Investigation of the early intestinal microflora in premature infants with/without necrotizing enterocolitis using two different methods (original) (raw)

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Necrotizing enterocolitis (NEC) is an acute inflammatory disease that affects the intestinal tracts of neonates (1); it is one of the most frequent gastrointestinal emergencies in premature neonates (2). The pathophysiology of NEC is multifactorial. A healthy intestine relies on perfect balance and interactions between the host epithelium, immune cells, and the microflora present. It is known that any abnormality in the ecosystem of the gastrointestinal tract may result in a pathological process potentially leading to NEC (3). It is suspected that abnormal colonization of the gastrointestinal tract or an unfavorable balance between commensal and pathogenic bacteria is part of the pathogenesis of NEC (4,5,6). It has been suggested that the ability of microflora to invade the epithelium and ferment unabsorbed nutrients (7), and the colonization by various bacterial pathogens in a sufficiently vulnerable host (8) could promote the development of NEC. Bacterial colonization of the neonatal gut is influenced by factors such as gestational age, feeding, medication, and diverse environmental flora (9). Premature neonates are exposed to the environmental flora present in the neonatal intensive care unit. Furthermore, they are often treated with broad-spectrum antibiotics and do not tolerate enteral feeds. It is likely that these circumstances promote bacterial colonization leading to NEC. The microflora in the premature intestine are characterized by decreased biodiversity (10) and imbalance, with overgrowth of potential pathogens. In this situation, mucosal lesions could give bacteria systemic access to the intestinal wall and contribute to the development of NEC.

Currently, there is a lack of detailed knowledge relating to the early bacterial colonization of the intestinal tracts of premature infants, and to the mechanisms underlying the establishment of intestinal microflora. The aim of this project was to determine the importance of bacterial flora in the development of NEC in premature infants. The bacterial flora were analyzed by fecal culture and DNA analysis in a large cohort of preterm infants during the first 4 weeks of life. Furthermore, the microflora from infants who developed NEC were compared with the flora of preterm infants who did not.

Results

A total of 192 premature infants, born at <30 weeks of gestation, were found to be eligible for this study. The parents of 165 of these infants were requested to consent to the enrolling of the infants in the study; in two cases, consent was declined. The premature neonates included in the study were born between 23 and 29 weeks of gestation. Of the 163 infants enrolled, 21 developed NEC during their hospital stay. Diagnosis was according to Bell’s criteria (14). The incidence of NEC had a strong inverse relationship with gestational age; the likelihood of developing NEC decreased by 8% (range 3.4, 13.2) for each additional day of gestational age. The characteristics of the infants are presented in Table 1 .

Table 1 Data on the premature population

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A total of 482 fecal samples were collected from the infants and subjected to culture and molecular methods for detection of bacteria. Between 1 and 3 fecal samples were collected from each of the infants during the first months of life, ranging from day 0 to day 96 after birth.

Detection of Fecal Bacteria in Culture

All fecal samples were subjected to culture, and all bacterial species isolated were identified by classical microbiological methods. The species of bacteria isolated are shown in Table 2 .

Table 2 Bacterial species detected in feces from premature neonates

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In the fecal samples from the neonates, very few bacterial species were detected, the predominant species being Staphylococcus spp., Enterococcus spp., Klebsiella spp., Escherichia coli, Clostridium spp., and Enterobacter spp., Yeast, Lactobacillus spp., and Bifidobacterium spp., were seldom, if ever, found.

On an assessment of the bacterial diversity of the fecal flora it was seen that neonates from whose feces fewer than three species of bacteria were grown in culture tended to be at increased risk of developing NEC (odds ratio 4.6 (95% confidence interval 0.98; 21.8)) ( Table 2 ).

Comparisons of the fecal microflora in the premature neonates showed that, overall, the intestines of those who did not develop NEC were colonized by a diversity of flora comprising both Gram-negative (G−) and Gram-positive (G+) bacterial species ( Table 2 ). In contrast, the premature neonates who developed NEC were generally those who were colonized predominantly by flora consisting of G+ bacteria.

