Probiotics are defined as ‘live microorganisms which when administered in adequate amounts confer a health benefit on the host’(1). Lactic acid bacteria and bifidobacteria are commonly found in the human gastrointestinal tract (GIT), and represent the majority of commercial probiotics. Antimicrobial activity, exclusion or inhibition of pathogens, enhancement of the intestinal epithelial barrier function(Reference Resta-Lenert and Barrett2), ability to degrade indigestible food components(Reference He, Priebe and Zhong3) and immunomodulation(Reference Baken, Ezendam and Gremmer4–Reference Evrard, Coudeyras and Dosgilbert7) are some of the numerous beneficial effects reported. Probiotics are thereby widely used as food supplements, which calls for a proper evaluation of the microbes in order to substantiate the health claims. Guidelines for such evaluation have been provided by the FAO/WHO, with the intension to establish a set of minimum requirements for probiotic status(8). Viability after exposure to the different challenging environments encountered in the upper GIT, ability to prolong intestinal residence by adhesion to mucus and/or intestinal epithelial cells (IEC), and the potential to modulate the immune system are commonly assayed when screening for microbes with potential probiotic properties.
The Gram-positive, facultative anaerobe lactic acid bacterium Enterococcus faecalis is a common component of the human commensal flora, but has received substantial attention due to its ‘dualistic’ behaviour toward human health(Reference Franz, Stiles and Schleifer9, Reference Foulquie Moreno, Sarantinopoulos and Tsakalidou10). E. faecalis is recognised as a multi-resistant, opportunistic pathogen and has become one of the leading causes of nosocomial infections(Reference Linden and Miller11, Reference Fisher and Phillips12). The E. faecalis strain V583 was the first vancomycin-resistant clinical isolate reported in the USA, and represents a well-described pathogenic strain(Reference Sahm, Kissinger and Gilmore13, Reference Paulsen, Banerjei and Myers14). Intriguingly, E. faecalis is also made into commercial products marketed as probiotics, such as Symbioflor-1 (SymbioPharm GmbH). Symbioflor-1 has been reported to reduce the number of relapses in patients with chronic recurrent hypertrophic sinusitis, as well as the number and severity of relapses in patients with chronic recurrent bronchitis(Reference Habermann, Zimmermann and Skarabis15, Reference Habermann, Zimmermann and Skarabis16). According to the manufacturer, these beneficial effects are due to a ‘natural training effect on the immune system’ initiated by bacteria–host interactions in the intestine. This immunomodulatory effect is then distributed to various mucous membranes throughout the body, and defence systems located at the paranasal sinus and bronchial tract are thereby enhanced. Beneficial effects of probiotics on respiratory tract infections (RTI) have also been reported by others(Reference Guillemard, Tondu and Lacoin17, Reference Vouloumanou, Makris and Karageorgopoulos18). Vouloumanou et al. (Reference Vouloumanou, Makris and Karageorgopoulos18) evaluated the clinical evidence regarding probiotic use for the prevention of RTI and concluded that administration of probiotics may have a beneficial effect on the severity and duration of symptoms, but does not appear to reduce the incidence of RTI.
Variations can exist in the molecular mechanisms employed by the probiotic, pathogenic and commensal E. faecalis strains upon host interaction. Strain-specific differences in the ability to, for example, colonise the intestine and/or elicit an immune response are likely. Such knowledge will be valuable when evaluating the risk associated with using Enterococcus as food starter cultures or as probiotics. As it is not possible to differentiate between virulent and a-virulent enterococcal strains, the Panel on Biological Hazards of the European Food Safety Authority (EFSA) has not included any taxonomical unit within the enterococci genus in the list of Qualified Presumption of Safety (QPS) micro-organisms(19). Due to the increasing evidence of pathogenicity, species of Enterococcus will no longer be assessed unless new scientific information becomes available.
Our objective was to study different characteristics of Symbioflor-1, in comparison with the pathogenic E. faecalis strain V583 and three other E. faecalis isolates (Table 1). We used several in vitro methods that are commonly employed when screening for potential probiotic bacteria. In this way, our approach differs from the investigations reported where numerous microbes are assayed for putative probiotic properties.
