Original Article





The aging population has grown rapidly into an aging society, which has led to an increase in diseases, exposure to harmful bacteria and the spread of multidrug- resistant bacteria. Furthermore, in the treatment of chronic hospitalized patients, misuses and abuses of antibiotics have resulted in antibiotic resistance genes of bacteria, which led to the emergence of super-bacteria resistant to most of the antibiotics (1, 2). Moreover, in modern society, where movements of people and commodities have increased due to various transportation technology advancements, super-bacteria are not a problem of a specific region or country, but rather a global issue. Also, recent studies have shown that, excessive or long-term use of antibiotics causes an imbalance in the intestinal microbial environment, in the case of young children, if they continue to take antibiotics at a time when the balance of the intestinal microbiome is changing, adversely affect their health at adults (3).

Probiotics refers to a group of microorganisms which contribute to health promotion by creating a beneficial microbial environment in the human gut, such as Lactobacillus, Bifidobacterium, etc. lactic acid producing bacterial organisms. However, in 1989, Fuller defined probiotics as a beneficial effect on the host by improving the intestinal microbiota, and it was established as a living microorganism (4). Probiotics produce various antimicrobial peptides such as bacteriocin, lactic acids, acetic acids, and other bacterial metabolites during living in intestinal microflora (5, 6). It also inhibits the activity of pathogens in the human body, has anti-inflammatory, antitumor, antibacterial, and antiviral effects, and down-regulates blood cholesterol level (7). Additionally, it is known that probiotics can enhance the ability of macrophages to recognize pathogens, and promote the secretion of immune substances in the intestinal environment, thereby exhibiting immunomodulatory effects (8). Probiotics can also enhance the antibacterial effect and reduce the resistance of antibiotics. It has been reported that the administration of probiotics to premature infants during antibiotic treatment reduced the resistance to antibiotics (9). Furthermore, according to Lesbros-Pantoflickova’s report, simultaneous administration of antibiotics and probiotics to Helicobacter pylori increased the inhibition of their growth, and reduced side effects of antibiotics (10).

However, many studies have only focused on the increase of antibacterial effects of antibiotics even viable lactic acid bacteria (LAB) against H. pylori in the stomach, through simultaneous administration of probiotics and antibiotics. Probiotics studies on increasing the efficacy of antibiotics against multidrug-resistant pathogenic bacteria are not sufficient, due to the fact that live LAB can be inactivated by the antibiotics (11). For this reason, most studies on the antibacterial efficacy of probiotics have been performed using viable LAB. However, LAB frequently has a low probability of reaching and adhering to the intestine through oral administration (12). Nevertheless, the inactivated cells of LAB remain in the digestive system providing beneficial effects to health, and they are characterized by containing antimicrobial active substances such as bacteriocin, large quantity of peptidoglycan, which is a glycoprotein within the cell wall of LAB, lipopolysaccharides (LPS), and organic acids. Also, probiotic stability can be ensured during storage, and the inactivated cells required can be sufficiently supplied in quantity less than that of viable cells (13).

In the intestinal microflora, Bifidobacteria is a gram-positive anaerobic bacterium, which predominates during the neonatal period, and gradually becomes established as the main bacterial species at early ages. The number of Bifidobacteria is further reduced with changing the intestinal microflora by getting older. A probiotic Bifidobacteria can create a healthy intestinal acidic environment leading to the construction of a low level of pathogenic bacteria (14). With actively utilize the physiological effects of Bifidobacteria, it may prevent or improve intestinal tract infections. For chronic patients who must be administered antibiotics for long periods of time, imbalance in the normal intestinal microbiome may be caused by antibiotics that were administered for therapeutic purposes, leading to intestinal diseases such as indigestion. It has been reported that a combined administration of antibiotics, and probiotic Bifidobacteria as a potential immune-adjuvant is advisable in such subjects (15).

With the goal of developing probiotics that possess these functions, the present report has been carried out in order to evaluate whether sonicated Bifidobacteria metabolites or viable cells are effective. The antibacterial activity of Bifidobacteria, as probiotics, was compared with eight strains of the viable and sonicated-inactivated cell, while verifying antimicrobial activity of Bifidobacterium spp. against multidrug-resistant pathogenic bacteria. Subsequently, a disc diffusion assay was conducted in an experiment to establish whether four strains of the viable and inactivated probiotic cell component could inhibit pathogenic bacteria growth.


