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Article

Protective Effects and Mechanism of a Novel Probiotic Strain Ligilactobacillus salivarius YL20 against Cronobacter sakazakii-Induced Necrotizing Enterocolitis In Vitro and In Vivo

by
Weiming Wang
1,*,†,
Meng Geng
2,3,†,
Caixia Zhu
2,3,†,
Lei Huang
2,3,
Yue Zhang
2,3,
Tengxun Zhang
2,3,
Chongjie Zhao
2,3,
Tongcun Zhang
2,3,
Xinjun Du
4 and
Nan Wang
2,3,*
1
School of Traditional Chinese Medicine, Southern Medical University, Guangzhou 510515, China
2
Key Laboratory of Industrial Fermentation Microbiology, Ministry of Education and Tianjin, College of Biotechnology, Tianjin University of Science and Technology, Tianjin 300457, China
3
Tianjin Engineering Research Center of Microbial Metabolism and Fermentation Process Control, Tianjin 300457, China
4
College of Biotechnology, Tianjin University of Science and Technology, Tianjin 300457, China
*
Authors to whom correspondence should be addressed.
†
These authors contributed equally to this work.
Nutrients 2022, 14(18), 3827; https://doi.org/10.3390/nu14183827
Submission received: 29 July 2022 / Revised: 13 September 2022 / Accepted: 13 September 2022 / Published: 16 September 2022
(This article belongs to the Section Prebiotics and Probiotics)
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Versions Notes

Abstract

:
Exposure to probiotics in early life contributes to host intestinal development and prevention of necrotizing enterocolitis (NEC). Cronobacter sakazakii (C. sakazakii), an opportunistic pathogen, can cause NEC, bacteremia, and meningitis in neonates, but the research of probiotics against C. sakazakii is limited relative to other enteropathogens. Here, the protective effect and mechanism of a novel probiotic Ligilactobacillus salivarius (L. salivarius) YL20 isolated from breast milk on C. sakazakii-induced intestinal injury were explored by using two in vitro models, including an C. sakazakii-infected intestinal organoid model and intestinal barrier model, as well as an in vivo experimental animal model. Our results revealed that L. salivarius YL20 could promote epithelial cell proliferation in intestinal organoids, rescue budding-impaired organoids, prevent the decrease of mRNA levels of leucine-rich repeat containing G protein-coupled receptor 5 (Lgr5), zonula occludens-1 (Zo-1) and Occludin, and reverse C. sakazakii-induced low level of Mucin 2 (MUC2) in intestinal organoids. Additionally, YL20 could inhibit C. sakazakii invasion, increase the expression of ZO-1 and occludin in C. sakazakii-infected HT-29 cells, and reverse TEER decrease and corresponding permeability increase across C. sakazakii-infected Caco-2 monolayers. Furthermore, YL20 administration could alleviate NEC in C. sakazakii-infected neonatal mice by increasing the mice survival ratio, decreasing pathology scores, and downregulating pro-inflammatory cytokines. Meanwhile, YL20 could also enhance intestinal barrier function in vivo by increasing the number of goblet cells, the level of MUC-2 and the expression of ZO-1. Our overall findings demonstrated for the first time the beneficial effects of L. salivarius YL20 against C. sakazakii-induced NEC by improving intestinal stem cell function and enhancing intestinal barrier integrity.

1. Introduction

Necrotizing enterocolitis (NEC), one of the most devastating gastrointestinal diseases with high morbidity and mortality, mainly occurs in newborn premature infants and exhibits an incidence of 15~20% in premature infants with a weight <1000 g [1,2], an average mortality of 15–30%, and even as high as 75–85% in its most severe forms [3,4]. The exact pathogenesis of NEC has been an area of intense investigation, and several risk factors, including prematurity, formula feeding, and the presence of pathogens, may cause NEC by stimulating intestinal inflammatory response, destroying enteric mucosal integrity, and inducing intestinal epithelial necrosis [5,6]. Notably, Cronobacter sakazakii (C. sakazakii), one of opportunistic pathogens, is implicated in severe outbreaks of NEC in premature and full-term infants, suggesting its potential important role in the pathogenesis of NEC [7]. C. sakazakii is a Gram-negative, facultative anaerobic, peritrichously flagellated, rod-shaped, and non-spore-forming pathogen in the Enterobacteriaceae family. It is mainly present in many low moisture foods like infant formula, and also in hospitals, homes, and equipment such as enteral feeding tubes and baby bottles. C. sakazakii can cause severe NEC, neonatal meningitis, and bacteremia, with mortality rates ranging from 40% to 80% for premature (<37 weeks of gestational age) and/or low-birth weight infants (<2500 g) [8,9]. Despite clinical recovery with antibiotics, the survivors of C. sakazakii infection are often accompanied by chronic sequelae, such as neurological impairment and developmental disorders [10].
Currently, probiotics have received significant attention due to their potential in the prevention and treatment of NEC [11]. Administering probiotics at the early stage can effectively improve intestinal health, promote intestinal development, and relieve intestinal damage by promoting intestinal motility and absorption, enhancing intestinal barrier integrity, stimulating immune system maturation, and balancing intestinal microbiota. Probiotics may resist pathogens through direct antagonism (competition for nutrition or epithelial adhesion sites), or indirect antagonism (release of metabolites such as organic acids, etc.). Clinical studies have confirmed the beneficial effects of probiotics including Bifidobacterium longum subsp. infantis (previously known as Bifidobacteria infantis) (B. infantis) and Lactobacillus acidophilus on NEC [12,13]. Several probiotic strains, including Bacteroides fragilis ZY-312 [5] and Lactococcus lactis [14], have also been reported to protect against C. sakazakii-induced intestinal inflammation in two different models, a neonatal rat model and a preterm rabbit model. A conditioned medium from B. infantis was found to be able to prevent C. sakazakii-induced NEC in newborn mice [15]. However, the research of probiotics against C. sakazakii is limited relative to other enteropathogens.
Infectious intestinal pathogens, including C. sakazakii, induced NEC through adhering to intestinal epithelial cells and damaging the intestinal barrier. Intestinal stem cell (ISC)-driven renewal of epithelial cells in crypts help maintain the intestinal barrier integrity against pathogen invasion, repair the damaged site, and prevent intestinal inflammation [16]. Studies on germ-free animals have shown that colonized intestinal microorganisms can influence early intestinal morphological development, intestinal epithelial cell proliferation and differentiation [17]. Intestinal organoids containing ISCs can generate all the differentiated lineages, including absorptive cells, goblet cells, enteroendocrine cells, paneth cells, etc., indicating that the intestinal organoid is an excellent model in studying host–microbial interactions in vitro [18]. Ligilactobacillus (formerly known as Lactobacillus) salivarius (L. salivarius) is generally considered as a beneficial probiotic and widely used in dairy foods and nutritional supplements. However, whether L. salivarius can inhibit C. sakazakii-induced NEC has been unknown.
To explore the protective effects and related mechanisms of our newly identified probiotic strain (L. salivarius YL20) on C. sakazakii-induced NEC, we first compared the stimulatory effects on intestinal epithelial development using the in vitro model of intestinal organoids and antagonistic activity against C. sakazakii between L. salivarius YL20 and other probiotic strains (Lactobacillus gasseri GM20, Lacticaseibacillus rhamnosus SW01, Lacticaseibacillus rhamnosus GG (LGG), etc.). The beneficial effects of L. salivarius YL20 on C. sakazakii-infected intestinal epithelial proliferation and repair were further investigated by using a caco-2 monolayer model and an experimental mice model. Our results suggest that L. salivarius YL20 could protect against C. sakazakii-induced intestinal inflammation by improving intestinal stem cell function and enhancing intestinal barrier.

