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  • Open Access

Dichotomous development of the gut microbiome in preterm infants

  • 1,
  • 1, 2,
  • 2,
  • 3, 4, 5,
  • 1,
  • 4, 5, 6 and
  • 1, 7Email author
Microbiome20186:157

https://doi.org/10.1186/s40168-018-0547-8

  • Received: 30 October 2017
  • Accepted: 3 September 2018
  • Published:

Abstract

Background

Preterm infants are at risk of developing intestinal dysbiosis with an increased proportion of Gammaproteobacteria. In this study, we sought the clinical determinants of the relative abundance of feces-associated Gammaproteobacteria in very low birth weight (VLBW) infants. Fecal microbiome was characterized at ≤ 2 weeks and during the 3rd and 4th weeks after birth, by 16S rRNA amplicon sequencing. Maternal and infant clinical characteristics were extracted from electronic medical records. Data were analyzed by linear mixed modeling and linear regression.

Results

Clinical data and fecal microbiome profiles of 45 VLBW infants (gestational age 27.9 ± 2.2 weeks; birth weight 1126 ± 208 g) were studied. Three stool samples were analyzed for each infant at mean postnatal ages of 9.9 ± 3, 20.7 ± 4.1, and 29.4 ± 4.9 days. The average relative abundance of Gammaproteobacteria was 42.5% (0–90%) at ≤ 2 weeks, 69.7% (29.9–86.9%) in the 3rd, and 75.5% (54.5–86%) in the 4th week (p < 0.001). Hierarchical and K-means clustering identified two distinct subgroups: cluster 1 started with comparatively low abundance that increased with time, whereas cluster 2 began with a greater abundance at ≤ 2 weeks (p < 0.001) that decreased over time. Both groups resembled each other by the 3rd week. Single variants of Klebsiella and Staphylococcus described variance in community structure between clusters and were shared between all infants, suggesting a common, hospital-derived source. Fecal Gammaproteobacteria was positively associated with vaginal delivery and antenatal steroids.

Conclusions

We detected a dichotomy in gut microbiome assembly in preterm infants: some preterm infants started with low relative gammaproteobacterial abundance in stool that increased as a function of postnatal age, whereas others began with and maintained high abundance. Vaginal birth and antenatal steroids were identified as predictors of Gammaproteobacteria abundance in the early (≤ 2 weeks) and later (3rd and 4th weeks) stool samples, respectively. These findings are important in understanding the development of the gut microbiome in premature infants.

Keywords

  • Very low birth weight infant
  • Gammaproteobacteria
  • Dysbiosis
  • Abbreviations
  • VLBWVery low birth weight
  • NECNecrotizing enterocolitis
  • OTUOperational taxonomic unit

Background

In newborn infants, the enteric microbiome is an important influence on mucosal immunity, nutrient absorption, and energy regulation in the developing intestine [1]. Healthy full-term neonates acquire a “core” enteric microbiome with the inocula received during and after birth from the maternal microbiota in the vaginal, fecal, and cutaneous compartments and from maternal milk [1, 2]. The gut microbiome in these infants shows dominance of Gram-positive Firmicutes such as Staphylococcus, Propionibacterium, Bifidobacterium, and Lactobacillus [2, 3]. However, in marked contrast to term infants, preterm infants are at risk of delayed and altered assembly of their intestinal microbiome [4, 5]. These patients have several clinical and physiological constraints, including absent or limited exposure to maternal microbiota due to shortened labor or cesarean birth, mucosal immaturity, and the lack of physical and immune defenses such as gastric acid, secretory IgA, and intestinal mucus, frequent multisystem organ dysfunction with consequent exposure to broad-spectrum antibiotics and various indwelling tubes and catheters, delays in enteral feeding, and intestinal dysmotility [3, 58]. Many premature infants show dysbiosis with a preponderance of Gram-negative bacteria of the class Gammaproteobacteria and its constituent families Enterobacteriaceae, Vibrionaceae, and Pseudomonadaceae [914]. There are concerns that such dysbiosis in preterm infants may be associated with adverse outcomes, including necrotizing enterocolitis, late-onset sepsis, and developmental delay [5, 10, 11, 15].

In this prospective observational study, we investigated the clinical antecedents of increased relative abundance of fecal Gammaproteobacteria in premature infants. Our goal was to identify the clinical characteristics of preterm infants who developed enteral dysbiosis, which in turn, could inform future efforts to direct microbiome screening in a clinical setting. We hypothesized that most premature infants begin with few Gammaproteobacteria in their stool and acquire these bacteria from the hospital microenvironment or from human interaction [1619], as a function of postnatal age. We reasoned that once introduced into the relatively uninhabited preterm intestine [20], the abundance of gammaproteobacterial taxa would expand with time. Therefore, we posited that (a) dysbiosis is a stable state wherein fecal Gammaproteobacteria would either increase in relative proportion or remain stable, but not decrease over time; and (b) Gammaproteobacteria-enriched dysbiosis may be seen in a majority of convalescing premature infants. To investigate these hypotheses, we recorded the demographic and clinical information from a cohort of inborn, very low birth weight (VLBW) infants and analyzed their fecal microbiome at serial time-points during the first month after birth.

