In vivo bioluminescent imaging permits the visualization of bacteria in live animals, allowing researchers to monitor, both temporally and spatially, the progression of infection in each animal. We sought to engineer stably luminescent clinical strains of Staphylococcus aureus, with the goal of using such strains in mouse models. The gram-positive shuttle vector pMAD was used as the backbone for an integration plasmid. A chloramphenicol resistance gene, a modified lux operon from Photorhabdus luminescens, and approximately 650 bp of homology to the chromosome of the USA300 S. aureus strain NRS384 were added, generating plasmid pRP1195. Electroporation into strain RN4220 followed by temperature shift led to integration of pRP1195 into the chromosome. The integrated plasmid was transferred to clinical strains by phage transduction. Luminescent strains displayed no in vitro growth defects. Moreover, luminescence was stable in vitro after three rounds of subculture over 48 hours of growth in the absence of antibiotics. Mice were infected with a luminescent strain of NRS384 in skin and intravenous models. In a mouse skin model, luminescent bacteria were present in lesions that formed and cleared over the course of several days, and in an intravenous model, bacteria inoculated in the mouse tail vein were observed spreading to multiple tissues. No statistically significant difference in virulence was observed between NRS384 and the luminescent strain in either infection model. These preliminary data suggest that this luminescent USA300 strain is suitable for use in mouse models. Similar strains were engineered using other sequenced clinical strains. Because these strains are stably luminescent, they should prove useful in animal models of infection.
Citation: Plaut RD, Mocca CP, Prabhakara R, Merkel TJ, Stibitz S (2013) Stably Luminescent Staphylococcus aureus Clinical Strains for Use in Bioluminescent Imaging. PLoS ONE 8(3): e59232. https://doi.org/10.1371/journal.pone.0059232
Editor: Holger Rohde, Universitätsklinikum Hamburg-Eppendorf, Germany
Received: September 21, 2012; Accepted: February 13, 2013; Published: March 12, 2013
This is an open-access article, free of all copyright, and may be freely reproduced, distributed, transmitted, modified, built upon, or otherwise used by anyone for any lawful purpose. The work is made available under the Creative Commons CC0 public domain dedication.
Funding: Stanley Kim was supported by the Food and Drug Administration Medical Countermeasures Initiative. Strain NRS384 was obtained through the Network on Antimicrobial Resistance in Staphylococcus aureus (NARSA; www.narsa.net) Program, supported under National Institute of Allergy and Infectious Diseases/National Institutes of Health Contract No. HHSN272200700055C. The funders had no role in study design, data collection and analysis, decision to publish, or preparation of the manuscript.
Competing interests: The authors have declared that no competing interests exist.
Staphylococcus aureus is responsible for a variety of illnesses, including skin and soft tissue infections, pneumonia, septic arthritis, endocarditis, and osteomyelitis. The incidence of infections with antibiotic-resistant strains is increasing, with community-acquired methicillin-resistant S. aureus (CA-MRSA) becoming a particular concern (reviewed in ). Studies of these infections using animal models are facilitated by the use of bioluminescent imaging (BLI), which allows tracking of the spatial progression of infection in individual animals over time.
For use in BLI, bacterial strains should be clinically relevant and brightly and stably luminescent. Although there are several reports using luminescent S. aureus strains in vivo , , , , , the strains used are often not stably luminescent. One issue is that if the genes required for luminescence are carried on a plasmid, then the signal may be lost in vivo in the absence of antibiotic selection, due to plasmid segregation. Moreover, in some of these reports, the strains used in BLI were luminescent versions of laboratory-passaged strains, which may not be clinically relevant to current human diseases.
In this report, we describe an integrative plasmid developed to engineer stably and brightly luminescent clinical strains of S. aureus. In preliminary experiments, we used one of these strains, a luminescent version of the USA300 MRSA strain NRS384, in two mouse models of infection. We found that the luminescent strain was as virulent as the wild-type strain, and that progression of the infections could be followed easily over time using BLI. The integrative plasmid and the luminescent clinical strains described here should prove useful in these and other animal models of S. aureus infection.