2. Materials and Methods

2.1. Bacterial Strains and Cell Culture

L. salivarius YL20 isolated from the breast milk of healthy mothers was confirmed by 16S RNA sequencing (GenBank: MT597593.1). C. sakazakii strain (ATCC No. 51329) was grown in lysogeny broth (LB) medium and all lactobacillus strains (Lacticaseibacillus salivarius YL20, Lactobacillus gasseri GM20, Lacticaseibacillus rhamnosus SW01, Lacticaseibacillus paracasei TX01, Lactobacillus delbrueckii Y2 and Streptococcus thermophilus ZY9) were cultured in MRS broth at 37 °C. HT-29 and Caco-2 cells were cultured in DMEM medium with 10% FBS, 100 mg/mL streptomycin, and 50 mg/mL penicillin G.

2.2. Intestinal Organoid Culture

Organoids from small intestines of C57BL/6 mice (4-week-old) were isolated and cultured as reported by Lee et al. [19]. After mouse intestines were cut into pieces, a gentle cell dissociation reagent (Stemcell, Vancouver, BC, Canada) was used to isolate intestinal crypts, and digestion was terminated by adding 0.1% bovine serum albumin (BSA) in PBS. Next, the intestinal crypt extract was filtrated by using a 70 μm cell strainer, centrifuged at 290× g for 5 min, followed by resuspending the pellets in complete medium (Stemcell, Vancouver, BC, Canada). After mixing the suspension with Matrigel at a volume ratio of 1:1.5, 50 μL mixture was placed on a pre-warmed 48-well plate, followed by incubation at 37 °C for 10 min, then adding 200 μL of complete medium to each well. The organoids were passaged by a combination of digestion and mechanical disruption.
Intestinal organoids were co-cultured with probiotics as previously described [20]. Briefly, after seeding at 50 organoids per well in a 48-well plate, intestinal organoids were co-incubated with YL20 (104 CFU) for 3 days, and their growth status and morphology were observed under a light microscope. EdU staining, RT-PCR and ELISA were performed as described below.

2.3. EdU Staining

The growth of intestinal organoids was detected using an EdU staining kit (Meilunbio, Dalian, China) as instructed by the manufacturer. Briefly, intestinal organoids in each well were incubated with 200 μL of 50 μM EdU medium for 2 h, followed by fixing with paraformaldehyde, permeabilization with 0.5% Triton X-100, and incubation with 1× Apollo reaction cocktail. After staining nuclei with Hoechst 33342, organoids were captured under a fluorescence microscope (Nikon, Tokyo, Japan), and the number of EdU+ cells was calculated.

2.4. Quantitative Real-Time PCR (qRT-PCR)

Before qRT-PCR analysis, organoids treated with CS or/and YL20 were collected and tissue samples were harvested from mouse small intestines, followed by total RNA extraction using Trizol reagent (Invitrogen, Carlsbad, CA, USA) and RNA reverse transcription using M-MLV reverse transcriptase (Promega, Madison, WI, USA) with the primers listed in Table 1. qRT-PCR was performed with Fast SYBR Green Master Mix using the Biosystems StepOneTM Real-time PCR system (Applied Biosystem, Waltham, MA, USA). The relative amounts of mRNA were analyzed using the 2−ΔΔCT method.

2.5. Enzyme Linked Immunosorbent Assay (ELISA)

The level of Mucin 2 (MUC2) in the organoids was detected by co-culturing intestinal organoids with probiotics, followed by collecting the supernatant for ELISA. To detect the levels of MUC2 and cytokines in the small intestines, small intestines were collected from euthanized mice, followed by homogenization, centrifugation, and measuring MUC2 (Cusabio, Wuhan, China), IL-1β (Solarbio, Beijing, China), IL-6 (Solarbio, Beijing, China), and TNF-α (Solarbio, Beijing, China) using ELISA kits as directed by the manufacturers.

2.6. Antagonistic Activity of Probiotics against C. sakazakii Using Agar Well Diffusion Method

The antagonistic activity of probiotics, including YL20, GM20, SW01, and LGG, against C. sakazakii was tested using agar well assay as previously reported with a few modifications [21]. Briefly, the overnight grown probiotic strains in MRS broth were centrifuged (2000× g for 5 min) to obtain supernatants. Meanwhile, the overnight (12 h) cultures of C. sakazakii were laid on the LB agar surface, followed by covering the surface with an Oxford cup (outer diameter 7.8 ± 0.1 mm, inner diameter 6.0 ± 0.1 mm, and height 10.0 ± 0.1 mm) containing 200 μL of each probiotic supernatant. After 24 h of incubation, the inhibition zone diameter (mm) was measured. The test was performed in triplicate and repeated three times.

2.7. Sensitivity to Antibiotics

The detection of YL20 susceptibility to antibiotics was performed followed a previously reported disk-diffusion method [22]. Briefly, the strain was cultured in MRS broth at 37 °C overnight and then diluted in MRS liquid medium to a final inoculation concentration of 107 CFU/mL. Next, 100 µL of diluted culture was coated onto MRS agar, and the antibiotic discs were put on agar surface. After incubation at 37 °C overnight, inhibition zone diameters were measured using a digital caliper. The test was performed in triplicate and repeated three times.

2.8. Invasion Assay

The inhibitory effects of YL20 against C. sakazakii adhering to HT29 cells were investigated by competition, exclusion, and replacement assays according to Fan et al. [5]. Briefly, after seeding at 1 × 105 cells per well in a 24-well plate, HT-29 cells were incubated with 1 × 107 CFU of C. sakazakii for 3 h (Control group). In a competition assay, the cells were incubated with both 1 × 108 CFU of YL20 and 1 × 107 CFU of C. Sakazakii for 3 h. To detect the replacement of C. sakazakii by YL20, cells were infected with 1 × 107 CFU of C. sakazakii for 1.5 h, followed by treatment with 1 × 108 CFU of YL20 for additional 1.5 h. In an exclusion assay, cells were preincubated with 1 × 108 CFU of YL20 for 1.5 h, followed by infection with 1 × 107 CFU of C. Sakazakii for additional 1.5 h (Figure 1A). After washing with PBS to remove the unbound bacterial cells, the HT-29 cells were treated with 0.1% Triton X-100 for 10 min, followed by culturing the broken cells with C. sakazakii on the LB agar plates and then calculating the number of intracellular C. sakazakii cells. The results were presented as the percentage of the invasive bacteria (% CFU invasive bacteria in experiment group/CFU invasive bacteria in control group).

2.9. Western Blotting Analysis

Briefly, after lysis with RIPA lysis buffer, the protein concentrations of HT-29 cells were analyzed using a BCA protein quantitative reagent kit (Solarbio, Beijing, China). After sodium dodecyl sulphate-poly acrylamide gel electrophoresis (SDS-PAGE), the extracted proteins were transferred to a nitrocellulose membrane, probed with primary antibodies against ZO-1 (21773-1-AP, Proteintech Group, Inc., Wuhan, China), occludin (sc-133255, Santa Cruz Biotechnology, Inc., Santa Cruz, CA, USA) and GAPDH (YM3215, ImmunoWay Biotech., Plano, TX, USA) overnight at 4 °C, followed by incubation with secondary antibodies IRDye-800CW IgG (926-32210, Li-COR Biosciences, Lincoln, NE, USA) or IRDye-680RD IgG (926-68071, Li-COR Biosciences, Lincoln, NE, USA) for 2 h at room temperature. The specific bands were analyzed using an Odyssey Infrared Imaging System (Li-COR Biosciences) and quantified using ImageJ software.