Bacterial strains and culture

In this experiment, three pathogenic bacteria species were tested, including Gram-positive bacteria Staphylococcus aureus (S. aureus) ATCC 25923, Gram-negative bacteria Pseudomonas aeruginosa (P. aeruginosa) ATCC 27853, and Eenterococcus faecalis (E. faecalis) ATCC 29212. The isolates were provided by Sahmyook medical center and stored at -70°C in nutrient broth (BD Difco, Detroit, MI, USA) with 20% glycerol before testing. Cultures of pathogenic bacteria were grown in Brain Heart Infusion (BHI) broth medium (BD Difco) at 37°C to achieve a concentration of 108~109 the colony forming unit (CFU)/mL.

Preparation of Bifidobacteria supernatant and inactivated Bifidobacteria samples

All Bifidobacterium strains were obtained from Korean Collection for Type Cultures (KCTC). Bifidobacterium strains were cultured in Lactobacilli MRS (Man Rogosa Sharpe) broth (BD Difco) with 0.05% (w/v) of L-cysteine in an anaerobic incubator (CO2 5%, H2 5%, N2 90%) at 37°C for 48 hrs (Table 1). After incubation, Bifidobacteria were centrifuged at 4,000 rpm for 10 min. The bacterial-free supernatant was then filtered through a sterilized 0.22 μm pore size low binding cellulose acetate filters (Millipore, Billerica, MA, USA). Homogenate inactivated cells are obtained by mechanical crushing of cells, which also exhibits the same effect as probiotics without the cellular denaturation by heat-killing (16). The bacterial-free supernatant was separated by centrifugation, and the pellets were sonicated by ultrasonic waves to make a pulverized solution and employed in the experiment. To produce sonicated-inactivated Bifidobacteria, the pellets were washed twice with phosphate-buffered saline (PBS) and suspended in the same buffer. Bacterial suspensions were adjusted to a final concentration of 1.0×109 CFU/mL before sonication for 6 min (amplitude 100%, pulse on 60s, and pulse off 60s) with a sonicator (VCX-130, Sonics & materials, USA). Sonicated-Bifidobacteria were centrifuged at 8000 rpm for 10 min, and filtered using a 0.22 μm syringe cellulose filter.

Table 1.

List of probiotic Bifidobacterium strains from KCTC

Probiotic strains KCTC number ATCC number Source
Bifidobacterium lactis KCTC 5854 - Fermented milk
Bifidobacterium bifidum KCTC 3202 ATCC29521 Infant
Bifidobacterium breve KCTC 3220 ATCC15700 Infant
Bifidobacterium catenulatum KCTC 3221 ATCC27539 Adult
Bifidobacterium dentium KCTC 3222 ATCC27534 Adult
Bifidobacterium longum KCTC 3128 ATCC15707 Adult
Bifidobacterium infantis KCTC 3249 ATCC15697 Infant
Bifidobacterium pseudocatenulatum KCTC 3223 ATCC27919 Infant

Growth inhibition assay of Bifidobacteria

The antimicrobial activity of the Bifidobacterium isolates against E. faecalis, P. aeruginosa, and S. aureus was determined by the agar dilution method based on the guidelines of the Committee for Clinical Laboratory Standards (CCLS) (17). All pathogenic strains were diluted to a concentration of 10 CFU/mL and cultured for 24 hrs. at 37°C in BHI broth, containing 25% (v/v) or Bifidobacteria supernatants. Percent of growth inhibition was detected by measuring the absorbance of the mixtures at 630 nm using a microplate reader. As a control, E. faecalis, P. aeruginosa, and S. aureus were cultured in BHI broth with the same quantity of sterile distilled water. The growth inhibitory effect of the Bifidobacteria supernatant and sonicated Bifidobacteria were calculated based on the turbidity measured by optical density.

Minimum inhibitory concentrations test by the medium dilution method

The minimum inhibitory concentration was measured with four antibiotics. Antibiotics utilized in the experiment were gentamicin (GEN), ciprofloxacin (CIP), erythromycin (ERY), and tetracycline (TET) (TCI, Tokyo, Japan). The concentration of each antibiotics was established by the serial dilution method, and each antibiotics was added to Mueller-Hinton broth (Difco). The test strains were transplanted in Mueller-Hinton broth and cultured in an incubator at 37°C for 24 hrs. The number of cells were counted per 0.5 McFarland standard, then adjusted to a final bacterial concentration of 1×104 CFU/mL for use as bacterial solutions for the MIC test. 50 µl of each of the prepared bacterial solutions was inoculated on a medium containing each antibiotic and incubated at 37°C for 48 hrs. Turbidity of the test broth was measured in terms of optical density at various dilutions. When the optical density values for each dilution of the LAB test broth and the pure bacterial culture medium were nearly identical, the minimum concentration of theLAB test broth was performed as the MIC.