Methods

Demographic and clinical information

This prospective study was performed after approval by Institutional Review Boards at University of South Florida and Tampa General Hospital (TGH). We enrolled all eligible VLBW infants admitted to the neonatal intensive care unit (NICU) at TGH, an academic regional referral center with a single-patient room floor plan, during the period May 2012–December 2013. Inclusion criteria included informed parental consent and the availability of a stool sample ≤ 2 weeks after birth. Infants with major congenital anomalies were excluded. The following maternal and neonatal information was obtained from medical records: maternal Hispanic ethnicity, maternal race (Black, White, Asian, and others), maternal age, duration of ruptured membranes, clinical chorioamnionitis, maternal hypertension, diabetes, and her body mass index; antenatal treatment with steroids and magnesium sulfate; mode of delivery, gestational age, birth weight, postnatal age, postmenstrual age (gestational age at birth + postnatal age, in weeks), gender, small-for-gestational age (SGA), singleton/multiple gestation, Apgar scores, admission temperature, early-onset or any sepsis (positive blood culture), respiratory distress syndrome, surfactant use, need for supplemental oxygen and/or positive pressure, patency of the ductus arteriosus, postnatal treatment with steroids or indomethacin/ibuprofen, days of antibiotic treatment during the first 2 weeks and the total number of days on antibiotics during the entire hospital stay, red blood cell transfusions, feeding (exclusive maternal/donor breast milk, exclusive formula, and mixed), NEC (Bell stages II or III [21]), chronic lung disease (need for supplemental oxygen at 36 weeks’ corrected gestational age), extra-uterine growth restriction, and the length of hospital stay.

Fecal DNA amplification

Stool samples obtained at ≤ 2 weeks, the 3rd week, and the 4th week after birth were stored at − 80°C under uniform conditions until analysis [22]. Total DNA from 100 to 250 mg stool (MoBio PowerFecal DNA kit, Qiagen, Carlsbad, CA) was used to amplify the V4 region of 16S rRNA gene using polymerase chain reaction with modified 515F and 806R primers [23, 24]. These DNA segments were sequenced using the MiSeq platform (Illumina, San Diego, CA) to generate about 15,000,250 base-pair paired-end reads per sample [24].

Statistical analysis

Demultiplexed DNA sequences were analyzed for bacterial identification to genus level using the CLC Biomedical Workbench 3.5.3 (Qiagen) using the default setting. Operational taxonomic units (OTUs) were assigned based on 97% sequence identity to the Greengenes v13.8 reference database, and their relative abundance (percentage) was computed. Bacterial diversity was measured within samples (alpha-diversity) as the number of OTUs, phylodiversity, and the Chao 1, Simpson, and Shannon indices; between samples (beta-diversity) by principal coordinate analysis and permutational multivariate analysis of variance (PERMANOVA) of weighted and unweighted UniFrac distance matrices, Jaccard coefficient, and the Bray-Curtis dissimilarity index. To improve upon the taxonomic resolution of the microbial analysis, we characterized OTUs to single nucleotide variants (SNVs) using Divisive Amplicon De-noising Algorithm 2 (DADA2) [25]. The V4 region 16S rRNA gene amplicon data was analyzed using the DADA2 pipeline. First, the demultiplexed fastq files were filtered and trimmed. Each sample was dereplicated, a portion of the data set was used to estimate the error parameters, and dada() was applied to the full pooled data set using those inferred error parameters. Paired reads were then merged, and removeBimeraDenovo() was used to remove chimeras. Taxonomy was assigned against the Greengenes v13.8 database (see Additional file 1 for Code for DADA2). Volatility analysis was performed by comparing unweighted UniFrac distances on SNVs between subgroups. To identify the predictive value of subgroups on microbiome community composition, we applied random forest machine learning (after rarefying to 5000 sequences/sample, 1000 trees) and Analysis of Composition of Microbiomes (ANCOM) [26]. Finally, to determine whether the data on relative abundance/proportions reflect a change in the absolute abundance of specific taxa, we performed Balance Tree Analysis using Gneiss [27].

Clinical information was analyzed using SPSS (IBM, Armonk, NY). Scalar variables were compared by the Mann-Whitney U [28] or Student’s t test [29], and categorical variables by Fisher’s exact test [30]. We used the linear mixed-effects modeling procedure [31] to identify determinants of fecal bacterial colonization. The linear mixed-effects procedure was performed using the maximum likelihood method. The autoregressive covariance matrix (with heterogeneous variances) was used as the dependent variables were anticipated to diverge with time. Best-fitting models were identified for lowest values of the − 2 log likelihood, Akaike’s information criterion, and Schwarz’s Bayesian criterion [32]. Important independent variables were shortlisted using bootstrap bagging [33], where a bootstrap dataset was constructed by not sampling a third of all subjects and replacing these by an equal number of duplicated samples. The bootstrap sample was analyzed by logistic regression with entry criterion of p < 0.2. The number of times a risk factor appeared in these 1000 analyses was taken as a reflection of the reliability. Because of the limited number of subjects in the study cohort and concern about model overfitting, multivariable analyses were limited to biologically plausible associations, to main effects for baseline measures, and time-dependent covariates for longitudinal measures. Models were adjusted for birth weight, gestation, and postmenstrual age. To ensure stability/reliability of estimates, 95% confidence intervals (CI) were re-estimated by bootstrapping (n = 1000). We also performed linear regression to identify the determinants of gammaproteobacterial abundance at each time-point of stool collection. Variables identified for the mixed-effects analysis were tested with entry at p < 0.2 and acceptance at p < 0.05, first using a one-step forced entry and then “stepwise” in the sequence of appearance during perinatal period [34]. To identify highly correlated variables, multicollinearity diagnostics (tolerance values < 0.2, variance inflation factors > 10) were reviewed [35]. The independence of variables was confirmed by the Durbin-Watson statistic (models accepted if between 1.5 and 2.5) [36]. Scatterplots of standardized residuals vs. standardized predicted values were evaluated for homoscedasticity and nonlinearity. Normality of residuals was confirmed by evaluation of histograms and normal probability plots. Statistical tests were two-tailed and considered significant at p < 0.05.