2.10. Immunofluorescence Analysis

After incubation with bacteria, Caco-2 cells were fixed in 4% paraformaldehyde for 30 min at room temperature and permeabilized with 0.5% Triton X-100 for 5 min. Subsequently, the cells were blocked in 5% BSA for 1 h at room temperature, followed by immunostaining with anti-ZO-1 antibody (21773-1-AP, Proteintech Group, Inc., Wuhan, China) and tetramethyl rhodamine isothiocyanate (TRITC)-coupled antibody (ZF-0316, ZSGB-BIO, Beijing, China). After nuclei staining with 4′,6-diamidino-2-phenylindole (DAPI), the cells were observed and photographed under a fluorescence microscope.

2.11. Measurement of Transepithelial Electrical Resistance (TEER) and Permeability across Caco-2 Monolayers

After seeding in transwell inserts, Caco-2 cells were cultured for at least 16 days to form monolayers. For TEER measurement, the monolayers were incubated with 1 × 108 CFU of YL20 and 1 × 107 CFU of C. sakazakii, followed by measuring TEER at 0, 6, 18 and 24 h after bacterial exposure using a Millicell electrical resistance apparatus (World Precision Instruments Inc., Sarasota, FL, USA). For paracellular permeability assays, the chambers were equilibrated with Hanks, followed by adding FITC-dextran (1 mg/mL) (Sigma, St Louis, MO, USA) to the upper chamber and incubation at 37 °C for 1.5 h in the dark. Next, the solutions in the lower chamber were collected, followed by measuring the fluorescence intensity at 520 nM with a microplate reader (Tecan, Zürich, Switzerland). As previously reported [23], apparent permeability coefficient (Papp) was counted by the formula: Papp = dQ/(dt × A × C0), where dQ/dt is the permeability rate; A, the diffusion area of monolayer; and C0, the initial concentration of the tested substance in the apical compartment.

2.12. Animal Experiment

All procedures were approved by the Animal Ethics Committee of Tianjin University of Science and Technology. Specifically, pregnant C57BL/6 mice were obtained from the PLA Military Academy of Medical Sciences Laboratory Animal Center (Beijing, China), and after delivery, the newborn pups were kept with their mothers and divided into four groups (7 mice/per goup): Control (PBS-treatment), CS (C. sakazakii-treatment), YL20 (YL20 treatment), and CS + YL20 (co-treatment with C. sakazakii and YL20). Specifically, two-day-old pups were gavaged once per day with 1 × 107 C. sakazakii (CS) or 1 × 107 YL20 (YL20) or both (CS + YL20) in 10 μL sterile PBS, with 10 μL PBS fed once per day for the Control pups. Body weight was recorded every day. After 10 days of experiment, all pups were euthanized, and the entire small intestines were collected, with one part of intestinal tissues fixed with 4% paraformaldehyde, and the other part directly frozen in liquid nitrogen and stored at −80 °C.

2.13. H&E Staining, PAS Staining, and Immunohistochemical Staining

Small intestine segments fixed in paraformaldehyde solution were paraffin embedded and then cut into 5 µM sections, followed by serial dehydration in xylene and ethanol. For observing intestine architecture, the sections were stained with hematoxylin and eosin (H&E). Pathology/inflammation scores was determined based on a previous report [5]. Goblet cells were detected by periodic acid-Schiff (PAS) staining using an AB-PAS Stain Kit (Solarbio, Beijing, China) as guided by the manufacturer. For ZO-1 staining, the sections were blocked in 1% normal goat serum and incubated overnight at 4 °C with an anti-ZO-1 antibody (21773-1-AP, Proteintech Group, Inc., Wuhan, China), and then for 1 h at room temperature with a TRITC-coupled secondary antibody (ZF-0316, ZSGB-BIO, Beijing, China). After nucleus staining with DAPI, all sections were observed and captured using a forward fluorescence microscope (Olympus, Tokyo, Japan).

2.14. Quantification of the Predominant Bacterial Groups in the Intestinal Contents

The genomic DNA of colonic and cecal contents were extracted using the stool genomic DNA extraction kit (Solarbio, Beijing, China). qRT-PCR was performed with Fast SYBR Green Master Mix using the Biosystems StepOneTM Real-time PCR system using primers that specifically target 16S rDNA (Table 2). The amplification was programed to start at 95 °C for 2 min, followed by 40 cycles (degeneration at 95 °C for 10 s, annealing at 60 °C for 30 s). Overall, 16 S rRNA gene abundance in samples was determined by comparing the cycle threshold (Ct) values to those generated by a standard curve.

2.15. Statistical Analysis

GraphPad Prism9 (GraphPad Software, San Diego, CA, USA) was used to assess statistical differences between experimental groups. Statistical differences between two experimental groups were evaluated by Student’s t tests, and statistical differences between multiple groups were calculated using one-way ANOVA followed by Tukey’s post hoc test. Shapiro–Wilk test was used to analyze the normality of variance. The homogeneity test of variance was performed by running one-way ANOVA analysis. Brown–Forsythe and Welch ANOVA test was performed when the variances are not equal. A p-value of 0.05 or lower was considered statistical significant and expressed as * p < 0.05, ** p < 0.01, and *** p < 0.001.

3. Results

3.1. Effects of Lactic Acid Bacteria on Intestinal Organoid Proliferation

To assess the stimulatory effect of lactic acid bacteria on intestinal epithelial cells, intestinal organoids were isolated from mice small intestines as an in vitro model for studying host–microbial interactions. A total of six strains, including Lacticaseibacillus salivarius YL20, Lactobacillus gasseri GM20, Lacticaseibacillus rhamnosus SW01, Lacticaseibacillus paracasei TX01, Lactobacillus delbrueckii Y2 and Streptococcus thermophilus ZY9 were isolated from breast milk and newborn feces and used for preliminary evaluation, with LGG as a positive control strain. As shown in Figure 1A,B, compared with control group, YL20, GM20 and SW01 could significantly promote cellular proliferation in organoids (p < 0.01, p < 0.001), with an EdU positive cell percentage of 18.17 ± 0.80%, 14.89 ± 1.02% and 13.22 ± 0.69%, respectively. Meanwhile, the control strain LGG showed an EdU positive cell percentage of 15.53 ± 1.08%. Additionally, the resistance of these three strains and LGG to C. sakazakii was detected by agar well diffusion method. In Table 3, it was shown that, compared with the other lactic acid bacteria, YL20 showed a larger bacteriostatic circle against C. sakazakii. In Table 4, antibiotic susceptibility test results indicated that YL20 was resistant to penicillin and streptomycin, but susceptible to other antibiotics, indicating that L. salivarius YL20 could be used for subsequent experiments.