Antibacterial assay by agar well diffusion method

Antibacterial diffusion assay of the CCLS was performed to determine the level of antibacterial activities against the screened pathogens on supernatant. Four supernatants, selected based on growth inhibitory effect results, were added to BHI agar medium to a 10% (v/v) level. Pathogenic bacterial strains were separated on solid agar medium (concentration of 108~109 CFU/mL) with an antibiotic disc, and cultured in a 37°C incubator for 24 hrs. Four different types of antibiotic discs utilized in the experiment were gentamicin, ciprofloxacin, erythromycin, and tetracycline. As a control, pathogenic bacteria strains were suspended on BHI agar medium incubated in a 37°C incubator for 24 hrs. The diameter of each clear zone after incubation was measured by calipers in millimeters.

Statistical analysis

Values were expressed as mean ± standard deviation (SD). For statistical evaluation of data, one-way ANOVA tests were applied, with SPSS statistical program (Windows version 25.0, IBM, Chicago, IL). Differences were assessed significant at P < 0.05 for all comparisons by Tukey test.


Growth inhibitory effect of Bifidobacterium spp.

To investigate the antibacterial effect of eight strains of the Bifidobacterium supernatant and the sonicated-inactivated Bifidobacteria, a concentration of 25% (v/v) was applied through the concentration gradient screening. The supernatants of four out of eight strains showed antimicrobial activity against S. aureus (B. dentium, B. longum, B. infantis, and B. pseudocatenulatum). Among them, the inhibition percentage of the B. bifidum supernatant was the lowest (22.28 ± 0.96%; Fig. 1C). The supernatants of the four strains above also exhibited antibacterial efficacy against P. aeruginosa and E. faecalis. The inhibition percentage against P. aeruginosa and E. faecalis was the lowest in B. breve (15.90 ± 2.17%, 6.32 ± 5.09; Fig. 1B, 1A), respectively. On the other hand, the antibacterial efficacy of the inactivated Bifidobacteria did not exhibit any significant difference from that of the control (Table 2). Among the eight strains of the inactivated-sonicated Bifidobacteria, B. lactis showed the antibacterial activity by moderate inhibition of the growth of three pathogenic bacteria. B.bifidum and B. dentium showed moderate growth inhibition with 34.78% and 39.90% inhibition results against P. aeruginosa, while B. bifidum showed 11.45% growth inhibition against S. aureus. However, B. infantis showed very low activity of less than 5%, and was not contained (Table 2). In summary, four types of Bifidobacteria supernatants exhibited antibacterial activity against pathogenic bacteria, whereas the inactivated Bifidobacteria showed comparatively low levels of antibacterial activity. B. lactis is not a human-derived strain, so it cannot be clarified whether it is an effective strain for human. Therefore, we employed the four types of Bifidobacterium supernatants in the agar well diffusion methods.

Fig. 1

Fig. 1. Growth Inhibitory effect with cultured eight strains of Bifidobacteria supernatants. All bacteria were treated with 25% (v/v) Bifidobacteria supernatants for 24 h. % of inhibition was determined by Growth Inhibition assay. The value represents the mean ± S.D. * p < 0.05. Con, control; ani, B. lactis; bif, B. bifidum; bre, B. breve; cat, B. catenulatum; den, B. dentium; lon, B. longum; inf, B. infantis; psc, B. pseudocatenulatum.

Table 2.

Growth inhibitory effect (%) of E. faecalis, P. aeruginosa, and S. aureus cultured with eight strains of inactivated Bifidobacteria. All LAB were treated with 25% (v/v) inactivated Bifidobacteria for 24 hrs. The value represents the mean ± S.D.