Table 1 Enterococcus faecalis strains
Material and methods
Cells and culture conditions
E. faecalis strains V583(Reference Sahm, Kissinger and Gilmore13), Symbioflor-1(Reference Domann, Hain and Ghai20) (SymbioPharm), 62(Reference Brede, Snipen and Ussery21, Reference Solheim, Brekke and Snipen22), 158B(Reference Solheim, Brekke and Snipen22, Reference Solheim, Aakra and Snipen23) and LMGT3208(Reference Solheim, Brekke and Snipen22) were kindly provided by the Laboratory of Microbial Gene Technology and Food Microbiology (Department of Chemistry, Biotechnology and Food Science, University of Life Science, Norway). All E. faecalis strains were cultivated at 37°C in brain–heart infusion (BHI) medium (Oxoid). Lactobacillus reuteri DSM 20 016(Reference Kandler, Stetter and Kohl24) and L. plantarum NC8(Reference Shrago, Chassy and Dobrogosz25) were kindly provided by Nofima AS and anaerobically cultivated in de Man, Rogosa and Sharpe (MRS) medium (Oxoid) at 37 and 30°C, respectively. All strains were stored at − 80°C in 20 % (v/v) glycerol.
The human colon adenocarcinoma cell line Caco-2 (HTB-37™; American Type Culture Collection (ATTC)), monocytes and dendritic cells (DC) were maintained in Roswell Park Memorial Institute (RPMI)-1640 medium supplemented with 2 mm-l-glutamine, 100 μm-non-essential amino acids, 1 mm-sodium pyruvate (all from PAA Laboratories), 10 % heat-inactivated fetal calf serum and gentamicin (24 mg/l) (Lonza). All experiments and maintenance of tissue culture cells were carried out at 37°C in a 5 % CO2 humidified air atmosphere.
Assaying bacterial cultivability
Overnight cultures were diluted 1:50 in BHI medium with either neutral or HCl-adjusted pH values, as specified. Cell growth at 37°C was monitored spectrophotometrically (optical density at 600 nm) every 30 min using a Bioscreen instrument (Bioscreen C). Sterile BHI medium was used as negative control and for background correction.
Collection of physiological gastric and duodenal juices from the upper digestive tract
Human gastric juice (HGJ) and duodenal juice (HDJ) were collected from healthy volunteers. Aspiration of six fasting volunteers (aged between 20 and 30 years) was performed at Moss Hospital, Norway. The aspiration was approved by the Norwegian Ethics Committee, and written consent of participation was given. Juices were collected by placing a flexible three-lumen silicone tube (Maxter Catheters) through the nose or mouth. Correct tube placement was monitored by radiology. Instillation of a stimulatory solution (17·5 g/l sucrose, 450 mg/l NaCl, 800 mg/l l-phenylalanine and 575 mg/l l-valine in water) was performed simultaneously. Juices were collected in 50 ml tubes on ice, controlled for cross-contamination (colour and pH) and centrifuged (4500 g for 10 min) to remove mucus and cell debris. Samples were pooled, frozen as 5 ml samples and stored at − 80°C. The final pH was 1·5 for the HGJ and 8·0 for the HDJ.
Assaying cell viability by fluorescent staining and flow cytometry
Overnight bacterial cultures were diluted 1:50 in BHI medium and cultivated for 3 h at 37°C. Cells were washed and re-suspended in PBS (PAA Laboratories) to strain-specific densities (optical density at 600 nm) previously estimated to yield 1 × 108 colony-forming units (CFU)/ml by plate counting. After harvesting 0·5 ml cell suspension, the bacterial pellets were re-suspended in equal amounts of challenging or control solutions, and incubated for 30 min at 37°C. Cells were washed and re-suspended in PBS and stained with 2·5 μm-SYTO9 (Invitrogen) for 15 min at room temperature. After washing in PBS, cells were stained with 0·25 μg/ml propidium iodide (PI) (Invitrogen) for 2 min before flow cytometric analysis. SYTO9 is a membrane-permeable nucleic acid stain detected in the green channel (FL-2, fluorescein isothiocyanate), and PI is a membrane-impermeable red fluorescent nucleic acid stain detected in the red channel (FL-4, PI/phycoerythrin-Cy5-A). Fluorescence was recorded using a MACSQuant flow cytometer and data were analysed with MACSQuantify software (Milteyi Biotech). The proper staining procedure of non-viable cells was ensured by assessing heat-treated cells (70°C; 60 min). Initial cell viability was confirmed in each experiment.