3.2. L. salivarius YL20 Attenuates C. sakazakii-Induced Damage of Intestinal Organoids by Promoting ISC-Mediated Epithelial Cell Proliferation and Enhancing Intestinal Barrier Function

The isolated small intestinal crypts formed bud structures and protruded outward for 2 to 3 d. The intestinal organoids were co-treated with YL20 and C. sakazakii for 2 d. As shown in Figure 2A–C, compared with the Control group, YL20 group showed a significant increase in the volume of organoids, and a notable increase in the number of buds and budding rate of organoids (p < 0.05). Furthermore, C. sakazakii infection caused the disappearance of buds and the disruption of organoids (p < 0.05, p < 0.01). Compared with the CS group, the CS + YL20 group could significantly inhibit the C. sakazakii-induced damage of organoids, with a significant increase in bud number (p < 0.001). Additionally, compared with the Control group, the CS group showed a decrease in the mRNA level of intestinal stem cell marker Lgr5 (p < 0.05), while the Lgr5 mRNA level was restored in CS + YL20 group (Figure 2D), suggesting that YL20 could promote intestinal stem cell proliferation. YL20 could also up-regulate the mRNA level of tight junctional protein Occludin (p < 0.05) and Zo-1 (p < 0.05) in C. sakazakii-infected organoids (Figure 2E,F). The C. sakazakii-induced decrease in the mRNA and protein level of MUC2 could be partly restored in the CS + YL20 group (p < 0.05) (Figure 2G,H), indicating the contribution of YL20 to the improvement of intestinal mucosal barrier. These results confirmed that L. salivarius YL20 could alleviate C. sakazakii-induced damage of intestinal organoids by increasing ISCs-mediated intestinal epithelial cell proliferation and improving intestinal barrier integrity.

3.3. L. salivarius YL20 Inhibits C. sakazakii Adherence to Intestinal Cells and Enhances the Expression of TJ Proteins in Intestinal Epithelial Cells

The adhesion and invasion ability of C. sakazakii to host intestinal epithelial cells is critical to disease pathogenesis. C. sakazakii is considered to invade and translocate into the blood stream to cause infection through intestinal epithelial cells [30], suggesting that the ability of probiotics to prevent/reduce pathogenic bacteria adherence to intestinal epithelial cells is very important in the prevention of pathogen infection. The potential antagonistic properties of YL20 against C. sakazakii were explored by using an in vitro model based on HT-29 cells. According to the adding sequence of YL20 and C. sakazakii into cell co-cultures, three adhesion experiments (competition, replacement, and exclusion) were designed, and the results are shown in Figure 3A. YL20 was shown to expel C. sakazakii from HT-29 cells with almost 70–80% efficiency (p < 0.01), suggesting its suppressive effect against C. sakazakii infection in HT-29 cells. Additionally, the effect of YL20 on epithelial barrier function was further investigated by analyzing tight junction protein expression in the intestine cell lines. In Figure 3B–D, C. sakazakii infection was seen to significantly decrease the expression of ZO-1 (p < 0.001) and occludin (p < 0.05), whereas YL20 pretreatment could significantly increase ZO-1 expression (p < 0.01) in C. sakazakii-infected HT-29 cells. Meanwhile, YL20 could also increase the occludin expression in C. sakazakii-infected HT-29 cells, but not significantly. Immunofluorescence staining confirmed that YL20 pretreatment could prevent the C. sakazakii-induced destruction of ZO-1 expression in Caco-2 cells (Figure 3E). These results indicated that YL20 could inhibit C. sakazakii adhesion to epithelial cells and C. sakazakii-induced low TJ protein expression.

3.4. L. salivarius YL20 Reverses TEER Decrease and Corresponding Membrane Permeability Increase across C. sakazakii-Infected Caco-2 Monolayers

The beneficial effect of YL20 on the intestinal barrier function was further tested by co-incubation of caco-2 monolayers with YL20 and C. sakazakii, followed by measuring TEER at 0, 6, 12, 18 and 24 h. In Figure 4A, CS treatment was seen to significantly (p < 0.001) reduce the TEER of Caco-2 monolayers from 715.67 ± 5.66 Ω/cm2 to 340.66 ± 46.65 Ω/cm2 in a time-dependent manner, but this TEER reduction was significantly (p < 0.001) reversed at 24 h in CS + YL20 treatment group. In Figure 4B, the effect of YL20 on the permeability of Caco-2 monolayers to FITC-dextran was detected following 1.5 h of exposure to C. sakazakii. The Papp values were 4.54 × 10−6 and 18.51 × 10−6 for Control and CS groups, respectively, suggesting that C. sakazakii infection could significantly increase permeability (# p < 0.05 vs. Control group). Additionally, compared with the CS group, the CS + YL20 group showed a significant (p < 0.05) decrease in permeability. These results showed that YL20 could restore TEER, prevent membrane permeability, and enhance intestinal barrier function.

3.5. YL20 Administration Attenuates C. sakazakii-Induced Clinical Symptoms and Intestinal Epithelial Damage in Newborn Mice

To evaluate whether YL20 could prevent C. sakazakii-induced NEC in vivo, newborn mice were gavaged with C. sakazakii or YL20 or both once per day from postnatal day 2 (P2) to postnatal day 10 (P10), with 10 μL PBS for Control mice. After infection with the C. Sakazakii strain, the mice pups showed severe weight loss from day 6 to 10 (# p < 0.05, ## p < 0.01 vs. Control group) (Figure 5A). YL20 intervention was shown to be effective in reducing weight loss. Compared with CS pups, CS + YL20 pups showed a significant increase in body weight (* p < 0.05, ** p < 0.01) (Figure 5A). Meanwhile, the mortality rate of mice was evaluated for each group, and CS pubs began to die on day 9, with a mortality rate of ~70% on day 10, in contrast to no death in the other three groups (Figure 5B).
Furthermore, the intestinal tissues from the C. sakazakii-infected mice showed severe epithelial damage, including villus cell loss, epithelial sloughing, and intestinal epithelial cell rupture. In Figure 5D, it was shown that compared with the Control pups, the CS pups showed higher pathological scores (p < 0.01), and compared with the CS pups, the CS + YL20 pups showed less intestinal injury (p < 0.0001). The morphology of intestines, especially the length of the villus and the ratio of the intestinal villus length to crypt depth, is positively correlated with intestine health [31]. In Figure 5E, the YL20 pups exhibited an increase in villus length relative to the Control pups, suggesting that YL20 could promote intestinal development. Compared with the Control pups, the CS pups showed a decrease of villus length (p < 0.01), but this decrease in villus length was significantly reversed in the CS + YL20 pups relative to the CS pups (p < 0.01) (Figure 5E). These observations indicated that YL20 could improve mice survival rate and attenuate C. sakazakii-induced intestinal injury.

3.6. YL20 Administration Inhibits C. sakazakii-Induced Rise of Inflammatory Factors in the Intestinal Tract of Newborn Mice

C. sakazakii-induced intestinal inflammation is associated with high levels of proinflammatory cytokines. The anti-inflammatory effects of YL20 were investigated by measuring the levels of inflammatory cytokines in mice small intestines with real-time PCR and ELISA. As shown in Figure 6A–C, the CS pups showed significant upregulation in the mRNA levels of IL-1β, IL-6 and TNF-α (p < 0.05, p < 0.01 vs. Control group), whereas this C. sakazakii-induced increase of these proinflammatory cytokines was obviously suppressed in the CS + YL20 pups (p < 0.05, p < 0.01 vs. CS group). In Figure 6D–F, compared with the Control group, the CS group showed significantly higher levels of these proinflammatory cytokines (p < 0.05, p < 0.01, p < 0.001), but this effect was significantly suppressed in the CS + YL20 group (p < 0.05, p < 0.01 vs. CS group). These results showed that YL20 could decrease the levels of proinflammatory cytokines, thus contributing to the prevention of C. sakazakii-induced NEC.