Bifidobacterium strains Pathogenic species
E. faecalis P. aeruginosa S. aureus
B. lactis KCTC 5854 13.01 ± 0.95 23.10 ± 1.26 10.89 ± 0.62
B. bifidum KCTC 3202 5.11 ± 0.24 39.90 ± 0.86 11.45 ± 0.25
B. breve KCTC 3220 6.38 ± 0.12 4.76 ± 0.25 7.99 ± 0.23
B. catenulatum KCTC 3221 3.52 ± 0.10 20.88 ± 0.77 9.67 ± 0.22
B. dentium KCTC 3222 0.21 ± 0.02 34.78 ± 0.79 6.10 ± 0.19
B. longum KCTC 3128 1.29 ± 0.17 25.54 ± 0.69 7.16 ± 0.21
B. infantis KCTC 3249 2.06 ± 0.18 2.31 ± 0.12 4.14 ± 0.13
B. pseudocatenulatum KCTC 3223 7.08 ± 0.22 4.58 ± 0.13 1.69 ± 0.09

As shown in Fig. 2, media containing Bifidobacterium supernatants have been shown to inhibit the growth activity of pathogenic bacteria compared to the control group. For the four antibiotics, such as GEN, CIP, ERY, and TET, pathogenic P. aeruginosa, E. faecalis and S. aureus showed high antibiotic resistant, expectably. All eight types of growth media with Bifidobacterium supernatant showed an inhibitory effect, and four strains out of eight (B. longum, B. pseudocatenulatum, B. dentium, and B. infantis) demonstrated remarkable effect in all three species of pathogenic bacteria. B. bifidum and B. breve had a lower inhibitory effect than other Bifidobacterium supernatants (Fig. 1). MIC values of the four types of antibiotics againstpathogenic P. aeruginosa, E. faecalis, S. aureus and Bifidobacterium spp.showed difference. However, statistical significance reliability was shown to be very low. (Table 3). To investigate specific differences, it will be need to identify by comparing the components of supernatant through subsequent experiments.

Fig. 2

Antibacterial activity of Bifidobacterium spp. apply for through the growth inhibitory effect with cultured eight strains of Bifidobacteria supernatants. ctrl, control; ani, B. lactis; bif, B. bifidum; bre, B. breve; cat, B. catenulatum; den, B. dentium; lon, B. longum; inf, B. infantis; psc, B. pseudocatenulatum.

Table 3.

MIC values of the four types of antibiotics against pathogenic P. aeruginosa, E. faecalis, S. aureus and Bifidobacterium spp.

MIC (μg/mL)
B. lactis 4 0.5 12.5 8
B. bifidum 6.25 0.25 12.5 2
B. breve 6.25 0.125 25 1
B. catenulatum 6.25 0.5 32 0.5
B. dentium 0.75 0.25 12.5 0.5
B. longum 6.25 0.125 3.12 1
B. infantis 2 0.125 25 2
B. pseudocatenulatum 2 0.25 3.12 2
E. faecalis ATCC 29212 64 >128 >128 >128
P. aeruginosa ATCC 27853 >100 >128 64 >128
S. aureus ATCC 25923 64 >128 >128 64

TET, tetracycline; GEN, gentamicin; ERY, erythromycin; CIP, ciprofloxacin

Antibacterial synergism of Bifidobacterium supernatant and antibiotics

Antibacterial disc diffusion assays were performed by adding 10% (v/v) of four kinds of Bifidobacterium supernatants to BHI agar medium. Against S. aureus, the antibiotic susceptibilities of TET and CIP were significantly increased by each of the four supernatants; moreover, resistance to GEN and ERY also increased. The B. longum supernatant showed TET, as Tetracycline family antibiotics, disc clear zone diameter of 36.48 ± 0.50 mm, which was 1.5 times that of the control. The inhibitory diameter of the CIP, as Fluoroquinolone family antibiotics, disc clear zone was 29.27 ± 0.98 mm when applying the supernatant of B. infantis, and the antibacterial activity increased to 1.1-fold higher than the control (Table 4A). In the antibiotic susceptibility of P. aeruginosa, TET and ERY increased in all four Bifidobacterium species. The B. pseudocatenulatum supernatant medium produced TET disc clear zone of 36.85 ± 0.68 mm, which was 1.5 times that of the control. The B. dentium supernatant produced ERY, as a Macrolide family antibiotics, disc clear zone of 31.10 ± 0.51 mm. The B. infantis supernatant was higher than the control group only in P. aeruginosa, and tends to be similar or decreased in other pathogenic bacteria (Table 4B). The results ofthe E. faecalis exhibited resistance to most of the antibiotics, and all three growth inhibition except that for GEN, as Aminoglycoside family antibiotics, were increased. In the B. dentium supernatant medium the diameter of the CIP disc clear zone was 28.44 ± 0.77 mm, reflecting a 1.5-fold increase in antimicrobial activity compared to the control (Table 4C).