Materials and Methods
Bacterial strains and plasmids
Bacterial strains and plasmids are listed in Table 1. The backbone for the integrative plasmid was the shuttle plasmid pMAD . The kanamycin resistance gene aphA(3), originally from S. aureus , was amplified from pSS4332  and inserted at the BglII site of pMAD, yielding plasmid pRP1179. Approximately 660 bp in the area of USA300HOU_1102 (annotated as a pseudogene in the sequenced USA300 strain TCH1516 ) was amplified from the S. aureus USA300 strain NRS384 and inserted into BamHI/SalI-digested pRP1179, generating pRP1186. Next, a modified luxBADCE operon, originally from Photorhabdus luminescens , was amplified from a derivative of pSS4530  such that the operon was under the control of a modified gapA promoter with consensus -35, extended -10, and -10 regions (TTGACACTGCGTAAGGTTTGTGTTATAAT) and inserted at the EagI site of pRP1186, yielding pRP1190. Separately, the chloramphenicol resistance gene cat (originally from pC194 ) was amplified from pBT2 , digested with KpnI, and inserted into similarly digested pMAD, generating plasmid pRP1192. Finally, a 6.8 kb BamHI-SalI fragment of pRP1190 (including the USA300HOU_1102 homology and the lux operon) was ligated with similarly digested pRP1192, generating pRP1195 (Fig. 1). Thus, pRP1190 (with aphA(3)) is suitable for use in S. aureus strains that are kanamycin-sensitive, whereas pRP1195 (with cat) is suitable for use in strains that are chloramphenicol-sensitive. Plasmids were transformed into RN4220 by electroporation as previously described  followed by growth at 30°C. For integration into the bacterial chromosome, strains were grown at 30°C overnight in tryptic soy broth (TSB) with 10 µg/ml chloramphenicol, followed by subculture (1∶100 dilution) in TSB without antibiotics at 30°C for 1–2 h, shift to 43°C for 6–7 h, serial dilution, plating on tryptic soy agar (TSA) with 10 µg/ml chloramphenicol, and overnight incubation at 43°C. Plates were imaged, and luminescent colonies were selected for further passage and analysis. Integration at the intended site was confirmed by PCR. Freely replicating or integrated plasmids were transferred to clinical strains by phi80 phage transduction as previously described .
Features added to the pMAD backbone as described in Materials and Methods include: cm, chloramphenicol resistance gene; homology, PCR fragment in the area of pseudogene USA300_HOU1102 amplified from NRS384; LuxB, A, D, C, and E, modified lux operon from Photorhabdus luminescens.
In vitro growth and luminescence
To assess the kinetics of growth in vitro, strains were grown overnight in TSB and subcultured at a dilution of 1∶100, and OD600 readings were taken at regular intervals. To assess the stability of luminescence following extended in vitro growth, strains were grown in TSB and subcultured three times (at 16, 24, and 40 h) in the absence of antibiotics, and after 48 h, serial dilutions were plated on TSA and incubated at 37°C.
Animal studies were conducted at the animal facility of the Center for Biologics Evaluation and Research, under the guidelines of the Institutional Animal Care and Use Committee (IACUC), which approved the animal protocols used. All efforts were undertaken to minimize animal suffering. For a skin and soft tissue model of infection, TSB without (NRS384) or with (SAP149) 10 µg/ml chloramphenicol was inoculated at a dilution of 1∶50 with an overnight culture, incubated at 37°C with shaking, grown to an OD600 of approximately 0.8, and then centrifuged at 4000× g for 15 min. The pellet was resuspended in PBS, and bacteria were counted using a hemocytometer and diluted in PBS to a concentration of 1.0×1011 cells/ml. The bacterial count was confirmed by serial dilution and plating of the suspension. BALB/c mice were anesthetized intraperitoneally with 2 mg ketamine (Ketaject, Phoenix Pharmaceutical, St. Joseph, MO) and 0.1 mg xylazine (AnaSed, Akorn, Decatur, IL). Left ears were swabbed with 70% isopropanol, and a Morrow Brown needle (Morrow Brown Allergy Diagnostics, Oakhurst, NJ) was used to administer 1.0×109 CFU to the left ear of each mouse. The mean delivered dose was found to be approximately 2.0×107 CFU/lesion with a standard deviation of 1.0×107 CFU/lesion. Mice were euthanized on days 1, 4, and 7 following infection, and the left ears were cleansed with 70% ethanol. Ear pinnae were removed using sterile scissors and homogenized in 500 μl of PBS with a Polytron PT 1200 handheld homogenizer (Kinematica, Bohemia, NY). Serial dilutions were plated on TSA and incubated overnight at 37°C, and CFU per ml of homogenate was calculated.