Results

Demographic and clinical information

We enrolled 45 eligible VLBW infants admitted to our NICU between May 2012 and December 2013. These infants were born at a gestation (mean ± standard deviation, SD) of 27.9 ± 2.2 weeks, with birth weight 1126 ± 208 g. Their clinical characteristics are summarized in Table 1.
Table 1

Perinatal and neonatal clinical characteristics

Characteristic

N = 45

Gestational age, weeks, (mean, SD)

28 (2)

Birth weight, grams, (mean, SD)

1126 (208)

Male

21 (46.7%)

Hispanic ethnicity

9 (20%)

Race

 Black

19 (42.2%)

 White

25 (55.6%)

Antenatal medications

 Steroids

39 (86.7%)

 Magnesium

34 (75.6%)

Vaginal birth

11 (24.4%)

Multiple birth

7 (15.6%)

Chorioamnionitis

26 (47.8%)

Maternal hypertension

13 (28.9%)

Small for gestational age

3 (6.7%)

Respiratory distress syndrome

26 (57.8%)

Oxygen on day 28

11 (24.4%)

Oxygen on day 36

2 (4.4%)

Patent ductus arteriosus

6 (13.3%)

Indomethacin

2 (4.4%)

Patent ductus arteriosus ligation

1 (2.2%)

Treated retinopathy of prematurity

0

Necrotizing enterocolitis

1 (2.2%)

Surgical necrotizing enterocolitis

1 (2.2%)

Days on antibiotics, (mean, SD)

4.5 (4.7)

Positive blood culture

5 (11.1%)

Packed red blood cell transfusion

16 (35.6%)

Feeding type

 Maternal breast milk only

25 (55.6%)

 Formula only

2 (4.4%)

 Mixed feeding types

18 (40.0%)

Discharge weight < 10th percentile

11 (24.4%)

Length of stay, days, (mean, SD)

68 (29)

Fecal microbiome

Three stool samples were analyzed from all infants, obtained at the postnatal age (mean ± SD) 9.9 ± 3, 20.7 ± 4.1, and 29.4 ± 4.9 days, respectively. The postmenstrual age at these time-points was 29.8 ± 2.3, 31.2 ± 1.9, and 32.6 ± 1.9 weeks, respectively. A total of 2,017,727 reads was obtained, with a mean 15,285 (± standard deviation 7139) sequences per sample. One of the stool samples at the first time-point had inadequate biomass for DNA sequencing and was excluded. The alpha-diversity metrics (number of OTUs, phylodiversity, and Shannon, Chao1, and Simpson indices) increased with postnatal age (see Additional file 2: Table S1).

Major bacterial communities in stool

Proteobacteria increased in abundance over time, comprising 46% (median; interquartile range/IQR = 0–90%) of all reads at ≤ 2 weeks, 83.5% (54.8–93.3%) in the 3rd and 77% (57–88.3%) in the 4th week (p < 0.001). The class Gammaproteobacteria dominated the Proteobacteria, comprising 42.5% (0–90%) at ≤ 2 weeks, 69.7% (29.9–86.9%) in the 3rd, and 75.5% (54.5–86%) in the 4th week (p < 0.001) (Fig. 1, Additional file 2: Table S2). Gammaproteobacteria comprised > 50% reads in 20/44 (45.5%) infants at ≤ 2 weeks, 29/45 (64.4%) in the 3rd week, and 36/45 (80%) in the 4th week. Klebsiella were the predominant gammaproteobacterial genus, dominating nearly all infants (median 44%, range 0–100% at ≤ 2 weeks, 85% (0–99%) in the 3rd, and 78.5% (0–99%) in the 4th week (changes not significant because of high inter-infant variability). A SNV mapping to Klebsiella comprised 0.18% of all reads (median, range 0–99.4%) at ≤ 2 weeks, 24.6% (0–99.5%) in the 3rd (p = 0.034), and 26.2% (0–99.4%) in the 4th week (not significant vs. ≤ 2 week samples). Identified gammaproteobacterial genera are listed in Additional file 2: Table S3.
Fig. 1
Fig. 1

Relative abundance of major bacterial taxonomic units in stool over time. Line diagrams (means ± standard deviation) show the relative abundances of major bacterial taxonomic units in stool, by cluster. Stool samples were collected during the first 2 weeks, and then during the 3rd and the 4th weeks, respectively. Repeated measures analysis of variance; *p < 0.05, **p < 0.01, and ***p < 0.001

Firmicutes were the second most abundant phylum at ≤ 2 weeks (median 41.5%, IQR 3.25–100%). The class Bacilli accounted for nearly all Firmicutes at ≤ 2 weeks (100%, IQR 60–100%), whereas Clostridia were dominant during the 4th week (42%, IQR 8.5–85%; p < 0.001). At the genus level, Staphylococcus were abundant at ≤ 2 weeks and decreased with age, whereas Enterococcus increased over time. Lactobacillus were scant. Other Firmicute genera are presented in Additional file 2: Table S4. Actinobacteria and Bacteroidetes were nearly absent from this cohort (see Additional file 2: Table S2).