3.7. YL20 Administration Improves Intestinal Barrier Integrity and Inhibits C. sakazakii-Induced Intestinal Barrier Damage

The effects of YL20 on the mucosal barrier in the in vivo model were evaluated by PAS staining analysis of the intestines of mice pups and RT-PCR and ELISA analysis of MUC2 levels. In Figure 7A,B, compared with the Control pups, the CS pups showed a significant decrease in the number of goblet cells (p < 0.05), while this reduction was reversed in the CS + YL20 pups relative to the CS pups (p < 0.05). In addition, the goblet cell number significantly increased in the YL20 pups relative to the Control pups (p < 0.05) (Figure 7B). Moreover, compared with the Control pups, the CS pups showed a notable downregulation in the mRNA level of Mucin-2 (p < 0.05) and this C. sakazakii-induced decrease in the mRNA level of MUC2 was obviously suppressed in the CS + YL20 pups (p < 0.05 vs. CS group) (Figure 7C). In Figure 7D, the decrease of MUC2 production was observed in the intestines of the CS pups (p < 0.05 vs. Control group), but was restored in the CS + YL20 pups (p < 0.05 vs. CS group).
The effects of YL20 on TJ protein levels in the in vivo model were analyzed by immunofluorescence staining of ZO-1 in the intestine of mice pups. In Figure 7E, the CS pups were lower than the Control pups in ZO-1 expression. The differences in the response of TJ protein expression to C. sakazakii infection with or without YL20 treatment were confirmed by immunoblot analysis of ZO-1, with a higher ZO-1 expression in the YL20 + CS pups than the CS mice pups (Figure 7E).
Furthermore, the effects of YL20 on intestinal stem cell proliferation were determined by RT-PCR analysis of Lgr5 mRNA level in the intestines of mice pups, and the results are shown in Figure 7F. The mRNA level of Lgr5 was remarkably increased (p < 0.05) in the YL20 pups relative to the Control pups, suggesting that YL20 could promote the proliferation of intestinal stem cells. Meanwhile, the CS pups showed a significant decrease in Lgr5 mRNA level (p < 0.05 vs. Control group), but this C. Sakazakii-induced decrease of Lgr5 mRNA level was effectively curbed in the CS + YL20 pups (p < 0.05 vs. CS group). These data supported that YL20 could improve tight junction and intestinal mucosal barrier integrity, thus playing a protective role against C. sakazakii-induced NEC.

3.8. YL20 Administration Improves Intestinal Microbiota Composition

As shown in Table 5, there was no significant difference in the total bacteria concentrations among the four groups. Compared to the Control group, C. sakazakii infection increased the abundance of Enterobacterium and Enterococcus, and decreased the abundance of Bifidobacterium, Bacteroidetes, and Lactobacillus. However, the administration of YL20 partly restore the proportions of these bacteria, resulting in a higher relative abundance of Lactobacillus and a lower relative abundance of Enterobacterium in the CS + YL20 group than in the YL20 group. Furthermore, the abundance of Lactobacillus was significantly increased and the abundance of Enterobacterium and Enterococcus was decreased in the YL20 group, compared to the Control group. Both C. sakazakii infection and YL20 administration had no significant effect on the populations of Clostridium perfringens.