Table 4.

Antimicrobial activity results of Bifidobacteria supernatant by disc diffusion method

A. Growth inhibition of S. aureus ATCC 25923
Bifidobacterium strains TET TGEN TERY TCIP
Inhibition zone diameter (ø, mm)
control 24.39 ± 0.91 24.08 ± 0.97 29.55 ± 0.26 26.49 ± 0.93
B. dentium 32.72 ± 0.75 21.08 ± 0.60 25.37 ± 0.81 28.21 ± 0.88
B. longum 36.48 ± 0.50 21.85 ± 0.43 26.14 ± 0.31 28.29 ± 0.38
B. infantis 32.89 ± 0.52 20.91 ± 0.57 25.75 ± 0.48 29.27 ± 0.98
B. pseudocatenulatum 35.02 ± 0.88 21.47 ± 0.68 27.34 ± 0.55 26.78 ± 0.86
B. Growth inhibition of P. aeruginosa ATCC 27853
Bifidobacterium strains TET GEN ERY CIP
Inhibition zone diameter (ø, mm)
control 24.96 ± 0.90 24.59 ± 1.02 26.72 ± 0.82 26.25 ± 0.44
B. dentium 30.57 ± 0.48 20.18 ± 0.57 31.10 ± 0.51 24.25 ± 1.03
B. longum 33.83 ± 0.57 18.05 ± 0.33 21.73 ± 0.75 24.20 ± 0.64
B. infantis 31.80 ± 0.49 17.61 ± 0.50 27.43 ± 1.03 20.91 ± 0.86
B. pseudocatenulatum 36.85 ± 0.68 20.30 ± 0.57 27.80 ± 0.23 28.19 ± 0.58
C. Growth inhibition of E. faecalis ATCC 29212
Bifidobacterium strains TET GEN ERY CIP
Inhibition zone diameter (ø, mm)
control 13.06 ± 0.43 8.44 ± 0.42 19.65 ± 0.23 18.48 ± 0.34
B. dentium 19.43 ± 0.76 7.63 ± 0.28 26.83 ± 0.97 28.44 ± 0.77
B. longum 20.74 ± 0.81 10.01 ± 0.54 19.45 ± 0.11 23.43 ± 0.72
B. infantis 16.80 ± 0.75 8.29 ± 0.34 20.63 ± 0.96 28.07 ± 0.96
B. pseudocatenulatum 17.09 ± 0.96 8.16 ± 0.45 20.59 ± 0.73 27.64 ± 0.85

The value represents the mean ± S.D. TET, tetracycline; GEN, gentamicin; ERY, erythromycin; CIP, ciprofloxacin.

As shown in Fig. 3, it was confirmed that the inhibitory zone diameter of the antibiotics increased in the media containing Bifidobacterium supernatant by agar well diffusion method. In some Bifidobacterium supernatants, which showed a significant growth inhibitory effect of pathogenic bacteria in concentration gradient previous experiments, the measurement of inhibitory zone diameter was rather reduced. Unlike previous experimental results, in E. faecalis, the measurement of the inhibitory zone of B. longum was large, in P. aeruginosa was observed to have an increase the measurement of inhibitory zone of B. pseudocatenulatum in S. aureus, the measurement of B. dentium was the most significantly increased in the inhibitory zone diameter included in the media containing Bifidobacterium supernatant (Fig. 3).

Fig. 3

In vitro antibacterial synergism of Bifidobacterium supernatant and antibiotics by agar well diffusion method. A, S. aureus; B, P. aeruginosa; C, E. faecalis; a, CIP; b, GEN; c, ERY; d, TET.


The use of various antibiotics for the treat of complex degenerative disease speed up recovery in hospitals, but community associated infections have increased significantly, with the spread of antibiotic-resistant bacteria at greater spread and diversity. Novel solutions are desperately required, as the effective antibiotics are limited (18). Several studies have shown that probiotics can inhibit the growth of methicillin-resistant S. aureus and P. aeruginosa(19, 20). AL-Saadi reported that B. breve had antagonistic activity against methicillin-resistant S. aureus (MRSA) (21). Also, Lee reported that Bifidobacterium strain could have a potential application for alternative therapy in P. aeruginosa and Acinetobacter baumannii (22). Therefore, the attempt of this investigation was to ascertain whether the combined administration of LAB may enhance the antibacterial effect of antibiotics.