Cluster analysis for fecal abundance of Gammaproteobacteria

The relative abundance of Gammaproteobacteria in ≤ 2 week samples varied widely (0–90%; see Additional file 2: Table S2). Therefore, we looked for evidence of clustering in our cohort. Hierarchical and K-means clustering [37] of Gammaproteobacteria percentages in the 44 first time-point stool samples showed 2 subgroups (Fig. 2a, b): cluster 1 (20 infants) started with low gammaproteobacterial abundance (mean ± SD 2.09 ± 5.91%, median 0, range 0–25%), whereas cluster 2 (24 infants) showed greater gammaproteobacterial relative abundance (mean ± SD 79.18 ± 21.6%, median 84.5%, range 31.36–99%; p < 0.001). Cluster 1 infants had lower birth weight (mean ± SD 1053 ± 227 g vs. 1176 ± 175 g in cluster 2; p = 0.049) and were less likely to have had a vaginal birth (1/20 in cluster 1 vs. 10/24 in cluster 2, p = 0.006). Their clinical characteristics are summarized in Additional file 2: Table S5, and the OTUs in Additional file 2: Table S6 a–c. Multiple birth participants sorted to the same cluster as their siblings, indicating the validity of this grouping. Random forest analysis predicted cluster identity with a prediction/error ratio of 2.2, but did not identify any SNVs with a large feature importance score (see Additional file 2: Table S7).
Fig. 2
Fig. 2

Clustering of VLBW infants by the relative abundance of fecal Gammaproteobacteria. a Dendrogram shows the average linkage (between the two groups) derived by hierarchical clustering. b. Scatter-plot shows that the VLBW infants included in our study were grouped into two distinct clusters based on the relative abundance of Gammaproteobacteria (percentages) in stool samples obtained during the first two postnatal weeks

Cluster 1 gained Gammaproteobacteria over time (p < 0.001, 3rd and 4th weeks compared to ≤ 2 week samples), whereas cluster 2 showed a transient drop in Gammaproteobacteria in the 3rd week before a 4th week rebound (p = 0.042; Fig. 3; in Additional file 2: Table S6 a–c). In cluster 2, Klebsiella was the most abundant genus (median 96%, range 0–99%; detected in 19/24 infants), and one particular SNV was dominant (60.8%, 0–99.4%). During the 3rd and the 4th weeks, both clusters showed increasing alpha-diversity and comparable Gammaproteobacteria relative abundance (Additional file 2: Tables S6b, c and S8a, b). Beta-diversity comparisons showed greater between-sample diversity in cluster 2 at ≤ 2 weeks, but these differences narrowed over time (Additional file 2: Table S8c). Volatility analysis confirmed a significant difference in variability in unweighted UniFrac distances between the clusters (p = 0.038; Fig. 4) (Additional file 3).
Fig. 3
Fig. 3

Relative abundance of major bacterial taxonomic units in stool, by cluster. Line diagrams (means ± standard deviation) show the relative abundances of major bacterial taxonomic units in stool in clusters 1 and 2. Stool samples were collected during the first 2 weeks, and then during the 3rd and the 4th weeks, respectively. Repeated measures analysis of variance; *p < 0.05, **p < 0.01, and ***p < 0.001

Fig. 4
Fig. 4

Volatility analysis of the two clusters: Histogram shows the distribution of unweighted UniFrac distances between successive time-points. A distance of 1 means maximally different communities, while a distance of 0 implies identical communities, so a curve shifted toward 0 means lower variability between successive time-points. The two clusters showed a significant difference in variability (p = 0.038)

ANCOM was performed to identify single nucleotide variant (SNV) sequences that described the variance in the microbiome community differences between clusters 1 and 2. A single variant of Klebsiella and a variant of Staphylococcus showed significantly different relative abundance between the two clusters (p < 0.05; after false discovery rate correction). This same Staphylococcus SNV also had a significantly different relative abundance between the three time-points (p < 0.001) and decreased over time. No SNVs were significantly different between individual infants. The heat map of the most abundant SNVs in the cohort is shown in Fig. 5.
Fig. 5
Fig. 5

Heat map of the most abundant single nucleotide variants (SNVs): Heat map shows the relative abundance of the 18 most abundant SNVs at each sample. The bar at the top is color coded according to time-point. Blue = most abundant, yellow = least abundant (minimum abundance displayed = 0.165% mean abundance across samples)

Data on relative abundance/proportions does not inform whether specific taxa have grown or decreased in absolute abundance. We performed Balance Tree analysis, which uses the concept of balances to account for the compositional nature of 16S rRNA data. We calculated a bifurcating tree relating the DADA2 sequence variants to each other by time-point (stool number) to determine if certain sequence variants appeared only in early or late stages. We then performed linear regression by cluster membership, which confirmed that cluster 2 showed increased Klebsiella (Fig. 6).
Fig. 6
Fig. 6

Balance tree analysis for major bacterial taxa. Bifurcating tree relating the DADA2 sequence variants to each other by the time-point for stool collection highlights specific sequence variants that appeared only in early or late stages. Linear regression by cluster membership confirmed increased Klebsiella in cluster 2. Cluster 1 showed a true increase in Staphylococcus sequence variant