Assaying bacterial adhesion to Caco-2 cells
E. faecalis strains were grown aerobically on BHI agar plates for 24 h at 37°C, and L. plantarum NC8 and L. reuteri DSM 20 016 were grown anaerobically on MRS agar plates for 48 h at 30 and 37°C, respectively. Cells were re-suspended in 5 ml PBS, washed, and re-suspended to a final concentration of 1 × 108 CFU/ml, as described above. Concentrations were verified in each experiment by plate counting. Confluent monolayers of Caco-2 cells (passage 12–25) prepared in twenty-four-well tissue culture plates (Nalge Nunc International) were washed with PBS and incubated with antibiotic-free RPMI medium for at least 1 h before infection with 2 × 106 bacteria/well. After 1 h of co-culture, non-adhered bacteria were removed by washing four times with PBS. The Caco-2 cells were lysed in 0·1 % Triton X-100 for 5 min at 37°C, and the adhered bacteria were suspended by pipetting. Adhered bacteria were diluted and plated onto appropriate agar plates by a WASP spiral plater (Don Whitley Scientific) and incubated aerobically at 30 or 37°C before enumeration of CFU on a colony counter (ProtoCOL2; Synbiosis). Triton X-100 treatment did not compromise the ability to form colonies, as tested by plate counting. Adhesion capacities were calculated as (CFU adhered/CFU added) × 100.
Assaying bacterial adhesion to mucin
Microtitre plate wells (Maxisorp Nunc) were coated with mucin (partially purified type III porcine gastric mucin; Sigma Aldrich) as described by Tallon et al. (Reference Tallon, Arias and Bressollier26). Bacterial suspensions were prepared, as described above, and 1 × 106 CFU were added per well. After 1 h incubation at 37°C, unbound bacteria were removed by washing four times with PBS. Adhered bacteria were detached using 25 μl 0·25 % trypsin/well at 37°C for 10 min with slow shaking, and further suspended in 225 μl PBS to enable plating. Determination of the number of adhered bacteria and calculation of adherence capacity were performed as described above.
Generation of monocyte-derived dendritic cells and immunomodulation
Monocytes were separated from buffy coats obtained from healthy volunteers according to institutional guidelines (Ostfold Hospital Trust, Norway). Peripheral blood mononuclear cells were separated by density gradient centrifugation using Lymphoprep medium (specific gravity 1·077 g/ml; Fresenius Kabi). CD14+ cells were selected using human CD14 MicroBeads (MACS Miltenyi Biotech) and seeded in twenty-four-well plates. CD14+ monocytes were differentiated to immature DC using GM-CSF (50 ng/ml) and IL-4 (25 ng/ml) (both from ImmunoTools). Cytokines were replenished at day 4. The immature DC were treated with UV-inactivated bacteria (60 min UV exposure) for 24 h on day 6. Successful inactivation of bacteria was confirmed by plating the final suspension on agar plates. A cocktail of lipopolysaccharide (100 ng/ml; Sigma-Aldrich), TNF-α (15 ng/ml; ImmunoTools) and PGE2 (5 μg/ml; Sigma-Aldrich) was used as a positive control for DC maturation(Reference Landi and Babiuk27). Finally, DC were labelled using phycoerythrin-Cy 5-conjugated mouse anti-human CD83 and Alexa Fluor 700 mouse anti-human CD86 antibodies (MACS Miltenyi Biotech), fluorescence recorded using a MACSQuant flow cytometer and data analysed with MACSQuantify software (Miltenyi Biotech).
Statistical methods
Statistical significance was evaluated using one- or two-way blocked ANOVA models. P values were calculated with t tests with correction for multiple hypothesis testing or Tukey's test by employing the open source statistical language and environment R (www.r-project.org).
Results
Bacterial cultivability and survival in acidic environments
The ability to multiply in acidic environments (pH 6, 5, 4 and 3) was assayed for different E. faecalis strains (Table 1) as an initial screen for acid tolerance. All strains showed a successive decrease in cultivability as the pH was reduced, and none was able to grow at or below pH 4 (data not shown). As this indicates a cut-off value between pH 5 and pH 4, cultivability was next assayed at pH 4·5. Symbioflor-1 was clearly the least acid-tolerant strain when growth at pH 4·5 was compared with growth at neutral pH (Fig. 1(a)). As cell survival after transit through the acidic environment in the stomach is more physiologically relevant than cultivability in acidic environments, we next assayed cell viabilities following incubation at pH 3 for 30 min. Cell viabilities were markedly reduced for all strains, as indicated by a shift from green (SYTO9) towards red (PI) fluorescence (Fig. 1(b)). Untreated cells were stained in each experiment to confirm intact cell membranes, indicating viable cells (data not shown). Impaired viability was most pronounced for Symbioflor-1, while V583 was least affected. Isolates 62, 158B and LMGT3208 showed intermediate tolerance to the treatments (158B and LMGT3208 not shown). These observations were reinforced by fluorescent microscopy imaging, mainly implemented for visual reference (Fig. 1(c)).
