eber MR, Laxminarayan R (2010) Increasing resistance of acinetobacter species to imipenem in United States hospitals, 1999–2006. Infect Control Hosp Epidemiol 31: 196–197.
  11. 11. Hidron AI, Edwards JR, Patel J, Horan TC, Sievert DM, et al. (2008) NHSN annual update: antimicrobial-resistant pathogens associated with healthcare-associated infections: annual summary of data reported to the National Healthcare Safety Network at the Centers for Disease Control and Prevention, 2006–2007. Infect Control Hosp Epidemiol 29: 996–1011.
  12. 12. Lautenbach E, Synnestvedt M, Weiner MG, Bilker WB, Vo L, et al. (2009) Epidemiology and impact of imipenem resistance in Acinetobacter baumannii. Infect Control Hosp Epidemiol 30: 1186–1192.
  13. 13. Kallen AJ, Hidron AI, Patel J, Srinivasan A (2010) Multidrug Resistance among Gram-Negative Pathogens Causing Healthcare-Associated Infections Reported to the National Healthcare Safety Network, 2006–2008. Infect Control Hosp Epidemiol 31: 528–531.
  14. 14. Sunenshine RH, Wright MO, Maragakis LL, Harris AD, Song X, et al. (2007) Multidrug-resistant Acinetobacter infection mortality rate and length of hospitalization. Emerg Infect Dis 13: 97–103.
  15. 15. Falagas ME, Rafailidis PI, Matthaiou DK, Virtzili S, Nikita D, et al. (2008) Pandrug-resistant Klebsiella pneumoniae, Pseudomonas aeruginosa and Acinetobacter baumannii infections: characteristics and outcome in a series of 28 patients. Int J Antimicrob Agents 32: 450–454.
  16. 16. Gordon NC, Wareham DW (2009) A review of clinical and microbiological outcomes following treatment of infections involving multidrug-resistant Acinetobacter baumannii with tigecycline. J Antimicrob Chemother 63: 775–780.
  17. 17. Munoz-Price LS, Zembower T, Penugonda S, Schreckenberger P, Lavin MA, et al. (2010) Clinical Outcomes of Carbapenem-Resistant Acinetobacter baumannii Bloodstream Infections: Study of a 2-State Monoclonal Outbreak. Infect Control Hosp Epidemiol 31: 1057–1062.
  18. 18. Adams MD, Nickel GC, Bajaksouzian S, Lavender H, Murthy AR, et al. (2009) Resistance to colistin in Acinetobacter baumannii associated with mutations in the PmrAB two-component system. Antimicrob Agents Chemother 53: 3628–3634.
  19. 19. Park YK, Jung SI, Park KH, Cheong HS, Peck KR, et al. (2009) Independent emergence of colistin-resistant Acinetobacter spp. isolates from Korea. Diagn Microbiol Infect Dis 64: 43–51.
  20. 20. Livermore DM, Hill RL, Thomson H, Charlett A, Turton JF, et al. (2010) Antimicrobial treatment and clinical outcome for infections with carbapenem- and multiply-resistant Acinetobacter baumannii around London. Int J Antimicrob Agents 35: 19–24.
  21. 21. Beavers SF, Blossom DB, Wiemken TL, Kawaoka KY, Wong A, et al. (2009) Comparison of risk factors for recovery of Acinetobacter baumannii during outbreaks at two Kentucky hospitals, 2006. Public Health Rep 124: 868–874.
  22. 22. Caricato A, Montini L, Bello G, Michetti V, Maviglia R, et al. (2009) Risk factors and outcome of Acinetobacter baumanii infection in severe trauma patients. Intensive Care Med 35: 1964–1969.
  23. 23. Metan G, Sariguzel F, Sumerkan B (2009) Factors influencing survival in patients with multi-drug-resistant Acinetobacter bacteraemia. Eur J Intern Med 20: 540–544.