Clinical antecedents of fecal colonization with Gammaproteobacteria

We performed mixed-effects modeling to identify the clinical determinants of the relative abundance of fecal Gammaproteobacteria. Small-for-gestational age (SGA), ethnicity, vaginal birth, antenatal steroids, magnesium sulfate, chorioamnionitis, gender, multiple births, postnatal age, enteral feedings, RDS, PDA, sepsis, and transfusions were defined as fixed effects. Maternal BMI, birth weight, gestation, postmenstrual age at stool collection, duration of ruptured membranes, antibiotic treatment, and the total length of hospital stay were defined as random effects. The best-fitting, parsimonious model (Table 2) showed positive associations of fecal Gammaproteobacteria with vaginal birth (F = 9.55, p = 0.002) and antenatal steroids (F = 4.23, p = 0.042). There was also a borderline, negative effect of maternal magnesium sulfate therapy (F = 3.87, p = 0.051). There was no effect of gestational or postmenstrual age. When we used Klebsiella as the dependent variable, the associations with vaginal birth (F = 10.91, p = 0.001) and antenatal steroids (F = 7.29, p = 0.008) remained consistent.
Table 2

Linear mixed-effects model for the relative fecal abundance of Gammaproteobacteria

Parameter

Estimate

Std. error

p value

95% CI

Bootstrapping 95% CI

Lower

Upper

Lower

Upper

Intercept

24.06

22.35

0.284

− 20.19

68.32

− 21.98

345.46

Absence of SGA status

1.90

13.28

0.887

− 24.40

28.19

− 72.52

23.13

Cesarean birth

− 23.63

7.65

0.002

− 38.77

− 8.49

− 40.33

− 4.88

Absence of Latino ethnicity

6.86

7.67

0.373

− 8.32

22.04

− 7.73

32.45

Absence of antenatal steroids

− 23.57

11.47

0.042

− 46.28

− 0.87

− 46.27

14.82

Absence of antenatal magnesium sulfate therapy

15.38

7.81

0.051

− 0.09

30.85

− 12.83

33.13

Absence of chorioamnionitis

8.41

6.70

0.212

− 4.85

21.67

− 7.79

25.40

Time

2.71

1.70

0.115

− 0.67

6.08

− 7.67

6.17

* Significant p-values (<0.05) are shown in italics

We next performed linear regression to identify the determinants of Gammaproteobacteria relative abundance at the three time-points of stool collection. At ≤ 2 weeks, Gammaproteobacteria abundance was associated with vaginal birth, Latino ethnicity, postnatal age, and the number of antibiotic days (r2 = 0.69, F = 5.66, p < 0.001; see Additional file 2: Table S13). When individual antibiotics were included, gentamicin (b = 15.03, SE 5.35, p = 0.009), but not ampicillin, showed a significant effect. The regression models were less robust during the 3rd week (r2 = 0.34, F = 3.02, p = 0.026), but postnatal age and antenatal steroids continued to show significant effects (see Additional file 2: Table S14). The 4th-week regression models were a better fit (r2 = 0.68, F = 4.26, p = 0.001) and showed positive effects of postnatal age, antenatal steroids, respiratory distress syndrome (RDS), and red cell transfusions, and negative effects of magnesium sulfate, admission temperature, and total antibiotic days. Individual antibiotics did not show a significant effect. There was a borderline, positive effect of human milk feedings (p = 0.055; see Additional file 2: Table S15).

In cluster 1, mixed modeling showed increased Gammaproteobacteria with postnatal age (p = 0.002). Cluster 2 showed increased Gammaproteobacteria with vaginal birth (p = 0.019) and antenatal steroids (p = 0.001), and negative associations with small-for-gestational-age status (SGA) (p < 0.001), Latino ethnicity (p = 0.009), and chorioamnionitis (p = 0.016; Tables 3 and 4). Regression analysis in cluster 1 at ≤ 2 weeks (r2 = 0.87, F = 8.88, p = 0.004) showed increased Gammaproteobacteria with human milk feedings. In cluster 2, patent ductus arteriosus (PDA) had a negative effect (Additional file 2: Table S9a, b).
Table 3

Linear mixed-effects model for the relative fecal abundance of Gammaproteobacteria in cluster 1

Parameter

Estimate

Std. error

p value

95% CI

Lower

Upper

Intercept

− 71.41

44.94

0.118

− 161.47

18.65

Absence of SGA status

− 14.95

30.96

0.631

− 76.99

47.08

Cesarean birth

3.24

21.84

0.883

− 40.53

47.00

Absence of Latino ethnicity

34.19

10.82

0.003

12.50

55.89

Absence of antenatal steroids

− 20.38

17.39

0.246

− 55.24

14.47

Absence of antenatal magnesium sulfate therapy

4.56

16.41

0.782

− 28.34

37.45

Absence of chorioamnionitis

5.18

8.50

0.545

− 11.85

22.20

Postnatal age

7.25

2.23

0.002

2.78

11.72

* Significant p-values (<0.05) are shown in italics

Table 4

Linear mixed-effects model for the relative fecal abundance of Gammaproteobacteria in cluster 2