For an intravenous model, TSB without (NRS384) or with (SAP149) 10 µg/ml chloramphenicol was inoculated at a dilution of 1∶100 with an overnight culture, incubated at 37°C with shaking, and grown to an OD600 of approximately 0.63. This absorbance reading was found to correspond to approximately 3.66×108 CFU/ml (data not shown). The culture was centrifuged at 4000× g for 10 min, and the pellet was resuspended in PBS. BALB/c mice were injected via the tail vein with 2×107 CFU of NRS384 or SAP149 in a volume of 100 µl. The dose was verified by serial dilution and plating on TSA. Over the course of 21 days, moribund mice were euthanized according to an IACUC-approved protocol.
Imaging, image processing, and statistical analyses
To follow the progression of the infection, mice were imaged with an IVIS-50 instrument (Caliper Life Sciences, Hopkinton, MA) as previously described . Agar plates were imaged with an LAS-3000 imaging system (Fujifilm Medical Systems, Stamford, CT). Typical settings for assessing luminescence were f/0.85, 1 min, no filter. Images were adjusted for brightness and contrast using PhotoShop CS3 (Adobe Systems, San Jose, CA). Prism 5 (GraphPad Software, La Jolla, CA) was used for statistical analyses.
Development and integration of a luminescence plasmid
In order to engineer strains of S. aureus that would be stably luminescent, we sought to integrate a plasmid into the bacterial chromosome. The shuttle plasmid pMAD , which contains a temperature-sensitive replication module, was used as the backbone. Because some clinical strains already carry erythromycin resistance, a gene encoding resistance to chloramphenicol  was added. In a search for potential integration sites, we considered pseudogenes in the chromosome of the sequenced USA300 strain TCH1516  (Accession NC_010079.1). We selected pseudogene USA300HOU_1102 (Gene ID: 5776586) as the site for integration, for the following reasons: 1) it is a pseudogene in several sequenced strains, decreasing the likelihood that insertion at that site would affect fitness or virulence; 2) flanking genes are encoded “toward” it, decreasing the likelihood of polar effects; and 3) the region is 98–100% conserved in 32 sequenced S. aureus strains, including strains commonly used in research (e.g., MW2, Newman, COL, and N315), enabling the use of homology cloned from one strain for integration of the plasmid into the chromosomes of multiple strains. A 662-bp PCR fragment in the area of pseudogene USA300HOU_1102 (coordinates 1171718-1172379) was amplified from the USA300 strain NRS384 and inserted into the plasmid, to permit integration of the plasmid into the bacterial chromosome via homologous recombination. Lastly, a modified lux operon originally from Photorhabdus luminescens ,  was added, under the control of a strong constitutive promoter, leading to the development of the integrative plasmid pRP1195 (Fig. 1).
The plasmid was transformed by electroporation into the restriction-deficient laboratory strain RN4220, and chromosomal integrants were selected by temperature shift in the presence of chloramphenicol. Phage phi80 was used to transduce the integrated plasmid into the strains NRS384, MW2, and Newman. In later experiments, freely replicating plasmid pRP1195 was transduced into the clinical strains and then integrated into the chromosomes of those strains by temperature shift in the presence of chloramphenicol. The site of integration was confirmed by PCR (Fig. 2) and sequencing.
Primers specific for pRP1195 and chromosomal sequences were used in PCR reactions with chromosomal DNA from SAP231 (integrant) and NRS384 (WT) as templates. Primers used were: C1, (GCATGCCATTTTCTTTATCATAAGTG); C2, (CAGTTATGGTGGTCTTATAGAGAGAC); P1, (CAGTCAGAGGAGCGCCGACAACACC); P2, (TTTCGTTTGTTGAACTAATGGGTGC). Molecular weight in kilobases is indicated on the left.
Evaluation of luminescent strains in vitro
The luminescent strains exhibited similar growth kinetics in vitro, relative to each other and to the parental strains (Fig. 3A). In order to assess the stability of the luminescence, the strains were grown in broth culture and subcultured three times over the course of 48 h in the absence of antibiotics, and serial dilutions were plated. All colonies were found to be luminescent (Fig. 3B), confirming the stability of the integrated plasmid in vitro.