4. Discussion

C. Sakazakii can cause serious NEC in infants, especially premature infants or low birth weight infants. The mechanism by which this disease affects patients is still not fully understood, thus limiting the development of treatment strategies for C. sakazakii-induced NEC other than supportive care. Probiotics have gained increasing attention because of their benefits to human digestive and immune systems. Here, we reported a new probiotic strain L. salivarius YL20, which could improve intestinal barrier function and mitigate C. sakazakii-induced NEC by promoting intestinal epithelial cell proliferation and repair.
Intestinal epithelial proliferation and replacement is sustained by ISCs, playing a very important role in intestinal barrier maintenance and intestinal injury repair [32]. In previous studies, intestinal organoids cultured in three-dimension (3D) were used as an in vitro model to explore the effects and mechanisms of host–microbial interactions [18]. In this study, we first established an ex vivo model of C. sakazakii-infected intestinal organoids and evaluated the effects of L. salivarius YL20 on intestinal epithelial proliferation and mucosal barrier function. Our results confirmed that L. salivarius YL20 could stimulate epithelial cell proliferation in organoids, promote the growth of intestinal organoids and protect their morphology under C. sakazakii infection by increasing the number of buds per organoid, the percentage of budding organoids, and the mRNA level of Lgr5. Recently, by using an in vitro intestinal organoid model and in vivo experimental animal model, researchers have investigated the effects of other probiotics on intestinal development as well as ISC growth and differentiation. For instance, neonatal colonization of mice treated with LGG showed enhancement in the proliferation and differentiation of intestinal epithelial cells [33], and the mRNA levels of Toll-like receptor 3 (TLR3) were increased in LGG-treated intestinal organoids [34]. Additionally, Limosilactobacillus reuteri D8 was reported to stimulate the growth of intestinal organoids in vitro and ameliorate DSS-induced intestinal mucosa damage in vivo, indicating that this protective effect was achieved through accelerating ISC regeneration [20]. Moreover, by using intestinal organoids and Lgr5+ mice, Lee et al. confirmed that Bifidobacterium and Lactobacillus spp. could stimulate the proliferation of ISCs and the regeneration of intestinal epithelial cells, with lactate as the main effective substance [35]. Consistent with these studies, L. salivarius YL20 could activate ISC-mediated intestinal epithelial cell proliferation, thus playing a protective role in C. sakazakii-induced intestinal organoid damage.
MUC2, the main component of the mucus layer, is produced by goblet cells and exerts a protective effect against chemical and microbial damage on the intestinal epithelial surface. As reported by Panida Sittipo et al., intestinal organoids derived from irradiated mice showed impaired budding, as well as decreased expression levels of Lgr5, Ki67 and Muc2, which could be reversed by heat-killed Lactobacillus acidophilus [36]. Several lactobacillus strains were shown to induce mucin expression, thereby blocking adhesion of pathogens to the intestinal epithelial [37,38,39]. For instance, Lactobacillus spp. could upregulate MUC3 expression in human intestinal epithelial cells, while stimulating MUC2 production and secretion [38,40]. Limosilactobacillus reuteri could attenuate DSS-induced colitis in mice by increasing mucus thickness [41]. Here, YL20 could up-regulate the mRNA level of Muc2 and stimulate MUC2 secretion in C. sakazakii-infected intestinal organoids.
Tight junctions are vital to maintain intestinal barrier integrity. The formation of TJ is very important to prevent the paracellular spread of bacteria, thus contributing to the resistance of intestinal inflammatory and infectious diseases in the infantile period. Several important epithelial TJ proteins, such as ZO-1, occludin, etc., contributed to the maintenance of intestinal epithelial barrier integrity [42]. Here, we investigated whether YL20 could increase the expression of these TJ proteins in intestinal organoids and intestinal epithelial cell lines. Our data indicated that YL20 treatment could reverse the C. sakazakii-induced low mRNA levels of Zo-1 and Occludin in intestinal organoids and restore their respective protein levels in C. sakazakii-infected HT-29 cells. Immunostaining of ZO-1 also indicated the protective effect of YL20 on the maintenance of tight junction integrity in Caco-2 cells. Our results are consistent with two previous studies on B. fragilis ZY-312 and L. salivarius. Specifically, pretreatment of B. fragilis ZY-312 could increase ZO-1 and occludin expression in C. sakazakii-infected Caco-2 cells [5]. L. salivarius was shown to increase the levels of ZO-1 and occludin in enterotoxigenic Escherichia coli (ETEC) K88 infected IPEC-J2 cells [43].
Adhesion and invasion are critical steps for C. sakazakii to enter host cells, leading to intestinal and extraintestinal diseases. Many isolated strains of C. sakazakii were reported to have the ability to adhere to human intestinal epithelial and endothelial cells [44], suggesting preventing C. sakazakii adhesion to intestinal epithelium could effectively inhibit its infection. Multiple probiotics, including B. fragilis ZY-312 [5], Lacticaseibacillus paracasei FJ861111.1 [21], etc. [45,46], were found to inhibit the adhesion of C. sakazakii to epithelial cells and intestinal mucus. Consistent with these studies, our results demonstrated that YL20 could inhibit the adhesion of C. sakazakii to epithelial cells in competition, replacement, and exclusion assays.
Intestinal barrier integrity is very important for resisting the invasion of pathogens. TEER and permeability assays were performed to study the protective effect of YL20 on C. sakazakii-induced epithelial barrier damage in Caco-2 monolayers. Our results showed that the TEER of C. sakazakii-infected Caco-2 monolayers decreased gradually over time, indicating the disruptive effect of C. sakazakii on epithelial barrier. However, YL20 treatment could reverse C. sakazakii-induced TEER reduction. Moreover, the disruptive effect of C. sakazakii on the monolayers was confirmed by an increase in the permeability of monolayers to FITC-dextran and this change could be reversed by YL20 treatment, indicating that YL20 could play an important role in protecting intestinal epithelial barrier integrity. This was consistent with several previous studies. Ruchi Jariwala et al. reported that all strains, including the nine lactobacillus strains (Limosilactobacillus fermentum FA-1,FA-5, GKI-1, GPI-3, GPI-7, and IIs11.2; Lactobacillus helveticus FA-7; Lactiplantibacillus plantarum GRI-2; L. salivarius GPI-1(S)) and LGG, were able to reverse enteropathogenic E. coli-induced TEER decreases and permeability increases across Caco-2 monolayers [47]. Fan et al. also determined that C. sakazakii infection induced a reduction in the TEER of Caco-2 monolayers in a time-dependent manner, and this TEER reduction was alleviated by B. fragilis ZY-312 treatment [5].
The research of probiotics against C. sakazakiiis-induced NEC in vivo is limited as compared to other enteropathogens. Lactobacillus lactis has been confirmed to reduce NEC incidence and severity in a preterm rabbit model [14]. Conditioned medium from B. infantis was demonstrated to mitigate C. sakazakii-induced NEC in newborn mice by preventing the reduction of body weight, the apoptosis of enterocytes, and the reduction of mucin production [15]. Here, our data confirmed that YL20 administration could increase body weight, reduce mortality and intestinal epithelium damage in C. sakazakii-infected mice. Additionally, YL20 could also restore the number of goblet cells, the production of MUC2, and the expression of ZO-1, indicating its protective effect in intestinal barrier function against pathogen infection. Furthermore, YL20 treatment alone could also increase villus height and Lgr5 mRNA level as well as up-regulate the number of goblet cells and the levels of MUC2. Combined with the results of organoid experiment in vitro, YL20 could contribute to intestine development and intestinal mucosal barrier formation by promoting ISC-mediated epithelial cell proliferation.
Ariadnna et al. demonstrated that flagella produced by Cronobacter species could activate pro-inflammatory cytokines TNF-α and IL-8 in macrophage derivatives from human monocytes [48]. C. sakazakii infection could up-regulate the relative mRNA levels of COX-2, IL-1β, IL-6, IL-8, iNOS, and TNF-α in human brain microvascular endothelial cells [49]. In this study, C. sakazakii infection was shown to stimulate the activation of pro-inflammatory factors such as IL-1β, IL-6, and TNFα in mice, and these C. sakazakii-induced inflammatory responses could be mitigated by YL20 administration. This agreed well with a previous report that B. fragilis ZY-312 could attenuate clinical symptoms and decrease the levels of TNF-α and IFN-γ in C. sakazakii-infected neonatal rats [5].
At present, there are few reports about the effect of C. sakazakii on intestinal microbiota. Recently, Alfreda et al. investigated the inhibitory effect of a potential synbiotic (six lactic acid bacteria strains and Vivinal GOS) on the growth of C. sakazakii, using a simulator of the human intestinal microbial ecosystem (SHIME) inoculated with infant fecal matter [50]. They reported a strong negative correlation between Cronobacter and Bifidobacterium, suggesting that the presence of Bifidobacterium in the gut of healthy infants could contribute to the inhibition of C. sakazakii. Premature or low birth weight infants may be more susceptible to C. sakazakii infection because they may lack some beneficial gut microbiota, including Bacteroides and bifidobacteria [51,52,53]. Consistent with Alfreda’s reports, our data confirmed that C. sakazakii infection led to the decrease in the abundance of Bifidobacterium. C. sakazakii infection also reduced the populations of beneficial bacteria Bacteroidetes and Lactobacillus, and enhanced the potential enteropathogenic bacteria Enterobacterium and Enterococcus, while these changes were partly reversed by the administration of YL20.
In this study, L. salivarius YL20 treatment was demonstrated to restore the budding and growth of organoids, up-regulate the mRNA level of Lgr5, Zo-1 and Occludin, and promote the production of MUC2 in C. sakazakiiis-infected intestinal organoids. Additionally, YL20 could inhibit C. sakazakii invasion and reverse the C. sakazakii-induced low protein expression of ZO-1 and occludin in HT-29 cells. Moreover, YL20 could prevent TEER decreases and corresponding permeability increases across C. sakazakii-infected Caco-2 monolayers. Furthermore, YL20 could effectively attenuate epithelial barrier damage and inflammation, thereby preventing the development of NEC in neonatal mice. Our findings have demonstrated for the first time that YL20 can improve intestinal stem cell function and enhance intestinal barrier integrity, thus contributing to the prevention of C. sakazakii-induced NEC.

Author Contributions

W.W., N.W. and M.G. contributed to the experiment design and manuscript preparation; M.G., C.Z. (Caixia Zhu) and T.Z. (Tengxun Zhang) contributed to the operation of experiments and analysis of data. L.H., Y.Z. and C.Z. (Chongjie Zhao) contributed to the data processing. X.D. and T.Z. (Tongcun Zhang) provided technical support. All authors have read and agreed to the published version of the manuscript.

Funding

This work was supported by the grants from the National Key R&D Program of China [No. 2017YFD0400304], the Innovative Research Team of Tianjin Municipal Education Commission [No. TD13-5015], and the National Natural Science Foundation of China [No. U20A20400, 82174060].

Institutional Review Board Statement

All animal experiments were approved by the Institutional Animal Care and Use Committee at Tianjin University of Science and Technology (No. 20200517CB) and performed following the National Institutes of Health Guide for the Care and Use of Laboratory Animals (8th Edition, revised in 2011).

Informed Consent Statement

Not applicable.

Data Availability Statement

The data obtained in this study are available on request from the author.

Conflicts of Interest

The authors declare no conflict of interest.