Fig. 1 Acid tolerance of Enterococcus faecalis strains. (a) Bacterial growth (optical density (OD) at 600 nm) of Symbioflor-1 (–○–), V583 (–●–), 62 (–Δ–), 158B (–▲–) and LMGT3208 (–□–) in brain–heart infusion (BHI) medium at 37°C with pH 4·5 plotted as percentage of growth at pH 7 against time. Samples were assayed in triplicate and average values plotted after background correction. The data are representative of four different experiments. (b) Flow cytometric analysis of bacterial cultures incubated in BHI medium (pH 3) for 30 min at 37°C subsequently stained with SYTO9 and propidium iodide (PI). A total of 10 000 events were analysed per sample and non-cellular background fluorescence was gated out using the respective side scatter/forward scatter (SSC/FSC) plots (P1). A further gating strategy was used to indicate subpopulations representing dead (P1/P2), sub-lethal (P1/P3) and viable (P1/P4) cells: the percentages of these cells are shown. The dot-plots are representative of at least five experiments. PE, phycoerythrin; FITC-A, fluorescein isothiocyanate-albumin. (c) Fluorescent images were captured of cells treated and stained as described in (b) using a Zeiss LSM 700 confocal microscope equipped with ZEN2010 software.
Bacterial viability after exposure to human gastric and duodenal juices
Bacteria were treated with HGJ (pH 1·5) for 30 min in order to mimic transit through the stomach. This treatment had a detrimental effect on the viability of all strains (Fig. 2(a)). The pH of HGJ was raised to 3·0 (using NaOH) in order to study potential effects of HGJ components other than the extremely low pH. Adjusting the pH to 3·0 enables comparison with the data obtained using media only with pH 3·0 (Fig. 1(b) and (c)), and ensures that digestive enzymes are still active. Viabilities were severely affected after treatment with HGJ (pH 3·0) (Fig. 2(b)), although not to the extent observed after treatment with HGJ with pH 1·5. No strain-specific differences were observed after treatment with either HGJ with pH 1·5 or HGJ with pH 3·0. To mimic transit through the duodenum, bacteria were treated with HDJ for 30 min. In this case, cell viabilities were only affected to a minor extent (Fig. 2(c)). Strain-specific differences were observed, and cells with impaired viability were quantified by gating the relevant subpopulations. Results from three different experiments showed that Symbioflor-1 was the most resistant to HDJ treatment, where only 9·1 % of the cells exhibited impaired viability, while LMGT3208 was the most susceptible strain, with 23·5 % affected.
Fig. 2 Tolerance of Enterococcus faecalis strains to human gastric juice (HGJ) and duodenal juice (HDJ). Bacterial cultures were treated for 30 min at 37°C with (a) HGJ (pH 1·5), (b) HGJ (pH 3) and (c) HDJ (pH 8). All samples were stained with SYTO9 and propidium iodide (PI) and analysed by flow cytometry. A total of 10 000 events were analysed per sample. Density-plots are representative of three independent experiments.
Adhesion capacity to intestinal epithelial cells and mucin
Adhesion to Caco-2 cells was assayed for all the E. faecalis strains (Table 1) and compared with the adhesion of L. reuteri DSM 20 016(Reference Kandler, Stetter and Kohl24) and L. plantarum NC8(Reference Shrago, Chassy and Dobrogosz25), previously reported to bind Caco-2 cells with high and low capacities, respectively(Reference Jensen, Grimmer and Naterstad28). Only 5·1 % of the added Symbioflor-1 cells adhered to IEC, which is significantly less (P < 0·01) than the adhesion capacities of isolate 62 (14·5 %), 158B (12·3 %) and LMGT3208 (10·6 %) (Fig. 3(a)). The adhesion capacity of Symbioflor-1 was comparable with that of L. plantarum NC8 (5·9 %). The same relative species-specific adhesion capacities were found when adhesion to mucin was assessed. Isolate 62, 158B and LMGT3208 bound significantly better to mucin (P < 0·01) than Symbioflor-1. Intermediate and rather poor adhesion capacities were observed for V583 to Caco-2 cells and mucin, respectively. Cells adhered in general better to Caco-2 cells than to mucin.