Parameter

Estimate

Std. error

p value

95% CI

Lower

Upper

Intercept

885.64

111.30

0.000

667.49

1103.78

Absence of SGA status

− 123.76

20.12

0.000

− 163.21

− 84.31

Cesarean birth

− 18.48

7.89

0.019

− 33.95

− 3.02

Absence of Latino ethnicity

29.33

11.18

0.009

7.36

51.29

Absence of antenatal steroids

− 51.94

14.89

0.001

− 81.17

− 22.71

Absence of antenatal magnesium sulfate therapy

− 1.12

8.05

0.889

− 17.09

14.84

Absence of chorioamnionitis

22.26

9.26

0.016

4.09

40.43

Postnatal age

− 7.76

1.74

0.000

− 11.17

− 4.35

* Significant p-values (<0.05) are shown in italics

Clinical determinants of the relative proportions of other bacterial phyla

Fecal Firmicutes were positively associated with cesarean birth (F = 21.49, p < 0.001) and negatively with postnatal age (F = 5.08, p = 0.026). We attempted, but did not find evidence of clear clustering of subjects based on the relative abundance of Firmicutes, Bacilli, or Clostridia. Comparison of clusters based on Gammaproteobacteria abundance (as described in preceding sections) showed interesting differences in the relative abundance of Firmicutes. Cluster 1 carried more Firmicutes and Bacilli than cluster 2 in the earliest (≤ 2 weeks) and 3rd week stool samples (Additional file 2: Table 6a–c and S10a). In cluster 1, Firmicutes were associated positively with Latino ethnicity and negatively with postnatal age (Additional file 2: Table S10b). Bacilli decreased with postnatal age in cluster 2 (Fig. 5 and Additional file 2: Table S11a–c). Staphylococcus was dominant in cluster 1 at ≤ 2 weeks (median 100%, range 2–100%; detected in all infants). Most mapped to one particular SNV (median abundance 98% of all Staphylococcus, range 1.8–100%), which was confirmed in Balance Tree analysis (Fig. 6). Clostridia increased with postnatal age (F = 8.81, p = 0.004), particularly in cluster 2 (Additional file 2: Table S12a–c).

Discussion

We present a detailed analysis of the clinical determinants of the proportion of Gammaproteobacteria in the stool of preterm infants. Consistent with our hypothesis, the overall proportion of Gammaproteobacteria increased in stool with postnatal age. However, we noted two distinct patterns: one group started with a low relative abundance of Gammaproteobacteria in early stool samples (≤ 2 weeks) that increased with time, whereas a second group of infants started with a high relative abundance of Gammaproteobacteria that dipped transiently during the 3rd week. By the 4th week, the two groups had similar levels of Gammaproteobacteria. To our knowledge, this is the first study to describe this dichotomy in gut microbiome assembly in premature infants.

The development of the preterm gut microbiome is an area of intense scientific scrutiny. Currently, there are two conceptual models: in the first [38], the microbiome is believed to develop in a non-random, patterned progression where host maturation is important and environmental factors have only a minimal, non-enduring influence on the gut microbiome. In the 2nd model, the environment is key: factors such as the hospital microflora, diet, and antibiotics are believed to fundamentally alter gut microbiome assembly [2, 3942]. Our findings suggest that both models have merit. Cluster 1 showed the sequential dominance of Bacilli, Gammaproteobacteria, and Clostridia in stool samples collected during the first 2, the 3rd, and the 4th weeks, respectively. These findings were consistent with those of La Rosa et al. [38], except that we did not find effects of gestational or postmenstrual age. These infants began life with a low relative abundance of Gammaproteobacteria but showed greater variability between time-points in our volatility analysis. The low alpha-diversity and high beta-diversity in cluster 1 may be interpreted as a gammaproteobacterial bloom during their NICU stay that transiently crowded out other members of a microbial community. These findings differ from those in cluster 2, who showed high relative abundance of fecal Gammaproteobacteria from the earliest stool sample. The identification of vaginal birth as the leading determinant of stool-associated Gammaproteobacteria in this group suggests that vertical, mother-to-infant transmission of Gammaproteobacteria may contribute to intestinal dysbiosis in some preterm infants. This information is important for clinical practice improvement and infection control measures. In preterm infants, early colonization with Gammaproteobacteria has been generally associated with horizontal transmission of these bacteria in the NICU and selection pressures from antibiotics and diet. However, the possibility of vertical transmission in some infants is novel and indicates a need for additional preventive strategies starting before and during birth.

The dominance of a single variant of Klebsiella in cluster 2 infants indicates a common, possibly hospital-derived, source. Women with high-risk pregnancies are often exposed repeatedly to the hospital environment while being monitored/treated for pregnancy complications and are at risk of becoming colonized with hospital microflora. In our cohort, 25/43 (58%) mothers had received inpatient care for ≥ 3 hospital days and 22/43 (51%) had ≥ 2 hospital visits before delivery, mostly for actual or imminent preterm labor. We speculate that cluster 2 infants, who were more likely to have had a vaginal birth, may have received a larger inoculum of Gammaproteobacteria/Klebsiella than cluster 1 because of the exposure to maternal microflora in the vaginal, fecal, and cutaneous compartments. We are unable to investigate these possibilities further as we did not collect maternal and hospital environmental samples in the present study. During pregnancy, the vaginal microbiome is dominated by Firmicutes [43, 44]. In women with vaginal dysbiosis, pathobionts such as Prevotella, Sneathia, Atopobium, Mycoplasma, and Gardnerella can be identified [43, 44], but Gammaproteobacteria are infrequent [45]. The putative microbiome of the placenta and the amniotic fluid includes Gammaproteobacteria [46] and could be a plausible source, but this should affect all infants, regardless of delivery mode. Other potential sources may include exposure to maternal enteric flora during vaginal birth and then to the microbiome of human milk, both of which contain Gammaproteobacteria and often Klebsiella in particular [47, 48].

