Species-specific viability analysis of Pseudomonas aeruginosa, Burkholderia cepacia and Staphylococcus aureus in mixed culture by flow cytometry
© Rüger et al.; licensee BioMed Central Ltd. 2014
Received: 30 April 2013
Accepted: 25 February 2014
Published: 7 March 2014
Bacterial species coexist commonly in mixed communities, for instance those occurring in microbial infections of humans. Interspecies effects contribute to alterations in composition of communities with respect to species and thus, to the course and severity of infection. Therefore, knowledge concerning growth and viability of single species in medically-relevant mixed communities is of high interest to resolve complexity of interspecies dynamics and to support development of treatment strategies. In this study, a flow cytometric method was established to assess the species-specific viability in defined three-species mixed cultures. The method enables the characterization of viability of Pseudomonas aeruginosa, Burkholderia cepacia and Staphylococcus aureus, which are relevant to lung infections of Cystic Fibrosis (CF) patients. The method combines fluorescence detection by antibody and lectin labeling with viability fluorescence staining using SYBR®Green I and propidium iodide. In addition, species-specific cell enumeration analysis using quantitative terminal restriction fragment length polymorphisms (qT-RFLP) was used to monitor the growth dynamics. Finally, to investigate the impact of substrate availability on growth and viability, concentrations of main substrates and metabolites released were determined.
For each species, the time course of growth and viability during mixed culture cultivations was obtained by using qT-RFLP analysis in combination with flow cytometry. Comparison between mixed and pure cultures revealed for every species differences in growth properties, e.g. enhanced growth of P. aeruginosa in mixed culture. Differences were also observed for B. cepacia and S. aureus in the time course of viability, e.g. an early and drastic reduction of viability of S. aureus in mixed culture. Overall, P. aeruginosa clearly dominated the mixed culture with regard to obtained cell concentrations.
In combination with qT-RFLP analysis, the methods enabled monitoring of species-specific cell concentrations and viability during co-cultivation of theses strains. Experimental findings suggest that the predominance of P. aeruginosa over B. cepacia and S. aureus in mixed culture under the chosen cultivation conditions is promoted by more efficient substrate consumption of P. aeruginosa, and antagonistic interspecies effects induced by P. aeruginosa.
KeywordsViability analysis Mixed communities Flow cytometry T-RFLP Cystic fibrosis Pseudomonas aeruginosa Burkholderia cepacia Staphylococcus aureus Interspecies effects
Microbial infections in humans are often characterized by a highly complex community of multiple bacterial species. Interspecies effects contribute to alterations in the composition of communities with respect to species and thus, to the course and severity of microbial infections. Moreover, changes in the composition of communities and interspecies effects may affect efficacy of antibiotics with severe consequences on therapeutic success. Consequently, determination of the dynamics of individual species in mixed communities is of high interest. Therefore, not only absolute and specific cell enumeration is required, but also information regarding viability of species. The composition of bacterial mixed communities can be determined efficiently by terminal restriction fragment length polymorphisms (T-RFLP) analysis. This has been widely demonstrated in numerous studies [1–6]. However, only few reports present absolute and species-specific cell numbers. For quantitative characterization of mixed communities by T-RFLP, Trotha et al. introduced an internal quantification standard , an 16S ribosomal RNA (rRNA) gene fragment from a known species with a defined cell number. Schmidt et al. adapted this quantitative T-RFLP (qT-RFLP) method for species-specific cell enumeration of a three-species mixed model community, comprising P. aeruginosa, B. cepacia and S. aureus, relevant to infections of lung of Cystic Fibrosis (CF) patients . Furthermore, the authors characterized the growth of these species in a defined mixed culture in chemostat cultivations, and a mathematical chemostat model was established to identify interspecies effects . Finally, Riedele et al. used the qT-RFLP protocol to study the efficacy of the antibiotic ceftazidime on the growth of these species in mixed culture . While qT-RFLP method allows to discriminate between species and to quantify cell concentration, viability is not determined. The latter, however, is of crucial importance for assessing antibiotic efficacy in case cell damage does not result in cell lysis but in loss of cellular functions, e.g. membrane integrity. Only based on the combination of qT-RFLP and species-specific viability analysis the detailed description of growth dynamics and the thorough characterization of interspecies effects are feasible.