Fig. 3 Adhesion capacities of Enterococcus faecalis strains. (a) Wells containing monolayers of Caco-2 cells (□) or mucin (▒) were infected with different strains of E. faecalis. After 1 h, non-adhered cells were washed off and adhered bacteria solubilised and enumerated by plate counting. Lactobacillus reuteri DSM 20 016 and L. plantarum NC8 were included as reference strains for high and low binding to Caco-2 cells, respectively. The amount of adhered cells is presented as the percentage of total cells added. All samples were assayed in triplicate and experiments were performed from three to six times. Data are means from three different experiments, with standard deviations represented by vertical bars. (b) Adhesion was assayed with (▒) or without (□) heparin (500 μg/ml) as described in (a).
Binding competition assay using heparin
A competitive-binding assay was employed to investigate the potential role of glycosaminoglycans as host cell receptors, as previously described for E. faecalis (Reference Sava, Zhang and Toma29). Caco-2 cells were pre-incubated with or without heparin (500 μg/ml) (Sigma-Aldrich) for 30 min before infection and binding to Caco-2 cells was assessed for Symbioflor-1, V583 and 62, as described above. A statistically significant reduction in adhesion (P < 0·01) was found in the presence of heparin (Fig. 3(b)). Heparin appeared to have the same effect for all strains.
Ability of different Enterococcus faecalis strains to elicit dendritic cell maturation
The ability of Symbioflor-1, V583 and 62 to mature DC was assayed by monitoring CD83+ and CD86+ cells using flow cytometry. CD83 and CD86 are well-described maturation markers for DC(Reference Evrard, Coudeyras and Dosgilbert7, Reference Zhou and Tedder30–Reference Zhou, Schwarting and Smith32). An increase in CD83+ and CD86+ cells was observed for all strains as compared with the negative control (Fig. 4). However, no strain-specific differences in the ability to mature DC were detected.
Fig. 4 Ability of different Enterococcus faecalis strains to elicit dendritic cell maturation. Immature dendritic cells were treated with UV-inactivated Symbioflor-1 (black), 62 (blue), V583 (light blue), or a cocktail containing lipopolysaccharide–PGE2–TNF-α (green) and compared with untreated cells (red). Expression levels of CD83 and CD86 were analysed using a phycoerythrin (PE)-Cy5-conjugated anti-CD83 antibody and an Alexa Fluor 700-conjugated anti-CD86 antibody by flow cytometry. These results are representative of three different experiments with parallel samples. PI, propidium iodide; APC, allophycocyanin.
Discussion
The object of the present study was to study several characteristics of Symbioflor-1, commonly assayed when screening bacteria for potential probiotic properties, in comparison with other E. faecalis strains (Table 1). Tolerance towards the different environments encountered during GIT transit, adhesion to intestinal cells or mucosa, and the ability to elicit an immune response are likely to be desirable traits(Reference Tuomola, Crittenden and Playne33, Reference Charteris, Kelly and Morelli34). In vitro methods were employed to address these subjects according to the FAO/WHO recommendations(8).
When ingested, probiotics must overcome environmental barriers in the upper GIT in sufficient numbers and arrive in the intestine in a state able to confer beneficial health effects. The physiological fitness of microbes after simulating exposure to environments in the upper GIT is therefore commonly assayed when screening for probiotic properties(Reference Charteris, Kelly and Morelli34–Reference de los Reyes-Gavilán, Suárez and Fernández-García38). The extreme acidity in the stomach (pH 1·5–3·0), in combination with gastric enzymes, is thought to represent a main challenge for survival. Acid tolerance is therefore a highly desirable probiotic trait. It was rather surprising that Symbioflor-1 was most susceptible to acid in comparison with other E. faecalis strains, as this microbe has been reported to confer probiotic properties in vivo (Reference Habermann, Zimmermann and Skarabis15, Reference Habermann, Zimmermann and Skarabis16). Poor acid tolerance was observed for Symbioflor-1, both when assessing cultivability in acidic environments and viability after simulating transit through the stomach using media with low pH.
Treated cells separated into three different subpopulations when assessed using flow cytometry (Fig. 1(b)). These subpopulations represent dead (high PI/low SYTO9), sub-lethal (high PI/high SYTO9) and live (low PI/high SYTO9) cells, in accordance with previous reports(Reference Jaeger, Schulz and Karapetkov39, 40). Such distribution patterns contain valuable information about the physiological fitness of bacterial cells, which is an advantage compared with conventional plating(Reference Jaeger, Schulz and Karapetkov39). Plating only enables the enumeration of cells able to form a colony, and fails to provide any information about metabolically active cells incapable of cellular division (i.e. forming a colony). Such cells are referred to as ‘active but non-culturable’ (ANC) cells(Reference Joux and Lebaron41), and are important populations to describe following injury or stress in different aspects of food microbiology.