The identification of postnatal age as a determinant of Gammaproteobacteria abundance was consistent with the acquisition of these bacteria from care providers and the hospital environment. However, the transient drop in fecal Gammaproteobacteria we observed in cluster 2 infants during the 3rd postnatal week was contrary to our hypothesis that once established in the relatively uninhabited preterm intestine [49], Gammaproteobacteria would either increase or remain stable, but not decrease, over time. These findings need to be confirmed with quantitative measurements of Gammaproteobacteria abundance, but if validated, would have important implications for evaluating dysbiosis as a predictor of adverse outcomes in VLBW infants [11] as the best timing for measuring Gammaproteobacteria abundance will need to be ascertained.

The association of Latino ethnicity with fecal Gammaproteobacteria may be rooted in genetic factors [50], although there may have been a confounding influence of the type of feedings: 8/9 (88.8%) Latino infants received only human milk vs. 17/36 (47.2%) infants of other ethnic groups (p = 0.03). The association of fecal Gammaproteobacteria with antenatal steroids, magnesium sulfate, and the admission temperature is also not easily explained. Interestingly, the effect of antenatal steroids was delayed, seen only in the later stool samples (from the 3rd and 4th weeks). Steroids could alter the host-microbial cross-talk by dampening leukocyte activation and cytokine expression [5154] or via epigenetic changes in the mucosa [55]. Perinatal exposure to magnesium sulfate alters gut motility and some immune responses [56, 57], but the effects on fecal microbiome need further study. Human milk feedings increased fecal Gammaproteobacteria at ≤ 2 weeks, but had a negative effect later. The early effects may be related to milk-borne Gammaproteobacteria [47], possibly selected under the influence of other factors such as antibiotics. Later, negative effects may reflect the benefits of milk prebiotics [58], but the high prevalence of dysbiosis in our cohort indicates that such protection, at least in hospitalized infants, may be modest. Antibiotics, and gentamicin in particular, were associated with increased Gammaproteobacteria during the early neonatal period, but in the 4th week, antibiotic days had a negative effect. Antibiotics do create an environment that promotes the abundance of Gammaproteobacteria [59], but it is unclear why these effects should change with postnatal age.

The strengths of our study are its prospective design, availability of clinical and laboratory data, and repeated measurements of the gut microbiome. The dataset comes from a NICU with a single-patient room floor plan, which is now the favored NICU design and should be representative of most centers in the USA. Emerging data indicate that the floor plan (patient pods vs. single-patient rooms) may be an important determinant of horizontal microbial spread in the NICU [60]. Our study is constrained by its limited sample size and single study site. In addition, the low incidence of NEC in our cohort is a limitation that prevented us from using NEC as a measured outcome. Our findings of high Gammaproteobacteria abundance in some infants within the first 2 weeks also indicate an opportunity to confirm these findings in meconium, which should contain the original, “at birth” microbiome. Finally, the detection of dysbiosis with predominance of a few bacterial communities does not imply pathogenicity, but needs further evaluation at higher levels of resolution.

Conclusions

We noted a dichotomous pattern of fecal colonization with Gammaproteobacteria in our cohort of preterm infants; some started with low relative abundance of Gammaproteobacteria and acquired those as a function of postnatal age, whereas others carried these bacteria in high abundance since the early postnatal period. The predominance of a single variant of Klebsiella indicated a common, possibly hospital-derived, source. Vaginal birth and antenatal steroids were identified as major determinants of stool-associated Gammaproteobacteria, indicating that vertical, mother-to-infant transmission of Gammaproteobacteria may contribute to intestinal dysbiosis in some infants.

Declarations

Acknowledgements

This research was funded by the National Institutes of Health awards NR015446 (MG), HL124078 (AM), HL133022 (AM), and T32GM007281 (ALY).

The authors thank the research nurses, Judy Zaritt and Marcia Kneusel, for identification of eligible infants, and collection of clinical information and stool samples. We are also indebted to their constant support.

Availability of data and materials

The datasets generated during and/or analyzed during the current study are available at https://www.ncbi.nlm.nih.gov/Traces/study/?acc=SRP136661

Authors’ contributions

TTBH collected and analyzed the data and wrote the manuscript. MWG supervised the laboratory process and advised on content of the manuscript. BK performed the laboratory analysis and advised on the laboratory techniques. ALY analyzed the 16S rRNA data. BAT advised on the content of the manuscript. JAG supervised the analysis of 16S rRNA data and advised on the manuscript content. AM supervised the data analysis and wrote the manuscript. All authors edited the manuscript and approved the final draft.

Ethics approval and consent to participate

The study was approved by the Institutional Review Boards at University of South Florida and Tampa General Hospital, Florida. An informed written consent was obtained for all participating infants prior to the sample and data collections.

Competing interests

The authors declare that they have no competing interests.