T-RFLP can also be used for selective detection of the viable cell fraction, when the method is modified as recently reported by Rogers et al., who stained cells with propidium monoazide (PMA) prior to cell disruption . This dye, which intercalates with DNA, is generally excluded from viable cells with intact membranes . By photo activation, PMA binding leads to irreversible modification of DNA, thus preventing DNA of dead cells with an permeabilized membrane from amplification by PCR . While the combination of standard T-RFLP with PMA-T-RFLP allows for discrimination between viable and dead cells, it has the disadvantage that it does not allow for identification of cells with a slightly damaged membrane, which may occur during growth due to short-term perforation of the cell wall during cell division and cell wall synthesis . Moreover, the PCR-based quantification of viable cells using PMA staining can be affected by the presence of a high number of dead cells in the sample . Due to these drawbacks a flow cytometric method for characterization of species-specific viability had been established. Flow cytometry provides a powerful tool for viability analysis of bacteria by applying fluorescent probes, which target or indicate specific cell functions such as respiratory activity, enzyme activity, substrate uptake, efflux pump activity, membrane potential or membrane integrity . Additionally, species discrimination can be achieved by species-specific fluorescence labeling of cells, e.g. by immunofluorescence using monoclonal antibodies. Flow cytometry has been widely applied for viability determination of bacteria, mainly by assessing membrane integrity of cells (see review ). Often, a nucleic acid double-staining (NADS) method is used using propidium iodide (PI) for identification of dead cells, and SYBR®Green I for total cell staining . This approach has been demonstrated successfully for a wide range of different species [17–23]. PI is generally excluded from cells with intact membranes, whereas it enters cells with permeabilized membranes, staining them by binding DNA as well as RNA . Concomitantly, SYBRGreen I penetrates all cells and intercalates selectively with double-stranded DNA . Therefore, fluorescence detection enables discrimination between viable and dead cells exhibiting an intact or permeabilized membrane, respectively. In contrast to PMA-T-RFLP, detection of cells with a slightly damaged membrane can be obtained after optimization of staining conditions, as recently demonstrated for S. aureus. For determination of species-specific viability by flow cytometry, fluorescence species-specific detection is a key prerequisite. Bacterial species can be detected specifically by fluorescence labeling with antibodies or lectins that bind specifically to epitopes or molecules on cell surface, and by labeling with nucleotide probes that hybridize specifically to complementary strands of 16S rRNA. Latter technique is not recommended for use in combination with viability staining, since labeling requires permeabilization of membranes. Even though fluorescence labeling using specific antibodies (immunofluorescence labeling) and lectins has been widely established in flow cytometry, the combination with viability staining has been used only very rarely to determine the species-specific viability in mixed cultures (see review ).
In this study, a flow cytometric method is presented for assessment of the species-specific viability in defined three-species bacterial mixed cultures comprising P. aeruginosa, B. cepacia and S. aureus, relevant to infections of the lung of CF patients. The approach combines species-specific fluorescence detection by lectin and antibody labeling with viability fluorescence staining using SYBR Green I and PI. Additionally, for growth characterization in mixed culture, species-specific cell enumeration analysis using qT-RFLP was applied. Finally, to study the effect of substrate availability on growth and viability, concentrations of main substrates and metabolites released into culture medium were quantified using an enzymatic assay and high performance liquid chromatography (HPLC) analysis.
Pseudomonas aeruginosa PAO1 was supplied by Kathrin Riedel (Department of Microbiology, Technical University Munich, Germany). Burkholderia cepacia DSM 7288 was supplied by the German Collection of Microorganisms and Cell Cultures (DSMZ, Braunschweig, Germany). Staphylococcus aureus ATCC 29213 was supplied by Brigitte König (Department of Medical Microbiology, Otto von Guericke University, Magdeburg, Germany).
For cultivation of bacteria, Gibco® cell culture basal medium powder M199 (without NaCO3) (Life Technologies, Carlsbad, CA, USA) buffered with phosphate was used. Additionally, nitrilotriacetic acid (NTA) was added to prevent precipitation. Briefly, 800 mL of ultrapure water, 16 mL of 0.25 mM NTA solution (Sigma-Aldrich, Steinheim, Germany) in 0.6 M NaOH and 25 mL of sodium potassium phosphate buffer (1.5 M NaH2PO4/K2HPO4, pH 7.0, Carl Roth, Karlsruhe, Germany) were mixed with the amount of powder indicated by the supplier and filled up to 1 L with ultrapure water .