Human GIT juice is relatively difficult and costly to obtain. As a result, few studies have employed human juices when assessing GIT transit survival(Reference Del Piano, Strozzi and Barba37, Reference de los Reyes-Gavilán, Suárez and Fernández-García38). Del Piano et al. (Reference Del Piano, Ballare and Anderloni42) found that several probiotic strains were more sensitive to bovine bile, commonly used in artificial solutions, than to human bile. However, it has also been reported that the sensitivity of probiotics to artificial and human pancreatic juice is very comparable(Reference Del Piano, Strozzi and Barba37). We exposed the E. faecalis strains to HGJ and HDJ in order to study strain-specific tolerance. However, the detrimental effects of HGJ treatments made comparison difficult as all cells were detected in the most compromised subpopulation after treatment (Fig. 2(a)). When using HGJ where the pH had been raised to 3, minor improvements of physiological fitness were observed (Fig. 2(b)). Nevertheless, the cell viabilities were still affected to such an extent that strain-specific differences could not be detected using gating strategies on the dot-plots. These results show that both the extremely low pH, but also other components of the HGJ, such as digestive enzymes, are efficient in killing the E. faecalis strains tested in the present study if orally ingested.
Using neat HGJ reflects the gastric environment of a fasting individual more so than in a normal in vivo situation where the gastric ventricle also contains a food matrix. Food and especially milk-based products are known to have a buffering capacity that consequently will protect ingested microbes from the lethal effect of HGJ(Reference Charteris, Kelly and Morelli34, Reference Jaeger, Schulz and Karapetkov39). The loss of viability reported in the present study is therefore expected to be higher than in a normal in vivo situation. Nevertheless, in view of the observed susceptibility to acidic environments, Symbioflor-1 might have a better chance of surviving transit through the stomach if implemented in a milk-based product, encapsulated or somehow protected against this harsh environment(Reference Jaeger, Schulz and Karapetkov39, Reference Sidira, Galanis and Ypsilantis43). Currently Symbioflor-1 is administrated as drops.
Some model systems simulating GIT transit involve the sequential immersion of microbes in gastric and duodenal solutions(Reference Charteris, Kelly and Morelli34–Reference Immerstrand, Paul and Rosenquist36, Reference de los Reyes-Gavilán, Suárez and Fernández-García38, Reference Ritter, Kohler and von Ah44). As the effect of HGJ treatment on the E. faecalis strains in our experiments was so pronounced, no strain-specific differences would have been observed with such a sequential model. We therefore assessed the effects of HGJ and HDJ treatments separately. In contrast to HGJ treatment, all strains survived exposure to HDJ relatively well (Fig. 2(c)). This suggests that transit through the gastric ventricle is the main determining factor for survival in the upper GIT for the strains studied. Strain-specific differences were observed after HDJ treatments, and Symbioflor-1 was identified as the most resistant strain. Bile acids are known as a major stress factor in the duodenal area; however, protecting mechanisms such as the synthesis of stress proteins and swift adaptive abilities have been reported for E. faecalis and might explain the high survival rate following HDJ treatment(Reference Bohle, Faergestad and Veiseth-Kent45–Reference Solheim, Aakra and Vebo47). However, the in vivo significance of this observation must be questioned, as the viability of Symbioflor-1 would already have been severely compromised in the preceding transit through the stomach.
Nueno-Palop & Narbad(Reference Nueno-Palop and Narbad35) included ten E. faecalis strains in a study assessing probiotic properties of bacteria isolated from human faeces. Only one of these E. faecalis strains, CP58, was able to survive a simulated in vitro digestion assay in adequate amounts. This highlights the existence of strain-specific variation in regards to GIT transit tolerance. More than 40 % of E. faecalis CP58 survived the digestion assay, which is considerably higher than the survival of Symbioflor-1 reported in the present paper. However, as milk was included in the media when assessing CP58, the relatively higher survival rate might be attributed to the well-described buffering effect of milk(Reference Charteris, Kelly and Morelli34, Reference Jaeger, Schulz and Karapetkov39).