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Figure 1. Effects of lactic acid bacteria on intestinal organoid proliferation. (A) Images of intestinal organoids stained with Hoechst33342 (blue) and EdU (green); scale bar = 50 μm. (B) Percentage of EdU-positive cells calculated for different lactic acid bacteria. ## p < 0.01, ### p < 0.001 vs. Control group, n = 3.
Figure 1. Effects of lactic acid bacteria on intestinal organoid proliferation. (A) Images of intestinal organoids stained with Hoechst33342 (blue) and EdU (green); scale bar = 50 μm. (B) Percentage of EdU-positive cells calculated for different lactic acid bacteria. ## p < 0.01, ### p < 0.001 vs. Control group, n = 3.
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Figure 2. Effects of L. salivarius YL20 on C. sakazakii-induced damage of intestinal organoids. (A) Effects of YL20 on the growth of C. sakazakii-infected organoids; the upper four images scale bar = 50 μm, the lower four images scale bar = 100 μm. (B) The number of buds per organoid. (C) The percentage of budding organoids. Effects of YL20 on the mRNA level of Lgr5 (D), Occludin (E), Zo-1 (F) and Muc2 (G) in C. sakazakii-infected organoids tested by RT-PCR. (H) The expression of MUC2 in the supernatant of intestinal organoids. # p < 0.05, ## p < 0.01 vs. Control group; * p < 0.05; *** p < 0.001 vs. CS group; n = 3.
Figure 2. Effects of L. salivarius YL20 on C. sakazakii-induced damage of intestinal organoids. (A) Effects of YL20 on the growth of C. sakazakii-infected organoids; the upper four images scale bar = 50 μm, the lower four images scale bar = 100 μm. (B) The number of buds per organoid. (C) The percentage of budding organoids. Effects of YL20 on the mRNA level of Lgr5 (D), Occludin (E), Zo-1 (F) and Muc2 (G) in C. sakazakii-infected organoids tested by RT-PCR. (H) The expression of MUC2 in the supernatant of intestinal organoids. # p < 0.05, ## p < 0.01 vs. Control group; * p < 0.05; *** p < 0.001 vs. CS group; n = 3.
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Figure 3. Effects of L. salivarius YL20 on C. sakazakii adherence to intestinal cells and the expression of TJ proteins in intestinal epithelial cells. (A) Effects of YL20 on C. sakazakii invasion of HT-29 cells. The results were presented as the percentage of the invasive bacteria (% CFU invasive bacteria in the experiment group/CFU invasive bacteria in the control group). (B) Western blotting analysis of the effects of YL20 on the expression of ZO-1 and occludin in C. sakazakii-infected HT-29 cells. (C,D) Quantification of the TJ proteins using Image J software. (E) Immunofluorescent staining analysis of ZO-1, scale bar = 50 μm. # p < 0.05, ## p < 0.01, ### p < 0.001 vs. Control group; ** p < 0.01 vs. CS group; n = 3.
Figure 3. Effects of L. salivarius YL20 on C. sakazakii adherence to intestinal cells and the expression of TJ proteins in intestinal epithelial cells. (A) Effects of YL20 on C. sakazakii invasion of HT-29 cells. The results were presented as the percentage of the invasive bacteria (% CFU invasive bacteria in the experiment group/CFU invasive bacteria in the control group). (B) Western blotting analysis of the effects of YL20 on the expression of ZO-1 and occludin in C. sakazakii-infected HT-29 cells. (C,D) Quantification of the TJ proteins using Image J software. (E) Immunofluorescent staining analysis of ZO-1, scale bar = 50 μm. # p < 0.05, ## p < 0.01, ### p < 0.001 vs. Control group; ** p < 0.01 vs. CS group; n = 3.
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Figure 4. Effects of L. salivarius YL20 on TEER and membrane permeability of C. sakazakii-infected Caco-2 monolayers. (A) During co-incubation of Caco-2 monolayers with YL20 and C. sakazakii, TEER was measured at 0, 6, 12, 18, and 24 h. (B) Permeability of Caco-2 monolayer to FITC-dextran after treatment with YL20 and/or C. sakazakii. # p < 0.05, ## p < 0.01, ### p < 0.001 vs. Control group; * p < 0.05, *** p < 0.001 vs. CS group; n = 3.
Figure 4. Effects of L. salivarius YL20 on TEER and membrane permeability of C. sakazakii-infected Caco-2 monolayers. (A) During co-incubation of Caco-2 monolayers with YL20 and C. sakazakii, TEER was measured at 0, 6, 12, 18, and 24 h. (B) Permeability of Caco-2 monolayer to FITC-dextran after treatment with YL20 and/or C. sakazakii. # p < 0.05, ## p < 0.01, ### p < 0.001 vs. Control group; * p < 0.05, *** p < 0.001 vs. CS group; n = 3.
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Figure 5. Effects of YL20 on C. sakazakii-induced clinical symptoms and intestinal epithelial damage in newborn mice. (A) Changes in body weight were monitored daily. (B) Mortality rate for neonatal mice in different groups during experiments. (C) Images of H&E-stained small intestinal sections from C. sakazakii-infected mice with or without YL20 administration; scale bar = 100 μm. (D) Pathology/inflammation scores. (E) The length of villus was measured in at least 50 villi/mouse. # p < 0.05, ## p < 0.01 vs. Control group; * p < 0.05, ** p < 0.01, **** p < 0.0001 vs. CS group; n = 3–7.
Figure 5. Effects of YL20 on C. sakazakii-induced clinical symptoms and intestinal epithelial damage in newborn mice. (A) Changes in body weight were monitored daily. (B) Mortality rate for neonatal mice in different groups during experiments. (C) Images of H&E-stained small intestinal sections from C. sakazakii-infected mice with or without YL20 administration; scale bar = 100 μm. (D) Pathology/inflammation scores. (E) The length of villus was measured in at least 50 villi/mouse. # p < 0.05, ## p < 0.01 vs. Control group; * p < 0.05, ** p < 0.01, **** p < 0.0001 vs. CS group; n = 3–7.
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Figure 6. Effects of YL20 administration on C. sakazakii-induced inflammatory factors in the intestinal tract of newborn mice. (A–C) RT-PCR analysis of the mRNA levels of IL-1β, IL-6 and TNF-α in small intestinal tissues from C. sakazakii-infected mice with or without YL20 administration. (D–F) ELISA analysis of the release of pro-inflammatory cytokines. # p < 0.05, ## p < 0.01, ### p < 0.001 vs. Control group; * p < 0.05, ** p < 0.01 vs. CS group; n = 3.