Bacteria were grown in 250 mL wide-neck Erlenmeyer flasks incubated in a humidified orbital shake incubator (Kuehner, Birsfelden, Switzerland) at 37°C, rotation speed 200 rpm, eccentric radius 1.25 cm, and relative humidity of 85%. Cultivations of mixed and pure cultures were conducted. Inocula were prepared as described previously by Riedele and Reichl  from pure culture of each species. Briefly, cells were grown overnight in 20 mL of culture medium, subsequently harvested, centrifuged at 3,522 × g for 10 min at 4°C (Heraeus® Multifuge 1S-R, Thermo Scientific, Waltham, WA, USA), and washed with PBS (8 g/L NaCl, 0.2 g/L KCl, 1.15 g/L NaH2PO4, 0.2 g/L K2HPO4, pH 7.4, Carl Roth, Karlsruhe, Germany). Afterwards, suspensions were centrifuged again (3,522 × g, 10 min, 4°C), resuspended in 20 mL of fresh culture medium and cultivated for 1.5 h. These cells were inoculated in 50 mL fresh pre-warmed culture medium. For both mixed and pure cultures, the inoculation volume of each species was adjusted to a total starting cell concentration of 1 × 106 cells/mL. Therefore, optical density at 650 nm (OD650) (photometer Ultraspec 3000, Amersham Biosciences, Otelfingen, Switzerland) was adjusted for each species based on linear correlation between OD650 and cell concentration determined by flow cytometric absolute counting. Consequently, for mixed culture, the inoculation volume of each species was three times lower than for pure culture (ratio between starting cell concentrations of species corresponds to 1:1:1). Cells were then cultivated over a period of 32 h.
For testing staining conditions, species were cultivated in pure cultures. Cells were grown overnight in 20 mL of culture medium, washed and regrown in 20 mL of fresh culture medium as described before. In contrast to inocula preparation, cells were cultivated over a period of 5 h. From these cultures samples were taken after 2 h and 5 h (exponential and stationary phase) for testing staining.
All cultivations were conducted in three biological replicates.
Sample preparation before staining
Cells were harvested by centrifugation at 4,700 × g for 10 min at 4°C (Heraeus® Fresco, Thermo Scientific, Waltham, WA, USA) and subsequently resuspended in Ringer solution (39 mM NaCl, 1.4 mM KCl, 0.6 mM NaHCO3, 0.5 mM CaCl2•2H2O, pH 7.2, Carl Roth, Karlsruhe, Germany). For fluorescence staining, Ringer solution was supplemented with 0.05 mg/mL glutaraldehyde (GTA) (50% grade I, Sigma-Aldrich, Steinheim, Germany), 0.05% (m/v) BSA (Carl Roth, Karlsruhe, Germany), and 3 M KCl (Carl Roth, Karlsruhe, Germany) (pH 7.2). For analysis, samples were diluted with Ringer solution prior to staining if necessary to OD650 in a range of 0.01 to 0.04 to ensure total cell concentrations between 1 × 106 and 1 × 107 cells/mL.
To verify viability staining of dead cells, controls for membrane permeabilization (positive controls) were prepared for each species from pure cultures. Briefly, after resuspension in Ringer solution, samples were treated with 70% (v/v) isopropanol (Merck, Darmstadt, Germany) for 1 h at room temperature (RT). Subsequently, suspensions were centrifuged at 4,700 × g for 10 min at 4°C (see above) and washed. Then, cells were resuspended in Ringer solution and diluted to an OD650 in the range of 0.01 - 0.04.
Labeling of WGA with Mix-n-Stain™ CF™405S
For Gram-staining of S. aureus, working solutions of 0.18 mg/mL CF™405S conjugated wheat germ agglutinin (WGA) were prepared. Briefly, 75 μg of WGA (Vector Laboratories, Burlingame, CA, USA), diluted in ultrapure water with 0.1 M NaHCO3 (Carl Roth, Karlsruhe, Germany), were labeled with Mix-n-Stain™ CF™405S antibody labeling kit (Biotium Inc., Hayward, CA, USA) according to the protocol recommended by the manufacturer.
Antibodies for immunofluorescence detection of B. cepacia
For indirect immunofluorescence labeling of B. cepacia, primary monoclonal antibodies (1°Ab, mouse anti-Pseudomonas cepacia, IgG3, clone 1144/209, Biotrend Chemikalien GmbH, Köln, Germany) and R-phycoerythrin (R-PE) conjugated secondary monoclonal antibodies (2°Ab, goat anti-mouse, IgG, Life Technologies, Carlsbad, CA, USA) were applied. For every day of experiment, fresh working solutions of 10 μg/mL 1°Ab and 60 μg/mL 2°Ab were prepared in Ringer solution.
SYBR Green I and PI for viability staining
For staining, working solutions of 1:100 SYBR®Green I (10,000 × concentrate in DMSO, Life Technologies, Carlsbad, CA, USA) and 1 mg/mL propidium iodide (Sigma-Aldrich, Steinheim, Germany) were prepared in ultrapure water.
Four-color staining for viability assessment in mixed culture
Cells were fluorescently stained with established four-color staining protocol. Briefly, after preparation, cell suspensions were incubated with 20 μg/mL WGA-CF405S for 15 min in the dark at RT. Thereafter, suspensions were washed twice applying centrifugation at 4,700 × g for 10 min at 4°C (Heraeus® Fresco, Thermo Scientific, Waltham, WA, USA) and resuspension in Ringer solution. Subsequently, pelleted cells were resuspended in working solution of 1°Ab (10 μg/mL, final) and incubated for 1 h on ice. Afterwards, suspensions were washed as described above. Thereafter, cells were resuspended in working solution of R-PE conjugated 2°Ab (60 μg/mL, final) and incubated for 1 h on ice. After washing, cells were resuspended in Ringer solution and incubated simultaneously with SYBR Green I (dilution 5 × 103) and PI (5 μg/mL) for 20 min in the dark at RT.