One may speculate whether the differences in test performance between Symbioflor-1 and the other E. faecalis strains are due to the reported absence of large genomic regions from the chromosome of Symbioflor-1, indicating gene loss(Reference Domann, Hain and Ghai20). Perhaps important determinants of acid tolerance or adhesion, such as proton pumps or surface proteins, have been lost from the genome of Symbioflor-1. However, genes encoding determinants such as aggregation substance, collagen adhesion protein, and the ability to resist oxidative stress were detected(Reference Domann, Hain and Ghai20), implying that Symbioflor-1 is somewhat equipped for exhibiting probiotic traits.
Whether intestinal adhesion is a prerequisite for probiotic cells is debatable. Nevertheless, adhesion will reduce the limiting effects of peristalsis on intestinal residence time, and may block pathogen attachment sites. Adhesion is therefore commonly addressed when screening for probiotic strains in vitro (Reference Nueno-Palop and Narbad35, Reference Jacobsen, Rosenfeldt Nielsen and Hayford48, Reference Li, Yue and Guan49). We investigated the adhesion capacities of the E. faecalis strains to IEC using the well-established Caco-2 cell line(Reference Sambuy, De Angelis and Ranaldi50–Reference Matsumoto, Erickson and Gum52). Culture-related conditions may lead to variations between cell cultures maintained in different laboratories, which makes it difficult to compare results in the literature(Reference Sambuy, De Angelis and Ranaldi50, Reference Natoli, Leoni and D'Agnano53). To ensure that the adhesion data were not biased due to a differentiated cell line, we performed experiments using cells maintained in two different laboratories. The resulting adhesion data correlated well, and were comparable with previous reports(Reference Jensen, Grimmer and Naterstad28, Reference Gaudana, Dhanani and Bagchi54, Reference Laparra and Sanz55). We found that Symbioflor-1 bound no better to IEC than the reference strain included for its low binding capacity (Fig. 3(a)).
The use of several different methods when studying bacterial adhesion to the intestine in vitro has been recommended in order to corroborate observations and perhaps elucidate the type of interactions and molecules that mediate the bacteria–host interaction(Reference Tuomola, Crittenden and Playne33, Reference Laparra and Sanz55). Furthermore, the model using Caco-2 cells has clear limitations, such as the lack of mucus secretion. We therefore expanded the adhesion studies by assessing binding capacities to mucin. Mucins are polymeric glycoproteins found in mucus and have been widely used for assaying intestinal adhesion of bacteria(Reference Tallon, Arias and Bressollier26, Reference Laparra and Sanz55–Reference Styriak, Nemcova and Chang59). The strain-specific adhesion capacities to mucin correlated well with our Caco-2 data and therefore support the observation that Symbioflor-1 has a rather poor adhesion capacity in vitro.
As mentioned above, variations in experimental protocols and in the maintenance of cell lines may cause deviations in adherence capacities for a given strain. Comparisons with other studies should therefore be done with great care. However, the percentage of added bacteria that adhered to the substratum in the present study correlates well with other reports.
In the present study the adhesion to mucin was generally lower than the adhesion to Caco-2 cells (Fig. 3(a)). Reported bacterial adhesion capacities to Caco-2 cells in comparison with mucin have been variable(Reference Tuomola, Crittenden and Playne33, Reference Laparra and Sanz55). Tuomola et al. (Reference Tuomola, Crittenden and Playne33) assayed the adhesion of six different commercial probiotic strains to Caco-2 cells and mucin and found great variability in whether the strains adhered best to cells or mucin. Laparra & Sanz(Reference Laparra and Sanz55) observed better adhesion of probiotics to mucin than to Caco-2 cells. Also, different variants of mucin are employed in these studies, complicating the comparison of results.
A higher affinity for Caco-2 cells, as compared with mucin, made it tempting to speculate that the E. faecalis strains adhere to one or several specific components on the intestinal cell surface. Glycosaminoglycans, ubiquitously expressed on the surface of mammalian cells, represent attachment sites for bacteria, including strains of E. faecalis (Reference Rostand and Esko60–Reference Baldassarri, Bertuccini and Creti62). Sava et al. (Reference Sava, Zhang and Toma29) provided evidence for the involvement of heparin in adhesion to Caco-2 cells for some, but not all, of the E. faecalis strains tested. Heparin has also been shown to block the binding of Escherichia coli O157:H7 to colonic epithelial cells(Reference Gu, Wang and Guo63). We speculated whether the poor adhesion capacities of Symbioflor-1 was a result of this strain being deficient in a putative surface molecule which normally confers binding to host receptors, such as glycosaminoglycans. The fact that an absence of large genomic regions has been reported for Symbioflor-1 in comparison with other E. faecalis strains(Reference Domann, Hain and Ghai20) strengthens this hypothesis. We therefore performed competitive binding assays using heparin in order to investigate such potential molecular mechanisms which might be responsible for the differences in Caco-2 adhesion observed for the different E. faecalis strains studied in the present experiment. Heparin was found to significantly reduce the binding of the strains tested (P < 0·01), which indicates that that glycosaminoglycans might be involved in the bacteria–host interactions. However, no significant differences in the effect of heparin on the strains with (Symbioflor-1) and without (V583 and 62) gene loss were observed (Fig. 3(b)).