A) In vitro growth curves. Strains were grown overnight in TSB with (luminescent strains) or without (parental strains) 10 µg/ml chloramphenicol and subcultured at a dilution of 1∶100 in TSB without antibiotic. MW2-Lux, SAP227; Newman-Lux, SAP229; NRS384-Lux, SAP231. B) Luminescence after in vitro outgrowth. SAP231 was grown in TSB and subcultured three times over the course of 48 h. Serial dilutions were plated on TSA in the absence of antibiotics, and plates were imaged as described in Materials and Methods.
In an intravenous model, mice were injected via the tail vein with the wild-type USA300 strain (NRS384) or with the luminescent derivative (SAP149). When mice infected with the luminescent strain were imaged over the course of 6d, luminescent bacteria were apparent by day 1 and were observed to have spread throughout the body of each animal (Fig. 4A). Mice injected with either strain succumbed to the infection, with time of death varying from 1 to 21 days (Fig. 4B). There was no statistically significant difference between the survival curves of mice infected with each strain.
In an intravenous model, mice were injected via the tail vein with either the wild-type USA300 strain (NRS384) or the luminescent strain (SAP149). Mice injected with the luminescent strain were imaged over the course of 6d (A); images are representative. There was no statistically significant difference in survival of mice injected with the two strains (B) by either the log-rank (Mantel-Cox) Test (P = 0.46) or the Gehan-Breslow-Wilcoxon Test (P = 0.68); n = 20 mice per group.
In a skin and soft tissue model of infection, wild-type or luminescent bacteria were transferred to a Morrow-Brown needle and inoculated onto the left ear of mice. Mice infected with the luminescent strain SAP149 were imaged over the course of several days (Fig. 5A). Luminescence was apparent on day 1 following infection, increased over the course of 3–5 days, and then began to wane. By day 7, the infection had nearly cleared, as evidenced by the reduction in luminescence and confirmed by bacterial counts (Fig. 5B). There was no statistically significant difference in CFU per ml of ear pinna homogenate between mice infected with the luminescent strain and those infected with the wild-type USA300 strain, suggesting that integration of the plasmid into the bacterial chromosome did not affect virulence.
In a skin and soft tissue model (SSTI), mice were inoculated in the left ear with NRS384 or SAP149. Mice inoculated with SAP149 were imaged over the course of several days (A); images are representative. On days 1, 4, and 7 post infection, mice were euthanized and ear pinna homogenates were serially diluted and plated (B). There was no statistically significant difference in CFU recovered per ml of homogenate between mice infected with each strain (two-tailed t-test; P = 0.55; bars represent 95% confidence interval; n = 8 mice per group).
In a previous study, we found that Bacillus anthracis engineered to be luminescent via integration of a plasmid by homologous recombination is very stably luminescent, even in the absence of antibiotic selection . In the present work, we used a similar approach to engineer luminescent S. aureus strains and found comparable stability. Our initial methods included integration of pRP1195 into RN4220, followed by transduction of the integrated plasmid into the strains NRS384 (USA300), MW2, and Newman. Because phage phi80 can package up to 42 kb of DNA , such an approach is less than ideal, as RN4220-specific DNA sequences could potentially be transferred to the target strain. To avoid such a possibility, we subsequently engineered additional luminescent strains by transducing the freely replicating plasmid from RN4220 to the target strains, shifting to the non-permissive temperature for plasmid replication, and isolating integrants. These strains should differ from the parent strains only in the presence of the integrated plasmid and should therefore prove useful in studies of S. aureus pathogenesis.
We thank Gail Christie for providing phage phi80 and Stanley Kim for technical assistance. NRS384 was obtained through the Network on Antimicrobial Resistance in Staphylococcus aureus (NARSA; http://www.narsa.net).
Conceived and designed the experiments: RDP TJM SS. Performed the experiments: RDP CPM RP. Analyzed the data: RDP CPM RP TJM SS. Wrote the paper: RDP SS.
- 1. Deleo FR, Otto M, Kreiswirth BN, Chambers HF (2010) Community-associated meticillin-resistant Staphylococcus aureus. Lancet 375: 1557–1568.
- 2. Pribaz JR, Bernthal NM, Billi F, Cho JS, Ramos RI, et al. (2012) Mouse model of chronic post-arthroplasty infection: noninvasive in vivo bioluminescence imaging to monitor bacterial burden for long-term study. J Orthop Res 30: 335–340.
- 3. Francis KP, Joh D, Bellinger-Kawahara C, Hawkinson MJ, Purchio TF, et al. (2000) Monitoring bioluminescent Staphylococcus aureus infections in living mice using a novel luxABCDE construct. Infect Immun 68: 3594–3600.