  24. 24. Furniss D, Gore S, Azadian B, Myers SR (2005) Acinetobacter infection is associated with acquired glucose intolerance in burn patients. J Burn Care Rehabil 26: 405–408.
  25. 25. D'Agata EM, Thayer V, Schaffner W (2000) An outbreak of Acinetobacter baumannii: the importance of cross-transmission. Infect Control Hosp Epidemiol 21: 588–591.
  26. 26. Tian GB, Adams-Haduch JM, Bogdanovich T, Pasculle AW, Quinn JP, et al. (2011) Identification of diverse OXA-40 group carbapenemases, including a novel variant, OXA-160, from Acinetobacter baumannii in Pennsylvania. Antimicrob Agents Chemother 55: 429–432.
  27. 27. Bartual SG, Seifert H, Hippler C, Luzon MA, Wisplinghoff H, et al. (2005) Development of a multilocus sequence typing scheme for characterization of clinical isolates of Acinetobacter baumannii. J Clin Microbiol 43: 4382–4390.
  28. 28. Spellberg B, Fu Y, Edwards JE Jr, Ibrahim AS (2005) Combination therapy with amphotericin B lipid complex and caspofungin acetate of disseminated zygomycosis in diabetic ketoacidotic mice. Antimicrob Agents Chemother 49: 830–832.
  29. 29. Molloy MP, Herbert BR, Slade MB, Rabilloud T, Nouwens AS, et al. (2000) Proteomic analysis of the Escherichia coli outer membrane. Eur J Biochem 267: 2871–2881.
  30. 30. Soares NC, Cabral MP, Parreira JR, Gayoso C, Barba MJ, et al. (2009) 2-DE analysis indicates that Acinetobacter baumannii displays a robust and versatile metabolism. Proteome Sci 7: 37.
  31. 31. Pitarch A, Pardo M, Jimenez A, Pla J, Gil C, et al. (1999) Two-dimensional gel electrophoresis as analytical tool for identifying Candida albicans immunogenic proteins. Electrophoresis 20: 1001–1010.
  32. 32. Pitarch A, Jimenez A, Nombela C, Gil C (2006) Decoding serological response to Candida cell wall immunome into novel diagnostic, prognostic, and therapeutic candidates for systemic candidiasis by proteomic and bioinformatic analyses. Mol Cell Proteomics 5: 79–96.
  33. 33. Shevchenko A, Wilm M, Vorm O, Mann M (1996) Mass spectrometric sequencing of proteins silver-stained polyacrylamide gels. Anal Chem 68: 850–858.
  34. 34. Shevchenko A, Jensen ON, Podtelejnikov AV, Sagliocco F, Wilm M, et al. (1996) Linking genome and proteome by mass spectrometry: large-scale identification of yeast proteins from two dimensional gels. Proc Natl Acad Sci U S A 93: 14440–14445.
  35. 35. Spellberg B, Ibrahim AS, Yeaman M, Lin L, Fu Y, et al. (2008) The anti-fungal rAls3p-N vaccine protects mice against the bacterium Staphylococcus aureus. Infect Immun 76: 4574–4580.
  36. 36. Luo G, Ibrahim AS, Spellberg B, Nobile CJ, Mitchell AP, et al. (2010) Candida albicans Hyr1p confers resistance to neutrophil killing and is a potential vaccine target. J Infect Dis 201: 1718–1728.
  37. 37. Spellberg BJ, Ibrahim AS, Avanesian V, Fu Y, Myers C, et al. (2006) Efficacy of the anti-Candida rAls3p-N or rAls1p-N vaccines against disseminated and mucosal candidiasis. J Infect Dis 194: 256–260.
  38. 38. Spellberg BJ, Ibrahim AS, Avenissian V, Filler SG, Myers CL, et al. (2005) The anti-Candida albicans vaccine composed of the recombinant N terminus of Als1p reduces fungal burden and improves survival in both immunocompetent and immunocompromised mice. Infect Immun 73: 6191–6193.