DC are antigen-presenting cells with a pivotal role in regulating the immune system at mucosal surfaces(Reference Coombes and Powrie64). Immature DC reside in peripheral tissues, such as the gut mucosa, and continuously sample the microenvironment via pattern recognition receptors (PRR), such as the Toll-like receptors(Reference Rakoff-Nahoum, Paglino and Eslami-Varzaneh65). Specific interactions between bacteria and PRR trigger DC maturation, and, importantly, modulate DC differentiation in such a way that both tolerance towards commensals and generation of protective immune responses against pathogens are enabled(Reference Coombes and Powrie64). Bacteria, including probiotics, differ in their immunomodulatory activity towards DC maturation and may therefore influence the polarisation of immune responses(Reference Christensen, Frokiaer and Pestka66–Reference Hart, Lammers and Brigidi68). We exposed immature DC to different E. faecalis strains to (i) establish whether these bacteria were able to induce DC maturation and (ii) to identify potential strain-specific differences. All strains tested increased the number of CD83+ and CD86+ cells as compared with untreated cells (Fig. 4). No strain-specific differences were observed, which is somewhat surprising considering the highly diverse in vivo effects of the probiotic, pathogenic and commensal strains. Inactivated bacteria are commonly used in similar experiments(Reference Evrard, Coudeyras and Dosgilbert7, Reference Christensen, Frokiaer and Pestka66, Reference Zeuthen, Fink and Frokiaer69), which is probably due to the presumption that bacterial cell-surface molecules are considered the key factors in bacteria–DC communication via the PRR(Reference Lebeer, Vanderleyden and De Keersmaecker5). However, one must not rule out other paths of communication between bacteria and the immune system such as via IEC. Substantial evidence has been provided for differential cross-talk between IEC, DC and bacteria involved in the regulation of intestinal homeostasis(Reference Zoumpopoulou, Tsakalidou and Dewulf67, Reference Rimoldi, Chieppa and Salucci70–Reference Butler, Ng and van Heel72). The possibility of a greater maturation potential by metabolically active bacteria in vivo can therefore not be ruled out.
According to the results presented in the present paper, acid tolerance and/or intestinal adhesion do not appear to be crucial factors involved in the beneficial effects of Symbioflor-1 on host health. This implies that in vitro observations may not always reflect the in vivo situation. In support of this, clinical studies have documented beneficial health effects of the well-studied probiotic strains L. rhamnosus GG and L. plantarum 299v(Reference Nobaek, Johansson and Molin73, Reference Hojsak, Abdovic and Szajewska74). Nevertheless, these strains did not perform well in a recent study using in vitro methods(Reference Jensen, Grimmer and Naterstad28). Vice versa, in vitro studies of L. plantarum MF1298 showed excellent in vitro probiotic properties(Reference Klingberg, Pedersen and Cencic75, Reference Klingberg, Axelsson and Naterstad76), but this bacterium was later reported to exhibit unfavourable effects on symptoms in subjects with irritable bowel syndrome(Reference Ligaarden, Axelsson and Naterstad77). In conclusion, in vitro testing is a rational starting point for selecting microbes with a probiotic potential or to establish possible mechanisms of action, but not adequate to predict the functionality of probiotic micro-organisms in the human body. In line with the recently expressed opinions of Rijkers et al. (Reference Rijkers, de Vos and Brummer78), it must be emphasised that human clinical trials are the definitive tool to establish probiotic status.
Acknowledgements
The present study was supported by The Norwegian University of Life Sciences, Norway and Østfold University College, Norway. T. E. C. was involved in experimental procedures and data analysis of all experiments, and wrote the manuscript. H. J. performed the adhesion experiments to mucin, some statistical analysis and contributed to discussions. C. R. K. contributed to experimental designs of flow cytometric analysis and discussions. G. D. performed statistical analysis. M. J. ensured access to human gastrointestinal juices and contributed to the experimental design of related experiments. T. L. supervised the project. All authors contributed to the critical revision of the manuscript. There are no conflicts of interest to declare.