Colonization by Staphylococcus spp. was significantly more prevalent in neonates who went on to develop NEC than in the control neonates who developed NEC (P = 0.004). It was striking that, ~1 month after birth (sample 3) the neonates who developed NEC continued to differ significantly from the control infants in respect to colonization by Staphylococcus spp. (P < 0.001). Certain G− bacterial species that are typically considered to be nosocomial pathogens were detected in the control infants. For instance, Klebsiella spp. were detected more frequently in control neonates than in the NEC neonates during the first month of life (for sample 1: P = 0.03; for sample 3: P = 0.003 ( Table 2 )).

Determination of Bacterial Diversity in Fecal Samples Using 16S rDNA PCR-DGGE

DNA was extracted from fecal samples, and 16S rDNA was amplified. The 16S rDNA denaturing gradient gel electrophoresis (DGGE) profile for each infant was unique. Bacterial diversity was assessed from the band richness of each sample. There were no differences in band richness between the profiles of neonates who developed NEC and those of the controls who did not develop NEC. This held true whether all the samples were considered together or sample 1, sample 2, or sample 3 were considered pairwise ( Table 3 ). Principal component analysis (PCA) was carried out, considering each DGGE profile to be the unique “fingerprint” of a particular neonate. PCA is a powerful multivariate technique that can extract patterns (i.e., certain combinations of bands/bacteria) related to children diagnosed with NEC and control children, provided these patterns are present in data. Using this approach it would be possible to evaluate whether certain combinations of bands are present in neonates with NEC but not in control neonates.

Table 3 Statistical analysis of culturing and PCR-DGGE from fecal samples

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Inspection of the score plots of the primary principal components showed no discriminating feature associated with any particular band position ( Figure 1 ), indicating that no specific bacterium or combination of bacteria were present in one patient group and absent in the other. This was validated using other multivariate techniques, and no patterns relating specifically to neonates with NEC could be found. The only apparent difference between the two patient groups was the number of bands, i.e., band richness. However, the mean band richness of all three samples (1–3) from a neonate or of each sample individually calculated, was not significantly correlated to development of NEC ( Table 3 ). Generally, all estimates were strengthened when analyzing the averages of all three samples.

Figure 1

Principal component analysis (PCA) plot based on denaturing gradient gel electrophoresis band profiles. (a) Data from all samples obtained during the first month of life; (b) PCA plot of sample 1 from all the infants, taken during 0–5 days after birth; (c) PCA plot of sample 2 from all the infants, taken 10 days after birth; and (d) PCA plot of sample 3 from all the infants taken 30 days after birth. Black dots represent fecal samples from control infants and red triangles represent fecal samples from infants who developed necrotizing enterocolitis.

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Also, there was no difference in the overall number of species as determined by culture, either when all samples were compared together or when matched samples (1, 2, or 3) were compared between the two patient groups (NEC vs. controls) ( Table 3 ).

Gender, gestation age, and feeding were treated as confounders in the analysis, and these had no association with the composition of the intestinal flora.

In the PCA analysis, we analyzed for antibiotic use as a confounder. However, because all the neonates received antibiotics at birth and/or subsequently for the treatment of sepsis, we could not register any influence of antibiotics on the colonization pattern.

Discussion

The advantages of culturing bacteria are obvious, given that the bacteria in question are isolated and available for further characterization. One of the limitations in using conventional microbiological methods is that only cultivable organisms are detected. Other limitations of the culture include the selection of bacterial growth depending on the culture media used, the stress imposed by culture procedures, and the necessity for strictly anoxic conditions. A range of selective and nonselective media were used. Culture bias can be caused by overgrowth of numerous species on the selective and nonselective plates. Molecular techniques are independent of these limitations; however, these techniques require good DNA quality and appropriate extraction methods. DGGE is a commonly used technique in molecular biology. The method is powerful and can rapidly provide a distribution pattern as an indication of population diversity. Because DGGE analysis requires significant amounts of DNA for detection, a PCR must be performed before the analysis. Therefore, all the troublesome features of sampling, DNA extraction, PCR primer design, and PCR conditions should be considered when troubleshooting DGGE problems. Problems at each stage of this molecular technique can impact negatively on each stage downstream. The main problem in practice is the PCR. In general, PCR-DGGE is found to be more sensitive than conventional culture, revealing numerous bands that indicate the presence of bacterial strains in addition to those that grow in culture.