In addition, SYBR Green I/PI double-stained controls were processed for each species (same washing procedure as described above). For this, untreated as well as isopropanol-treated cells (positive controls) from both exponential (t = 4 h) and stationary growth phases (t = 12 h) were used.
In this study, a CyFlow® space flow cytometer (Partec, Münster, Germany) equipped with a 16 mW 375 nm UV diode laser and a 20 mW 488 nm argon solid state laser was used for flow cytometric analysis. Forward (FSC) and side scatter (SSC) signals were collected at 488 nm. To reduce electronic background noise during analysis, SSC was defined as a discriminator. Threshold value was set to a lower limit of 300 (channel value) at a voltage of SSC of 260 mV. Fluorescence of WGA-CF405S was excited by the 375 nm laser and collected through a 455/50 nm band pass (BP) filter. R-PE immunofluorescence, SYBR Green I and PI fluorescence were excited by the 488 nm laser and collected through a 590/50 nm BP, 527/30 nm BP or a 630 nm long pass filter, respectively. Detected signals were amplified logarithmically (4 decades).
Degassed ultrapure water was applied as sheath fluid. Analysis was carried out with a sampling rate in the range of 100 to 1,000 particles/s. Samples were diluted accordingly with sheath fluid prior to analysis. To increase statistical significance, the total number of particles analyzed was set to 20,000 events for pure culture and to a minimum of 20,000 events for mixed culture samples, respectively. Data was collected with FloMax software (Version 2.70, Partec, Münster, Germany).
Flow cytometric data analysis
Analysis, compensation and gating of data were performed using FlowJo software (Version 7.6.4, Tree Star Ashland, OR, USA). Due to spectral overlapping, fluorescence signals of SYBR Green I, R-PE and PI were compensated. Therefore, for every species, single-stained controls were processed in each experiment with the respective dye or fluorescence conjugate. PI single-stained controls were performed with isopropanol-treated cells. Compensation matrices were determined based on positive fluorescence signals of single-stained controls and subsequently applied for data analysis.
Flow cytometric data is presented in 2-D graphs either in pseudo color dot plots or in 5% quantile contour plots. Fluorescence intensities are given as relative fluorescence units (RFU).
For determination of species-specific viability, manually set gates were applied based on control samples. To discriminate cells from background, a gate for cell detection was applied. Only events with SYBR Green I positive fluorescence (intensities ≥ 1 RFU) were referred to as cells. Single species were detected based on WGA-CF405S fluorescence and R-PE immunofluorescence signals using a fixed gate for species discrimination. Subsequently, for each species, viability subpopulations were detected based on SYBR Green I and PI fluorescence signals. Applied viability gates were defined separately for each species for each exponential and stationary growth phase. Taking WGA-associated aggregation of S. aureus cells into account, for this strain, an additional gate for viability detection of single cells was used. This gate was set manually based on scatter signals (SSC vs FSC) of a SYBR Green I/PI double-stained sample from pure culture, which showed predominantly single cells.
Species-specific cell concentrations by qT-RFLP
Growth of pure and mixed culture was determined by quantitation of species-specific cell concentrations using qT-RFLP analysis. Samples were treated and analyzed according to the description of Schmidt et al. . Briefly, two samples were taken at each sampling point during cultivation and analyzed in parallel. 1 mL of sample was mixed with an internal quantification standard (IQS), an aliquot of Campylobacter jejuni with a fixed cell concentration. DNA of mixed sample was extracted by enzymatic cell lysis followed by DNA purification applying a commercially available kit (QIAamp DNA Blood Mini Kit, QIAGEN, Hilden, Germany). 16S rRNA genes were amplified by a gene-specific and fluorescently labeled primer using Polymerase Chain Reaction (PCR) method. Amplicons were then purified using an agarose gel and a commercially available extraction kit (QIAquick Gel Extraction Kit, QIAGEN, Hilden, Germany). Subsequently, amplicons were restricted with an HhaI endonuclease (R0139L, New England Biolabs Inc., Ipswich, MA, USA). Finally, species-specific rDNA fragments were separated by capillary gel electrophoresis and detected by laser-induced fluorescence (CGE-LIF) using a Genetic Analyzer ABI Prism 3100 Avant (Life Technologies, Carlsbad, CA, USA).