- 4. Kadurugamuwa JL, Sin L, Albert E, Yu J, Francis K, et al. (2003) Direct continuous method for monitoring biofilm infection in a mouse model. Infect Immun 71: 882–890.
- 5. Steinhuber A, Landmann R, Goerke C, Wolz C, Fluckiger U (2008) Bioluminescence imaging to study the promoter activity of hla of Staphylococcus aureus in vitro and in vivo. Int J Med Microbiol 298: 599–605.
- 6. Dumont AL, Nygaard TK, Watkins RL, Smith A, Kozhaya L, et al. (2011) Characterization of a new cytotoxin that contributes to Staphylococcus aureus pathogenesis. Mol Microbiol 79: 814–825.
- 7. Arnaud M, Chastanet A, Debarbouille M (2004) New vector for efficient allelic replacement in naturally nontransformable, low-GC-content, gram-positive bacteria. Applied and Environmental Microbiology 70: 6887–6891.
- 8. Gray GS, Fitch WM (1983) Evolution of antibiotic resistance genes: the DNA sequence of a kanamycin resistance gene from Staphylococcus aureus. Mol Biol Evol 1: 57–66.
- 9. Cybulski RJ Jr, Sanz P, Alem F, Stibitz S, Bull RL, et al. (2009) Four superoxide dismutases contribute to Bacillus anthracis virulence and provide spores with redundant protection from oxidative stress. Infect Immun 77: 274–285.
- 10. Highlander SK, Hulten KG, Qin X, Jiang H, Yerrapragada S, et al. (2007) Subtle genetic changes enhance virulence of methicillin resistant and sensitive Staphylococcus aureus. BMC Microbiology 7: 99.
- 11. Meighen EA (1991) Molecular biology of bacterial bioluminescence. Microbiol Rev 55: 123–142.
- 12. Loving CL, Khurana T, Osorio M, Lee GM, Kelly VK, et al. (2009) Role of anthrax toxins in dissemination, disease progression, and induction of protective adaptive immunity in the mouse aerosol challenge model. Infect Immun 77: 255–265.
- 13. Horinouchi S, Weisblum B (1982) Nucleotide sequence and functional map of pC194, a plasmid that specifies inducible chloramphenicol resistance. J Bacteriol 150: 815–825.
- 14. Bruckner R (1997) Gene replacement in Staphylococcus carnosus and Staphylococcus xylosus. FEMS Microbiol Lett 151: 1–8.
- 15. Bae T, Glass EM, Schneewind O, Missiakas D (2008) Generating a collection of insertion mutations in the Staphylococcus aureus genome using bursa aurealis. Methods Mol Biol 416: 103–116.
- 16. McNamara P (2008) Genetic manipulation of Staphylococcus aureus. In: Lindsay JA, editor. Staphylococcus: Molecular Genetics. Norfolk, United Kingdom: Caister Academic Press. 89–129.
- 17. Christie GE, Matthews AM, King DG, Lane KD, Olivarez NP, et al. (2010) The complete genomes of Staphylococcus aureus bacteriophages 80 and 80α—implications for the specificity of SaPI mobilization. Virology 407: 381–390.
- 18. Kreiswirth BN, Lofdahl S, Betley MJ, O'Reilly M, Schlievert PM, et al. (1983) The toxic shock syndrome exotoxin structural gene is not detectably transmitted by a prophage. Nature 305: 709–712.
- 19. Hunt C, Dionne M, Delorme M, Murdock D, Erdrich A, et al. (1999) Four pediatric deaths from community-acquired methicillin-resistant Staphylococcus aureus – Minnesota and North Dakota, 1997–1999. Jama-Journal of the American Medical Association 282: 1123–1125.
- 20. Baba T, Takeuchi F, Kuroda M, Yuzawa H, Aoki K-i, et al. (2002) Genome and virulence determinants of high virulence community-acquired MRSA. The Lancet 359: 1819–1827.
- 21. Duthie ES, Lorenz LL (1952) Staphylococcal coagulase; mode of action and antigenicity. J Gen Microbiol 6: 95–107.
- 22. Baba T, Bae T, Schneewind O, Takeuchi F, Hiramatsu K (2007) Genome sequence of Staphylococcus aureus strain Newman and comparative analysis of Staphylococcal genomes: polymorphism and evolution of two major pathogenicity islands. Journal of Bacteriology 190: 300–310.