Most studies on the composition of the gut microflora in neonates who go on to develop NEC have been carried out using traditional techniques of culture (11,12,13,14). Some studies have found an association between various bacterial species and NEC (15,16,17,18,19,20), whereas others did not observe any association between NEC and any specific bacterial species (8,21).

By carrying out culture of the fecal samples, we showed that the neonates who developed NEC were colonized predominately by G+ bacteria, whereas the control neonates were colonized by diverse bacterial flora comprising both G+ and G− bacterial species. In contrast, we found no association between the composition of fecal bacteria and development of NEC when we used molecular methods of analysis. These results are consistent with the findings of Millar et al. (22), who were the first to describe microflora using 16S rRNA gene PCR and DGGE in 32 premature neonates including 10 neonates with NEC. They found that, as compared with fecal samples from control neonates, samples from neonates who went on to develop NEC included many more kinds of bacteria that did not grow in culture. de la Cochetiere et al. (23), using the molecular technique of temperature gradient gel electrophoresis, detected a band corresponding to Clostridium perfringens in three cases of neonates with NEC but in none of the controls. In our study, no specific DNA bands were correlated with the development of NEC. Similarly, Mshvildadze et al. (20) found that the overall microbial profiles of samples from neonates with NEC were indistinguishable from those in control neonates.

In a comparison of DGGE profiles, there was no distinctive band associated with the development of NEC. There was a tendency for the simpler PCR-DGGE pattern for all the neonates at birth to become more diverse over time, but this was not a statistically significant trend. The increase in the bacterial complexity of the fecal samples during the first months after birth has previously been described, and these findings support the validity of our assays (24,25). Furthermore, our data indicate that each neonate has a unique band pattern, and that this pattern does not resemble any other neonate’s pattern during the time of the hospital stay as previously described (25). This could be because fecal samples were collected at distinct time points during the first 4 weeks of the neonate’s life rather than over a long period of time (such as 2 years). In this cohort study, as reported by others (24,26), DGGE profile analysis produced findings similar to those obtained from culture studies, confirming a lower biodiversity of bacteria in infants who go on to develop NEC.

It has been shown that there is a link between the presence of bacteria in amniotic fluid and the occurrence of preterm delivery. All the neonates included in this study were <30 weeks of gestation. However, bacteria frequently associated with preterm delivery, such as Mycoplasma hominis and Ureaplasma urealyticum (22), were not detected by culture techniques. Nevertheless, in the meconium, bacteria were detected both by culture and in the commensal PCR-DGGE.

Although we had a large population of premature neonates and a relatively large subpopulation who developed NEC, the statistical power of our study was nevertheless limited. Another difficulty was that each infant was found to host a particular pattern of fecal microflora (27), thereby defying simple statistical analysis. Finally, the interactions between abdominal symptoms, use of antibiotics, and fecal microflora are not likely to be simple. Some of the differences in fecal flora between cases with NEC and controls at 30 days of age may be a result of antibiotic treatment of NEC rather than part of the etiology. We did not attempt to disentangle these complexities because we predicted that the task would require a much larger study population.

We have recently shown, by in situ fluorescent hybridization laser capture microdissection and sequencing, a large variability in the bacteria in tissue specimens from neonates with NEC (28). Nevertheless, no potential pathogenic bacterial species, whether singly or in combination, was dominant in the samples, thereby serving to emphasize the complexity of the disease.