Species-specific cell concentration was determined by calculating the ratio of detected peak area for the given species to the peak area of the IQS [7, 8]. Concentrations were declared as genome equivalents per mL (ge/mL) as described previously by Riedele and Reichl .
Analysis of substrates and metabolites
Samples were harvested by centrifugation at 16,200 × g for 10 min at 4°C (Heraeus® Fresco, Thermo Scientific Waltham, WA, USA). Supernatants were withdrawn and filtrated using a syringe (Injekt 2 mL, B. Braun AG, Melsungen, Germany) with a 0.2 μm filter (Spartan 13/RC, Whatman GmbH, Dassel, Germany), and stored at 4°C until analysis.
Extracellular concentrations of glucose, glutamate and glutamine in the culture medium were determined according to a protocol of Riedele and Reichl  with a validated enzymatic quantification method using a Bioprofile 100 Plus (Nova Biomedical, Waltham, MA, USA). Quantitation limits and standard deviation (SD) of the method were as follows: glucose: 1.022 mM, SD 0.100 mM; glutamate: 0.254 mM, SD 0.025 mM; glutamine: 0.162 mM, SD 0.016 mM.
Extracellular concentrations of metabolites 2-keto-D-gluconic acid (2-KDG) and gluconic acid released in the culture medium, were quantified by HPLC (Agilent 1200 series, Agilent Technologies, Inc., Santa Clara, CA, USA) equipped with a Rezex-ROA organic acid column 300 × 7.6 mm (Phenomenex, Aschaffenburg, Germany). The applied method was in agreement with the method used by Riedele and Reichl  and comprised 0.075 M H2SO4 as eluent with a flow rate of 0.5 mL/min. From each sample 10 μL were injected and separation was performed at 45°C (column). Metabolites were detected by a diode array detector (DAD G1315B, Agilent Technologies, Inc., Santa Clara, CA, USA) at 210 nm. Quantitation limits and SD of the method were as follows: 2-KDG: 0.155 mM, SD 0.016 mM; gluconic acid: 0.267 mM, SD 0.026 mM.
To compare results obtained under different (mixed versus pure culture) or identical cultivation conditions, either unpaired or paired Student t-tests (p < 0.05) were performed, respectively.
Characterization of viability using flow cytometry
Species-specific viability analysis in mixed culture
Assessment of growth and viability in pure and mixed culture cultivations
Maximum specific growth rates μ max in pure and mixed culture
0.88 ± 0.11
0 - 4
1.22 ± 0.05
0 - 6
0.77 ± 0.02
0 - 6
0.86 ± 0.09
0 - 6
1.08 ± 0.37
0 - 4
1.29 ± 0.31
0 - 4
For P. aeruginosa, the viability in pure and mixed culture was initially high at about 99%. Then it remained relatively constant before decreasing after 12 h to achieve about 73% towards the end of cultivation (Figure 8(B)). For B. cepacia, viability in pure and mixed culture was as high as for P. aeruginosa in the beginning. However, viability was reduced during exponential growth phase after 4 h to about 89% in pure or 80% in mixed culture, respectively. Subsequently, viability increased in both cultures to a level of about 98% to remain constant from 8 h to 12 h (Figure 8(D)). Afterwards, viability decreased in both cultures slightly towards the end of cultivation. For S. aureus, the viability in pure and mixed culture was initially as high as determined for the Gram-negative bacteria. Viability differed slightly between pure and mixed culture during exponential growth phase (0 h to 4 h). However, at 8 h, viabilities achieved again similar levels of about 98%. Afterwards, the time course of viability of S. aureus differed significantly between pure and mixed cultures (Figure 8(F)). Although viability decreased in both cultures towards the end of cultivation, in mixed culture, it decreased earlier than in pure culture and initially at a faster rate. Briefly, viability in mixed culture dropped instantly from 8 h to 12 h to about 47%, whereas viability in pure culture remained high at about 97%. Afterwards, viability decreased continuously in both cultures to levels of about 13%. The frequency of dead cells of S. aureus in pure and mixed culture correlated well with the time course of viable cells over a cultivation period of 24 h or 12 h, respectively. Remarkably, for S. aureus in mixed culture, loss of viability resulted first in an increase of damaged cells and subsequent in an increase of dead cells, whereas in pure culture, damaged cells increased with dead cells. However, in both cultures, damaged cells decreased towards the end of cultivation, whereas dead cells continued increasing.