There are various mechanisms conjectured that could be responsible for the probiotic effect, even though the definition of probiotics includes that the probiotic bacteria must be viable, and administered in enough quantity to produce a health effect in human. As one of them, not only with viable cells but some other with bacterial metabolites or inactivated components could be involve. The physiological adhesion activity of inactivated cells increases in the intestine epithelial cell, and are induced by direct contact with immune cells. If the demonstrated effect examined, the components of the inactivated cells of probiotic LAB differ from one strain to another. The microbial component exhibits immunomodulatory activity by selectively passing through a binding that recognizes toll like receptors through microfold (M) cells in the intestinal epithelial mucus membrane such as Peyer’s patches. Even before passing through to the M cell, it also contacts the intestinal immune cells through dendritic cells (23). The inactivated microbial component passing through M cells activates macrophages to express cytokines, and stimulates immune responses. Since antibiotics have been in use for a long history, pathogens are less susceptible to antibiotics and bacterial resistance to antibiotics proliferate more strongly and selectively, leading to a phenomenon of microbial shift (24). It is a different way from that of living cells producing organic acid, and secreting bacteriocin to show antibacterial activity. However, heat-killed cells also do not induce direct cytotoxicity, and have similar effects to live cells. They inhibit the proliferation of pathogenic bacteria by inducing phagocytosis or inflammatory cytokines of immune system (25, 26). Additionally, it forms a conjugate with pathogenic bacteria to help discharge it out of the digestive system.

Based on these theories, Bifidobacterium supernatants and sonicated-inactivated Bifidobacteria, were administered to compare their antibacterial effects in the present report. Supernatants produced notable antibacterial effects, but the inactivated Bifidobacteria were not effective. It is presumed that this lower antibacterial effect was due to sonication-induced decomposition of antibacterial metabolites. Consequently, among the eight strains of probiotic supernatants, four strains that displayed the highest antibacterial activity levels were selected, and disc diffusion assays were performed to clarify whether antibiotic susceptibility increased when the probiotic supernatants and antibiotics were administered simultaneously. As expected, the antibacterial efficacy of most the observed antibiotics have increased. The susceptibility of pathogenic bacteria to TET was increased in all Bifidobacteria supernatant-added media. Moreover, some Bifidobacterium supernatants such as B. longum and B. pseudocatenulatum, showed synergism with the antibacterial activity of antibiotics. Therefore, further research and clinical studies are required on the interactions that occur when various specific strains of Bifidobacterium spp. are combined administer with antibiotics.

Through a summary of the experimental results, we believe that when Bifidobacterium strains are administered with antibiotics, the antimicrobial effect may increase, allowing reductions of the treatment duration or dosage, and therefore reducing the potential for overuse of antibiotics. Consequently, it may result in suppressing the emergence of multidrug- resistant bacteria due to the use of antibiotics, which is perceived as a need to be combined with probiotics. We anticipate the possibility of clinical use of inactivated probiotics with specific strains as a combined administration of antibiotics or immune adjuvants through continuous following research on mechanisms of synergistic antibiotic effects.


The present study was supported by the Duksung Women’s University research grants of 2019.



Gould K. Antibiotics: From prehistory to the present day. J Antimicrob Chemother 2016;71:572-5.


Kraemer SA, Ramachandran A, Perron GG. Antibiotic pollution in the environment: From microbial ecology to public policy. Microorganisms 2019;7:180.


Blaser MJ. Antibiotic use and its consequences for the normal microbiome. Science 2016;352:544-5.


Fuller R. Probiotics in man and animals. J Appl Bacteriol 1989;66:365-78.


Anukam KC, Reid G, ARM C. Probiotics: 100 years (1997-2007) after Elie Metchnikoff's observation. Communicating current research and educational topics and trends in applied microbiology 2007;1:466-74.


Mastromarino P, Cacciotti F, Masci A, Mosca L. Antiviral activity of Lactobacillus brevis towards herpes simplex virus type 2: Role of cell wall associated components. Anaerobe 2011;17:334-6.


Shadnoush M, Shaker HR, Mehrabi Y, Delpisheh A, Alipoor E, Faghfoori Z, et al. Probiotic yogurt affects pro- and anti-inflammatory factors in patients with inflammatory bowel disease. Iran J Pharm Res 2013;12:929-36.