To date, our study is the largest one involved in analyzing the fecal flora of premature neonates during the first month of life. By culturing the bacteria in fecal samples, we showed that premature neonates who develop NEC are colonized predominately by G+ bacteria, in contrast to control neonates (who did not develop NEC), who were colonized by a significant diversity of microflora. Surprisingly, when we used molecular methods, we found no association between microflora profiles and subsequent development of NEC.

Methods

Patients and Sample Collection

Between September 2006 and January 2009, preterm neonates of <30 weeks of gestation were recruited from a single level III neonatal intensive care unit at Rigshospitalet, Copenhagen, Denmark. All the patients underwent routine neonatal intensive care unit care as determined by the managing service. Only neonates with definite or advanced NEC, corresponding to Bell stage II or III (29), were included in the NEC group. The study was approved by the ethical committee for Copenhagen and Frederiksberg, Denmark (KF 01 287895), and informed consent was obtained from the parents of the neonates.

Fecal samples from the infants were collected by nurses of the department. The samples were collected from the neonates’ diapers using sterile plastic spoons, and put in sterile plastic screw-cap tubes. The fecal samples were collected at the following time points: postnatal day 0–5 (sample 1), day 10 (sample 2), and day 30 (sample 3). The samples were stored at 4 °C and processed as soon as possible. When the samples were received at the microbiological laboratory at Statens Serum Institute, they were immediately processed. The samples were prepared for culture, while the remaining fecal material was mixed with 1 ml ox-broth and 10% vol/vol glycerol (SSI, Copenhagen, Denmark) and stored at −80 °C awaiting molecular analysis.

Identification of Neonatal Fecal Bacterial Flora From Culture

From each fecal sample,~200 mg was transferred 1 ml of sterile ultrapure water and mixed thoroughly. Samples were then plated on nonselective and selective media (SSI Diagnostica, Copenhagen, Denmark; see Table 4 ). Blood agar plates (5% horse blood) and chocolate agar plates were used for general culture; blue agar plates (modified Drigalski) were used for the detection of G− bacteria, especially Enterobacteriaceae; and sabouraud agar plates were used for selective growth of yeast/fungi. The plates were incubated aerobically at 37 °C for 24 h. Cycloserine cefoxitin fructose agar plates were used as selective media for the detection of Clostridium difficile, incubated anaerobically (5% CO2, 3%H2, 5%O2, and 87%N2 at 37 °C) for 48 h. All anaerobic microorganisms were tested for the absence of growth under aerobic conditions (for 2 days), and antimicrobial susceptibility was tested by disk diffusion of 5 µg metronidazole and 1 µg kanamycin (Oxoid, Hampshire, UK). Subsequently, microbial identification was carried out on the basis of their growth on selective media, characteristics of colonies, and cellular morphology. All identifications of bacteria were confirmed biochemically using the automated identification system VITEK 2 (Bio Mérieux, Nürtingen, Germany). Isolates from the anaerobic plate were preserved at −80 °C for future identification. Quantification of bacterial load was not performed. The microorganisms were identified primarily at the species level.

Table 4 Culture media used for microbiological analysis

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Extraction of Bacterial DNA From Fecal Samples

Bacterial DNA extraction from fecal material is critical; essentially, it was carried out using a method developed in our laboratory (30). For DNA extraction, 200 mg of the fecal sample was added to a 2 ml vial containing 1.4 ml of ASL buffer (stool lysis buffer; Qiagen, Hilden, Germany). To the sample, 0.3 g of zirconium beads (diameter, 0.1 mm; Biospec Product, Bartlesville, OK) was added, and disrupted at 30 Hz for 6 min by a TissueLyser system (Qiagen). DNA was extracted using the QIAamp DNA stool Mini Kit (Qiagen) in accordance with the instructions of the manufacturer. DNA was eluted in a final volume of 100 µl and stored at −20 °C until use.