  39. 39. Joly-Guillou ML, Wolff M, Pocidalo JJ, Walker F, Carbon C (1997) Use of a new mouse model of Acinetobacter baumannii pneumonia to evaluate the postantibiotic effect of imipenem. Antimicrob Agents Chemother 41: 345–351.
  40. 40. van Faassen H, KuoLee R, Harris G, Zhao X, Conlan JW, et al. (2007) Neutrophils play an important role in host resistance to respiratory infection with Acinetobacter baumannii in mice. Infect Immun 75: 5597–5608.
  41. 41. Song JY, Cheong HJ, Lee J, Sung AK, Kim WJ (2009) Efficacy of monotherapy and combined antibiotic therapy for carbapenem-resistant Acinetobacter baumannii pneumonia in an immunosuppressed mouse model. Int J Antimicrob Agents 33: 33–39.
  42. 42. Chiang DH, Wang CC, Kuo HY, Chen HP, Chen TL, et al. (2008) Risk factors for mortality in patients with Acinetobacter baumannii bloodstream infection with genotypic species identification. J Microbiol Immunol Infect 41: 397–402.
  43. 43. Dizbay M, Tunccan OG, Sezer BE, Hizel K (2010) Nosocomial imipenem-resistant Acinetobacter baumannii infections: Epidemiology and risk factors. Scand J Infect Dis.
  44. 44. Gomez J, Simarro E, Banos V, Requena L, Ruiz J, et al. (1999) Six-year prospective study of risk and prognostic factors in patients with nosocomial sepsis caused by Acinetobacter baumannii. Eur J Clin Microbiol Infect Dis 18: 358–361.
  45. 45. Jang TN, Lee SH, Huang CH, Lee CL, Chen WY (2009) Risk factors and impact of nosocomial Acinetobacter baumannii bloodstream infections in the adult intensive care unit: a case-control study. J Hosp Infect 73: 143–150.
  46. 46. Alsultan AA, Hamouda A, Evans BA, Amyes SG (2009) Acinetobacter baumannii: emergence of four strains with novel bla(OXA-51-like) genes in patients with diabetes mellitus. J Chemother 21: 290–295.
  47. 47. Choi CH, Hyun SH, Lee JY, Lee JS, Lee YS, et al. (2008) Acinetobacter baumannii outer membrane protein A targets the nucleus and induces cytotoxicity. Cell Microbiol 10: 309–319.
  48. 48. King LB, Swiatlo E, Swiatlo A, McDaniel LS (2009) Serum resistance and biofilm formation in clinical isolates of Acinetobacter baumannii. FEMS Immunol Med Microbiol 55: 414–421.
  49. 49. Kim SW, Choi CH, Moon DC, Jin JS, Lee JH, et al. (2009) Serum resistance of Acinetobacter baumannii through the binding of factor H to outer membrane proteins. FEMS Microbiol Lett 301: 224–231.
  50. 50. Russo TA, Beanan JM, Olson R, MacDonald U, Luke NR, et al. (2008) Rat pneumonia and soft-tissue infection models for the study of Acinetobacter baumannii biology. Infect Immun 76: 3577–3586.
  51. 51. McConnell MJ, Pachon J (2010) Expression, purification, and refolding of biologically active Acinetobacter baumannii OmpA from Escherichia coli inclusion bodies. Protein Expr Purif 77: 98–103.
  52. 52. McConnell MJ, Pachon J (2010) Active and passive immunization against Acinetobacter baumannii using an inactivated whole cell vaccine. Vaccine 29: 1–5.
  53. 53. McConnell MJ, Dominguez-Herrera J, Smani Y, Lopez-Rojas R, Docobo-Perez F, et al. (2010) Vaccination with outer membrane complexes elicits rapid protective immunity to multidrug-resistant Acinetobacter baumannii. Infect Immun 79: 518–526.
  54. 54. Piechaud M, Second L (1951) [Studies of 26 strains of Moraxella Iwoffi]. Ann Inst Pasteur (Paris) 80: 97–99.