Species-specific determination of viability by flow cytometry
In this study, flow cytometry has been shown to be a highly capable technique for efficient determination of species-specific viability of P. aeruginosa, B. cepacia and S. aureus in defined mixed cultures relevant to lung infections of CF patients. Even though, a combination of the applied qT-RFLP method with PMA pre-treatment may enable detection of viable cells, in this study, the use of flow cytometry was preferred for viability analysis due to two practical limitations of PMA-T-RFLP: First, cells with slightly damaged membranes, which may occur during growth due to short-term perforation of the cell wall during cell division and cell wall synthesis , cannot be discriminated by PMA-T-RFLP from viable cells or dead cells, respectively. Second, quantification of viable cells by T-RFLP using PMA pre-treatment can be affected by the presence of a high number of dead cells in the sample (see review ), in particular, with a concentration of dead cells exceeding 104 cells/mL [30–33].
Viability was determined by flow cytometry assessing the membrane integrity of cells using an adapted NADS protocol (see Methods). PI was applied for identification of dead cells in combination with SYBR Green I for total cell staining. For each species, the protocol enabled detection of dead and viable cells with permeabilized or intact membranes, respectively. It is assumed that the loss of membrane integrity is associated with missing reproductive growth and missing metabolic activity and eventually leads to cell death . Thus, cells labeled as viable can be metabolically active or inactive as well as culturable or non-culturable cells. PI fluorescence signal intensities of dead cells increased most likely by quenching from SYBR Green I to PI when cells are double-stained . Fluorescence intensities of viable and dead cells varied between species, which can be largely attributed to differences in cell wall structure , total DNA content and base composition , as well as in efflux pump activity . Weak SYBR Green I fluorescence intensities, especially for viable cells of P. aeruginosa, suggest an out-pumping of dye from cells by active efflux pumps. In contrast, dead cells of P. aeruginosa exhibited intense SYBR Green I fluorescence, which is most likely due to missing efflux activity when membranes are permeabilized. For S. aureus, damaged cells were additionally detected, which were referred to as “cells with a slightly damaged membrane” by taking results of other authors [16, 23] into account. These cells are probably stained with a low amount of PI resulting in incomplete quenching from SYBR Green I to PI .
For assessment of species-specific viability in mixed cultures, Gram-specific staining of S. aureus and indirect immunolabeling of B. cepacia using fluorescently labeled WGA and monoclonal antibodies, respectively, were employed successfully in combination with the adapted NADS protocol. However, the establishment of the method was very time consuming, since every single staining condition had to be tested separately for each bacterial species. Moreover, such an approach can only be applied for bacteria cultivable in pure culture, since labels and viability dyes need to be tested a priori for each species. Thus, the use of such technique is restricted to defined mixed cultures. The established four-color staining method allowed for efficient specific detection of P. aeruginosa, B. cepacia and S. aureus in mixed culture samples and subsequent determination of viability. WGA was shown to bind exclusively to S. aureus, most likely to the outer peptidoglycan layer of the cell wall, since it is known to bind specifically to N-acetylglucosamine and N-acetylneuroaminic residues . The fact that WGA does not bind to Gram-negative bacteria in mixed culture is most probably attributed to the presence of an outer membrane . WGA staining of S. aureus was as efficient and reproducible as presented in a previously published report for specific detection of S. aureus in binary mixed cultures . Moreover, the binding capacity of WGA remained stable over the time period covered in the conducted cultivations, as demonstrated in pure culture. Indirect immunolabeling allowed for efficient specific detection of B. cepacia in mixed culture samples, when four-color staining method was applied. Cross reaction of both monoclonal antibodies to S. aureus was also observed, and is most probably attributed to the presence of protein A in the cell wall of this strain. Protein A is known to react with antibodies [39, 40], particularly with high affinity to immunoglobulin G . Specific detection of B. cepacia by immunolabeling was very efficient and reproducible, but reduced recoveries were observed during the exponential growth phase. This may be explained by low accessibility of surface-exposed epitopes at proliferation. This is in agreement with conclusions made from insufficient immunofluorescence labeling of bacteria in a report of Hughes et al., who suggested a cell cycle-dependent exposure of the targeted outer membrane protein of the species of interest . Overall, the cell recoveries of specifically detected species were very high for the obtained samples throughout the cultivations, as demonstrated for pure cultures. However, they were less than 100%. Accordingly, with respect to species-specific labels, false negative counts of B. cepacia and S. aureus cells cannot be excluded completely. Consequently, this may have a slight impact on the detected relative frequencies of viable and dead P. aeruginosa. However, for the purpose of this study describing the viability dynamics in mixed culture, the specificity of this protocol was sufficiently high. For other purposes a third species-specific label may be advisable.
Mixed culture effects on viability and growth
To investigate mixed culture effects on viability and growth of the three single species, mixed culture as well as pure culture cultivations were performed. Species-specific viability was assessed using the established flow cytometric method. Growth of single species was assessed by quantification of species-specific cell concentrations using qT-RFLP analysis. To investigate a possible impact of cell concentrations at time point of inoculation onto dynamics in the mixed culture, cultivations were carried out with one-log-reduced starting cell concentrations in comparison to cultures conducted in the study of Riedele and Reichl . However, the ratio between species in mixed culture was maintained.