Figure 6. Effects of YL20 administration on C. sakazakii-induced inflammatory factors in the intestinal tract of newborn mice. (A–C) RT-PCR analysis of the mRNA levels of IL-1β, IL-6 and TNF-α in small intestinal tissues from C. sakazakii-infected mice with or without YL20 administration. (D–F) ELISA analysis of the release of pro-inflammatory cytokines. # p < 0.05, ## p < 0.01, ### p < 0.001 vs. Control group; * p < 0.05, ** p < 0.01 vs. CS group; n = 3.
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Figure 7. Effects of YL20 administration on intestinal barrier integrity and C. sakazakii-induced intestinal barrier damage. (A) PAS staining analysis of C. sakazakii-infected mice pups with or without YL20 administration; scale bar = 100 μm. (B) The number of positively stained cells. (C) The mRNA levels of Muc2 in small intestine tissues of pups by RT-PCR. (D) The protein levels of MUC2 in small intestine tissues of pups by ELISA. (E) Immunohistochemical staining analysis of ZO-1 expression levels in the intestines of mice pups; scale bar = 100 μm. (F) The mRNA levels of Lgr5 in small intestine tissues of mice pups by RT-PCR. # p < 0.05 vs. Control group; * p < 0.05 vs. CS group; n = 3.
Figure 7. Effects of YL20 administration on intestinal barrier integrity and C. sakazakii-induced intestinal barrier damage. (A) PAS staining analysis of C. sakazakii-infected mice pups with or without YL20 administration; scale bar = 100 μm. (B) The number of positively stained cells. (C) The mRNA levels of Muc2 in small intestine tissues of pups by RT-PCR. (D) The protein levels of MUC2 in small intestine tissues of pups by ELISA. (E) Immunohistochemical staining analysis of ZO-1 expression levels in the intestines of mice pups; scale bar = 100 μm. (F) The mRNA levels of Lgr5 in small intestine tissues of mice pups by RT-PCR. # p < 0.05 vs. Control group; * p < 0.05 vs. CS group; n = 3.
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Table
Table 1. Primers used in real-time PCR.
Table 1. Primers used in real-time PCR.
Gene NamePrimer Sequence
Tnf-αGCTCTGTGAAGGGAATGGGTGTT
GTCCAGGTCACTGTCCCAGCATC
Il-6ACTTCCATCCAGTTGCCTTCTTG
TGTTGGGAGTGGTATCCTCTGTG
Il-1βCAGAGTTCCCCAACTGGTACATC
GGGAAGGCATTAGAAACAGTCC
GapdhTGCCCAGAACATCATCCCT
TCCTCAGTGTAGCCCAAG
Muc2GACGGCGATGTCTACCGATT
TCCTTGTAGGAGTCTCGGCA
Lgr5CCTACTCGAAGACTTACCCAGT
GCATTGGGGTGAATGATAGCA
Zo-1GTTGGTACGGTGCCCTGAAAGA
GCTGACAGGTAGGACAGACGAT
OccludinTGGCAAGCGATCATACCCAGAG
CTGCCTGAAGTCATCCACACTC
Table
Table 2. Primers used for bacteriological analyses.
Table 2. Primers used for bacteriological analyses.
Target OrganismOligonucleotide Sequence (5′–3′)Reference
Total bacterialF′-CGGTGAATACGTTCYCGG
R′-GGWTACCTTGTTACGACTT		[24]
BacteroidetesF′-GGTGTCGGCTTAAGTGCCAT
R′-CGGAYGTAAGGGCCGTGC		[25]
LactobacillusF′-AGCAGTAGGGAATCTTCCA
R′-CACCGCTACACATGGAG		[26]
BifidobacteriumF′-AGGGTTCGATTCTGGCTCAG
R′-CATCCGGCATTACCACCC		[26]
EnterobacteriaceaeF′-CATTGACGTTACCCGCAGAAGAAG
R′-CTCTACGAGACTCAAGCTTGC		[27]
EnterococcusF′-CCCTTATTGTTAGTTGCCATCAT
R′-ACTCGTTGTACTTCCCATTGT		[28]
Clostridium perfringensF′-CGCATAACGTTGAAAGATGG
R′-CCTTGGTAGGCCGTTACCC		[29]
Table
Table 3. Antagonistic activity of lactic acid bacteria against C. sakazakii.
Table 3. Antagonistic activity of lactic acid bacteria against C. sakazakii.
Bacterial StrainDiameter (mm)
Lacticaseibacillus salivarius YL2012.5 a ± 0.3
Lactobacillus gasseri GM2012.1 a ± 0.8
Lacticaseibacillus rhamnosus SW0111.1 a ± 0.7
Lacticaseibacillus rhamnosus GG11.9 a ± 0.7
a Means in the column with the same superscript letter are not significantly different.
Table
Table 4. Antibiotic susceptibility of L. salivarius YL20.
Table 4. Antibiotic susceptibility of L. salivarius YL20.
AntibioticContentInhibition Zone Diameter
(mm)		Sensitivity
Penicillin10 IU7.1 ± 0.2R
Streptomycin10 μg10.3 ± 0.3R
Gentamicin10 μg17.2 ± 0.6S
kanamycin30 μg19.2 ± 0.8S
Tetracycline30 μg35.5 ± 0.5S
Chloramphenicol30 μg26.3 ± 0.8S
Ciprofloxacin5 μg27.9 ± 0.9S
Rifampicin5 μg32.5 ± 0.7S
Cephalothi30 μg30.2 ± 0.8S
Cefotaxime Sodium30 μg34.8 ± 0.6S
Ceftazidime30 μg22.5 ± 0.7S
Erythromycin15 μg24.0 ± 0.7S
Vancomycin30 μg15.8 ± 0.8S
Cotrimoxazole1.25 μg20.3 ± 0.8S
Imipenem10 μg36.0 ± 0.8S
S: susceptible, R: resistance.
Table
Table 5. Effect of YL20 on the abundance of dominant groups of bacteria (Lg [copies/g]).
Table 5. Effect of YL20 on the abundance of dominant groups of bacteria (Lg [copies/g]).
Target OrganismControlCSYL20CS + YL20
Total bacterial42.45 ± 0.33 a42.16 ± 0.20 a42.39 ± 0.38 a41.97 ± 0.19 a
Bacteroidetes4.98 ± 0.32 a3.95 ± 0.13 b4.22 ± 0.17 ab4.01 ± 0.14 ab
Lactobacillus7.17 ± 0.12 b5.87 ± 0.07 c8.32 ± 0.05 a7.33 ± 0.04 b
Bifidobacterium5.68 ± 0.12 a4.32 ± 0.13 b5.35 ± 0.25 ab5.13 ± 0.19 ab
Enterobacteriaceae5.20 ± 0.04 b6.30 ± 0.08 a4.28 ± 0.08 c5.33 ± 0.05 b
Enterococcus5.53 ± 0.11 b6.69 ± 0.23 a4.93 ± 0.15 c5.81 ± 0.32 ab
Clostridium perfringens7.10 ± 0.16 a7.31 ± 0.20 a6.93 ± 0.28 a7.45 ± 0.13 a
a, b, c Values with different superscripts within the same row indicate significant differences, p < 0.05.
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Wang, W.; Geng, M.; Zhu, C.; Huang, L.; Zhang, Y.; Zhang, T.; Zhao, C.; Zhang, T.; Du, X.; Wang, N. Protective Effects and Mechanism of a Novel Probiotic Strain Ligilactobacillus salivarius YL20 against Cronobacter sakazakii-Induced Necrotizing Enterocolitis In Vitro and In Vivo. Nutrients 2022, 14, 3827. https://doi.org/10.3390/nu14183827

AMA Style

Wang W, Geng M, Zhu C, Huang L, Zhang Y, Zhang T, Zhao C, Zhang T, Du X, Wang N. Protective Effects and Mechanism of a Novel Probiotic Strain Ligilactobacillus salivarius YL20 against Cronobacter sakazakii-Induced Necrotizing Enterocolitis In Vitro and In Vivo. Nutrients. 2022; 14(18):3827. https://doi.org/10.3390/nu14183827

Chicago/Turabian Style

Wang, Weiming, Meng Geng, Caixia Zhu, Lei Huang, Yue Zhang, Tengxun Zhang, Chongjie Zhao, Tongcun Zhang, Xinjun Du, and Nan Wang. 2022. "Protective Effects and Mechanism of a Novel Probiotic Strain Ligilactobacillus salivarius YL20 against Cronobacter sakazakii-Induced Necrotizing Enterocolitis In Vitro and In Vivo" Nutrients 14, no. 18: 3827. https://doi.org/10.3390/nu14183827

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