PCR Amplification of Bacterial DNA

Aliquots (10 µl) of purified DNA were applied to the following to give a 50 µl PCR mixture: 4 µl of sterilized water, 20 µl of Eppendorf Mastermix (2.5×) (Eppendorf, Hamburg, Germany), and 8 µl of each of the universal primers HDA1-GC and HDA2 (31). PCR was run in a Peltier Thermal Cycler (MJ Research). Initial preheating was at 96 °C for 4 min, followed by 30 cycles of denaturation at 96 °C for 30 s, annealing at 56 °C for 30 s, replication at 68 °C for 1 min, and termination at 68 °C for 7 min.

Analysis of Fecal Microflora by DGGE

DGGE was carried out using the procedure described by Muyzer et al. (32), using a DCode Universal Maturation Detection System instrument and gradient former model 475 in accordance with the manufacturer’s instructions (Bio-Rad Labs, Hercules, CA). The denaturing gradient was formed with two 8% polyacrylamide gel (wt/vol, acrylamide/bisacrylamide, 37.5:1) stock solutions (Bio-Rad Labs) in 1 × TAE (20 mmol/l Tris, 10 mmol/l acetate, 0.5 EDTA, pH 7.4). The gels were made with denaturing gradient solution ranging from 30 to 65%. The 100% denaturant solution contained deionized formamide and 7 mol/l of urea. Before loading, 20 µl of the PCR product was mixed with 3 µl of 6× loading dye solution. Gels were run in 1× TAE at 60 °C for 16 h at 70 V, stained with GelRed (Biotium, Harvard, CA) for 35 min, and viewed by UV transillumination. The BioNumerics software, version 6.01 (Applied Maths, Sint-Martens-Latem, Belgium) was used for identification of bands and normalization of band patterns from DGGE gels.

Statistics

Statistical analyses were performed using SAS version 9.1.3 for Windows (SAS Institute, Cary, NC). A one-way analysis of variance by Fisher was used to evaluate the results obtained from culture. Bacteria were categorized as G+ and G− bacteria. All factors that showed a statistically significant correlation with simple linear regression were analyzed together in a stepwise linear regression. The factors selected for analysis as being possibly explanatory were gender, gestational age, birth weight, type of enteral feed (own mother’s milk, donated breast milk, formula), parenteral nutrition, and antibiotics administered.

Molecular data obtained by DGGE were represented as 0 (indicating the absence of a band) or 1 (indicating the presence of a band) and autoscaled (centered and scaled to unit variance for each variable) for PCA; the resultant PCA scores were plotted two-dimensionally. The PCA models were developed in LatentiX version 2.00 (Latent5, Copenhagen, Denmark).

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Acknowledgements

The authors thank all the clinical staff at the Neonatal Department, Rigshospitalet, Copenhagen, Denmark, for their help with obtaining the samples, and Berit Jensen for her valuable technical assistance with laboratory analyses. We would like to pay our respects to our late colleague S. Bodé, Neonatal Department, Rigshospitalet, Copenhagen, who was a driving force during this study.

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Author notes

1. Susan Bodé: Deceased

Authors and Affiliations

1. Department of Microbiological Surveillance and Research, Statens Serum Institut, Copenhagen, Denmark
   Birgitte Smith, Hengameh Mirsepasi & Karen A. Krogfelt
2. Department of Neonatology, Rigshospitalet, Copenhagen, Denmark
   Susan Bodé & Gorm Greisen
3. Department of Food Science, University of Copenhagen, Frederiksberg, Denmark
   Thomas H. Skov

Authors

1. Birgitte Smith
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2. Susan Bodé
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3. Thomas H. Skov
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4. Hengameh Mirsepasi
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5. Gorm Greisen
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6. Karen A. Krogfelt
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Correspondence toKaren A. Krogfelt.

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Smith, B., Bodé, S., Skov, T. et al. Investigation of the early intestinal microflora in premature infants with/without necrotizing enterocolitis using two different methods.Pediatr Res 71, 115–120 (2012). https://doi.org/10.1038/pr.2011.1

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• Received: 01 November 2010
• Accepted: 14 July 2011
• Published: 15 December 2011
• Issue Date: January 2012
• DOI: https://doi.org/10.1038/pr.2011.1