Isolauri E, Kirfavainen PV, Salminen S. Probiotics a role in the treatment of intestinal infection and inflammation? Gut 2002;50:54-9.


Esaiassen E, Hjerde E, Cavanagh JP, Pedersen T, Andresen JH, Rettedal SI, et al. Effects of probiotic supplementation on the gut microbiota and antibiotic resistome development in preterm infants. Front Pediatr 2018;6:347.


Lesbros-Pantoflickova D, Corthésy-Theulaz I, Blum AL. Helicobacter pylori and probiotics. J Nutr 2007;137:812S-8S.


Sawada D, Sugawara T, Ishida Y, Aihara K, Aoki Y, Fujiwara S, et al. Effect of continuous ingestion of a beverage prepared with lactobacillus gasseri cp2305 inactivated by heat treatment on the regulation of intestinal function. Food Res Int 2016;79:33-9.


Cuevas-González PF. Liceaga AM, Aguilar-Toalá J. Postbiotics and paraprobiotics: From concepts to applications. Food Res Int 2020;136:109502.


Adams CA. The probiotic paradox: live and dead cells are biological response modifiers. Nutr Res Rev 2010;23:37-46.


Khokhlova EV, Smeianov VV, Efimov BA, Kafarskaia LI, Pavlova SI, Shkoporov AN. Anti-inflammatory properties of intestinal Bifidobacterium strains isolated from healthy infants. Microbiol Immunol 2012;56:27-39.


Yang J, Yang H. Effect of Bifidobacterium breve in combination with different antibiotics on Clostridium difficile. Front Microbiol 2018;9:2953.


Pessi T, Sütas Y, Saxelin M, Kallioinen H, Isolauri E. Antiproliferative effects of homogenates derived from five strains of candidate probiotic bacteria. Appl Environ Microbiol 1999;65:4725-8.


CLSI. Performance standards for antimicrobial susceptibility testing; twenty-eighth informational supplement. CLSI document M100-S28. Wayne, PA: Clinical and Laboratory Standards Institute, 2018.


Ventola CL. The antibiotic resistance crisis: Part 2: management strategies and new agents. PT 2015;40:344-52.


Karska-Wysocki B, Bazo M, Smoragiewicz W. Antibacterial activity of Lactobacillus acidophilus and Lactobacillus casei against methicillin-resistant Staphylococcus aureus (MRSA). Microbiol Res 2010;165:674-86.


Layus BI, Gerez CL, Rodriguez AV. Antibacterial activity of Lactobacillus plantarum CRL759 against methicillin-resistant Staphylococcus aureus and Pseudomonas aeruginosa. Arab J Sci Eng 2020;45:4503-10.


AL-Saadi ZN. In vitro antagonistic activity of Bifidobacterium breve isolated from breast-fed infants human gastrointestinal microflora against two clinical strains of Staphylococcus aureus (MRSA and MSSA). J Advances in Biology & Biotechnology 2016;10:1-9.


Lee DK, Kim MJ, Kang JY, Park JE, Shin HS, Ha NJ, et al. Probiotic with antimicrobial activity against multidrug resistant Pseudomonas aeruginosa and Acinetobacter baumannii. KJ Microbiology 2013;49:245-52.


Corr SC, Gahan CC, Hill C. M-cells: origin, morphology and role in mucosal immunity and microbial pathogenesis. FEMS Immunol Med Microbiol 2008;52:2-12.


Zaura E, Brandt BW, Teixeira de Mattos MJ, Buijs MJ, Caspers MP, Rashid MU, et al. Same exposure but two radically different responses to antibiotics: resilience of the salivary microbiome versus long-term microbial shifts in feces. mBio 2015;6:e01693-15.


Jorjão AL, de Oliveira FE, Leão MV, Carvalho CA, Jorge AO, de Oliveira LD. Live and heat-killed Lactobacillus rhamnosus ATCC 7469 may induce modulatory cytokines profiles on macrophages RAW 264.7. Scientific World Journal 2015;2015:716749.


Geraldo BMC, Batalha MN, Milhan NVM, Rossoni RD, Scorzoni L, Anbinder AL. Heat-killed Lactobacillus reuteri and cell-free culture supernatant have similar effects to viable probiotics during interaction with Porphyromonas gingivalis. J Periodontal Res 2020;55:215-20.

페이지 상단으로 이동하기