For all species, analysis of cell concentrations by qT-RFLP revealed clear differences in growth dynamics between mixed and pure culture. P. aeruginosa showed improved growth in mixed culture. According to conclusions drawn by Riedele and Reichl from their experiments this extended exponential growth phase is most likely due to the reduced starting cell concentrations in mixed culture compared to pure culture (see Methods), which enabled an increasing number of cell divisions while the substrate is consumed until depletion . This is supported by the finding that levels of glutamine and glucose dropped below the detection limit after 4 h or 8 h, respectively, following comparable time profiles in mixed and pure culture. Furthermore, in both cultures, level of gluconate dropped below the detection limit after 4 h or 8 h, respectively. However, the higher specific growth rate in mixed culture compared to pure cultures may be caused by an unknown interspecies effect and remains to be identified. In case of B. cepacia, growth stagnated in mixed culture after 6 h of cultivation, whereas growth in pure culture was observed until the end of cultivation. These differences may be explained partially by competition for glutamine with P. aeruginosa during growth. This is supported by the finding that glutamine was consumed in mixed culture as fast as in pure culture of P. aeruginosa and thus, faster than in pure culture of B. cepacia. Furthermore, growth stagnation of B. cepacia in mixed culture may be caused by antagonistic interaction through action of inhibitory active substances against B. cepacia, e.g. pyocins, produced by P. aeruginosa. The latter could further explain the decrease of cell concentrations of B. cepacia in mixed culture towards the end of cultivation. In fact, the PAO1 strain is known to produce pyocins [43, 44], and its inhibitory activity against B. cepacia was demonstrated in a study of Bakkal et al. , in which different clinical strains of B. cepacia and P. aeruginosa isolated from CF patients were tested in mixed culture. Although Riedele and Reichl  suggested in their study no significant alterations for cell doublings of B. cepacia between growth in pure and mixed culture, the cell concentrations clearly reveal the same trend towards the end of cultivation as observed in this study. However, the mode of action of inhibitory active substances against B. cepacia produced by P. aeruginosa remains to be elucidated. Despite of this, obtained results indicate no antagonistic interactions from S. aureus to P. aeruginosa or to B. cepacia. The latter is in agreement with findings of a previously published study, in which these strains were characterized in binary mixed cultures .
For S. aureus, mixed culture cultivations did not affect growth of single species. Interestingly, other authors reported inhibition of growth in similar mixed cultures [10, 46], possibly caused by interspecies competition for glucose and glutamine  as well as through action of antistaphylococcal pyocyanine or pseudomonas quinoline signals (PQS) produced by P. aeruginosa[46–48]. Although the ratio between species used to initiate mixed culture experiments was similar to the study of Riedele et al. , in this study, growth characteristics of S. aureus were comparable between mixed and pure cultures. This is probably attributed to more favorable growth conditions for the Gram-positive bacteria in mixed culture at reduced starting cell concentrations of each species, e.g. due to the higher ratio of initial substrate-to-biomass . However, S. aureus seems to be outcompeted during stationary growth phase, as cell concentrations decreased in mixed culture towards the end of cultivation. This may be explained by action of inhibitory and lytic active substances produced by the competing species. Especially, P. aeruginosa is known to produce antistaphylococcal virulence factors, either bactericidal active, e.g. phenazine pyocyanine [50, 51], or bacteriolytic active, e.g. LasA protease . This hypothesis is further supported by results obtained in a proteomic study published recently by Kluge et al., where induction of phenazine synthesis of P. aeruginosa was suggested due to increased expression levels of PhzS, PhzD and PhzG2 in a similar mixed culture . Additionally, the authors found for S. aureus an increased expression level of an alkyl hydroperoxide reductase, which typically evokes resistance against oxidative stress. Despite of antistaphylococcal action of P. aeruginosa in mixed culture, it is likely, that virulence factors of B. cepacia also contribute to lysis of S. aureus, e.g. peptidoglycan hydrolases . This interaction, however, still needs to be demonstrated. Cell concentrations of B. cepacia in pure and mixed culture determined by qT-RFLP might, however, be underestimated, in particular at time point of inoculation. Although cell concentrations were adjusted (see Methods), the determined values were up to one-log unit below concentrations measured for P. aeruginosa and S. aureus. In contrast, flow cytometry suggested for B. cepacia a cell concentration in mixed culture at time point of inoculation to as high as adjusted (see Methods). Detected relative frequencies revealed a ratio between starting cell concentrations of species of about 1:1:1 (Figure 7(C)).
In general, viability of species shifted over the cultivation period. Experimental data indicates that the loss of viability in pure culture during stationary phase, particularly for P. aeruginosa and S. aureus, is a consequence of the depletion of the main substrates glucose, glutamine and glutamate within the first 12 h of cultivation. Moreover, gluconate and 2-KDG were also depleted within this time period, which are intermediates produced via extracellular glucose oxidation by P. aeruginosa and B. cepacia[54, 55]. With depletion of nutrients the metabolic activity decreases and active transports are impaired, which eventually leads to permeabilization of cytoplasmic membranes . In contrast, viability of B. cepacia in pure culture remained relatively constant throughout the entire cultivation period, although the main substrates and metabolites were also depleted within the first 12 h of cultivation. Interestingly, in this phase, growth of B. cepacia was still detected by increasing cell concentrations by qT-RFLP analysis. The latter suggests an uptake of other substrates available for growth in the culture medium, e.g. amino acids. Reduced viability levels during exponential growth phase, as observed most prominently for S. aureus, may be caused by PI false positive stained cells. This can probably be attributed to the entry of PI due to short-term perforation of cell walls during cell division and cell wall synthesis [13, 56]. Additionally, for S. aureus, aggregates of viable and dead cells might also increase total number of damaged bacteria due to clumping during growth .
Mixed culture cultivation impaired viability of B. cepacia and S. aureus, but did not affect viability of P. aeruginosa. For B. cepacia, viability in mixed cultures was reduced slightly compared to pure cultures from 12 h to 32 h. This may be caused by action of inhibitory pyocins produced by P. aeruginosa, as discussed above. For S. aureus, clear differences in the time course of viability in mixed and pure cultures were found. In mixed culture, viability decreased earlier and initially at a faster rate than in pure culture. This can most probably be explained by antagonistic interactions from Gram-negative bacteria towards S. aureus, most likely from P. aeruginosa due to dominance with regard to cell concentrations in mixed culture. Antistaphylococcal action can be transmitted by expressed virulence factors, e.g. pyocyanine or LasA protease, as discussed above. However, earlier reduction in viability of S. aureus in mixed culture may be additionally caused by other virulence factors, e.g. peptidoglycan hydrolases produced by B. cepacia. Moreover, differences in dynamics of damaged and dead cells of S. aureus between pure and mixed culture clearly suggest the presence of various damaging processes in mixed culture, differing at least in time of action, which finally lead to a loss of membrane integrity. In general, the detection of damaged S. aureus cells might reflect a slower damaging process of membranes than for B. cepacia and P. aeruginosa, which is most probably due to differences in cell wall structures. Interestingly, for B. cepacia and S. aureus in mixed culture, a simultaneous increase of relative frequency of dead cells and a decrease of cell concentration was observed. These results suggest co-occurrence of cell dead (loss of membrane integrity) and lysis, which would further support simultaneous action of a set of various antagonistic interspecies effects during co-cultivation, differing in mode and time of action. Despite of this, synergistic interactions between the species cannot be excluded. For instance, Riedel et al. reported in their study of increased pathogenicity of B. cepacia induced by P. aeruginosa via quorum sensing signaling . However, proteome data presented in a recently published report of Kluge et al. suggested no synergistic interspecies effects between the three species of interest in a similar mixed culture .
In the presented study, iron availability in the culture medium was not analyzed, although it might have a certain impact on growth and viability of single species in mixed culture. Iron limitation in medium in mixed culture will probably evoke interspecies effects for competition for remaining iron. Moreover, the expression of virulence factors might be regulated based on iron occurrence, as reported for P. aeruginosa for a large number of factors [59, 60]. The impact of iron availability on growth and viability in the mixed culture remains to be clarified in further studies.
Overall, P. aeruginosa clearly dominated the mixed culture after 6 h of cultivation, with regard to the obtained cell concentrations. This emphasizes the predominance of P. aeruginosa over B. cepacia and S. aureus in the mixed culture under the chosen cultivation conditions, particularly due to very efficient substrate consumption of P. aeruginosa. Additionally, obtained growth and viability results suggest predominance of P. aeruginosa by induced antagonistic interspecies effects against B. cepacia and S. aureus. Interestingly, in patients with CF disease, P. aeruginosa is also often found to dominate late-term lung infections. This suggests that P. aeruginosa is dominant over B. cepacia and S. aureus in mixed community under a variety of growth conditions.
A three-species mixed culture comprising P. aeruginosa, B. cepacia and S. aureus was characterized using a combination of analytical assays for monitoring species-specific cell concentrations and viabilities as well as determination of substrates and extracellular metabolites in the culture medium. The approach allowed for a comprehensive description of mixed culture dynamics of bacteria relevant to lung infections of CF patients, and enabled the identification of interspecies effects. In addition, the characterization of species-specific viability by flow cytometry provided insights into dynamics of cell damage in mixed cultures.
The authors cordially thank Corina Siewert for excellent technical assistance.
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