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Authors’ Affiliations

(1)
Department of Pediatrics, Morsani College of Medicine, University of South Florida, Tampa, FL, USA
(2)
College of Nursing, University of South Florida, Tampa, FL, USA
(3)
Interdisciplinary Scientist Training Program, University of Chicago, Chicago, IL, USA
(4)
Microbiome Center, University of Chicago, Chicago, IL, USA
(5)
Department of Surgery, University of Chicago, Chicago, IL, USA
(6)
Argonne National Laboratory, Chicago, IL, USA
(7)
Department of Pediatrics, Johns Hopkins University, 1800 Orleans St, JHCC 8530, Baltimore, MD 21287, USA

References

  1. Turnbaugh PJ, Hamady M, Yatsunenko T, Cantarel BL, Duncan A, Ley RE, Sogin ML, Jones WJ, Roe BA, Affourtit JP, et al. A core gut microbiome in obese and lean twins. Nature. 2009;457(7228):480–4.View ArticlePubMedGoogle Scholar
  2. Palmer C, Bik EM, DiGiulio DB, Relman DA, Brown PO. Development of the human infant intestinal microbiota. PLoS Biol. 2007;5(7):e177.View ArticlePubMedPubMed CentralGoogle Scholar
  3. Penders J, Thijs C, Vink C, Stelma FF, Snijders B, Kummeling I, van den Brandt PA, Stobberingh EE. Factors influencing the composition of the intestinal microbiota in early infancy. Pediatrics. 2006;118(2):511–21.View ArticlePubMedGoogle Scholar
  4. Groer MW, Luciano AA, Dishaw LJ, Ashmeade TL, Miller E, Gilbert JA. Development of the preterm infant gut microbiome: a research priority. Microbiome. 2014;2:38.View ArticlePubMedPubMed CentralGoogle Scholar
  5. Stewart CJ, Embleton ND, Marrs ECL, Smith DP, Fofanova T, Nelson A, Skeath T, Perry JD, Petrosino JF, Berrington JE, et al. Longitudinal development of the gut microbiome and metabolome in preterm neonates with late onset sepsis and healthy controls. Microbiome. 2017;5(1):75.View ArticlePubMedPubMed CentralGoogle Scholar
  6. Biasucci G, Rubini M, Riboni S, Morelli L, Bessi E, Retetangos C. Mode of delivery affects the bacterial community in the newborn gut. Early Hum Dev. 2010;86(Suppl 1):13–5.View ArticlePubMedGoogle Scholar
  7. Fricke WF. The more the merrier? Reduced fecal microbiota diversity in preterm infants treated with antibiotics. J Pediatr. 2014;165(1):8–10.View ArticlePubMedGoogle Scholar
  8. Gasparrini AJ, Crofts TS, Gibson MK, Tarr PI, Warner BB, Dantas G. Antibiotic perturbation of the preterm infant gut microbiome and resistome. Gut Microbes. 2016;7(5):443–9.View ArticlePubMedPubMed CentralGoogle Scholar
  9. Wang Y, Hoenig JD, Malin KJ, Qamar S, Petrof EO, Sun J, Antonopoulos DA, Chang EB, Claud EC. 16S rRNA gene-based analysis of fecal microbiota from preterm infants with and without necrotizing enterocolitis. ISME J. 2009;3(8):944–54.View ArticlePubMedPubMed CentralGoogle Scholar
  10. Warner BB, Deych E, Zhou Y, Hall-Moore C, Weinstock GM, Sodergren E, Shaikh N, Hoffmann JA, Linneman LA, Hamvas A, et al. Gut bacteria dysbiosis and necrotising enterocolitis in very low birthweight infants: a prospective case-control study. Lancet. 2016;387:1928–36.View ArticlePubMedPubMed CentralGoogle Scholar
  11. Pammi M, Cope J, Tarr PI, Warner BB, Morrow AL, Mai V, Gregory KE, Kroll JS, McMurtry V, Ferris MJ, et al. Intestinal dysbiosis in preterm infants preceding necrotizing enterocolitis: a systematic review and meta-analysis. Microbiome. 2017;5(1):31.View ArticlePubMedPubMed CentralGoogle Scholar
  12. Torrazza RM, Ukhanova M, Wang X, Sharma R, Hudak ML, Neu J, Mai V. Intestinal microbial ecology and environmental factors affecting necrotizing enterocolitis. PLoS One. 2013;8(12):e83304.View ArticlePubMedPubMed CentralGoogle Scholar
  13. Morrow AL, Lagomarcino AJ, Schibler KR, Taft DH, Yu Z, Wang B, Altaye M, Wagner M, Gevers D, Ward DV, et al. Early microbial and metabolomic signatures predict later onset of necrotizing enterocolitis in preterm infants. Microbiome. 2013;1(1):13.View ArticlePubMedPubMed CentralGoogle Scholar
  14. Zhou Y, Shan G, Sodergren E, Weinstock G, Walker WA, Gregory KE. Longitudinal analysis of the premature infant intestinal microbiome prior to necrotizing enterocolitis: a case-control study. PLoS One. 2015;10(3):e0118632.View ArticlePubMedPubMed CentralGoogle Scholar
  15. Goyal MS, Venkatesh S, Milbrandt J, Gordon JI, Raichle ME. Feeding the brain and nurturing the mind: linking nutrition and the gut microbiota to brain development. Proc Natl Acad Sci U S A. 2015;112(46):14105–12.View ArticlePubMedPubMed CentralGoogle Scholar
  16. Gibson MK, Wang B, Ahmadi S, Burnham CA, Tarr PI, Warner BB, Dantas G. Developmental dynamics of the preterm infant gut microbiota and antibiotic resistome. Nat Microbiol. 2016;1:16024.View ArticlePubMedPubMed CentralGoogle Scholar
  17. Raveh-Sadka T, Thomas BC, Singh A, Firek B, Brooks B, Castelle CJ, Sharon I, Baker R, Good M, Morowitz MJ, et al. Gut bacteria are rarely shared by co-hospitalized premature infants, regardless of necrotizing enterocolitis development. Elife. 2015;4. https://www.ncbi.nlm.nih.gov/pmc/articles/PMC4384745/.
  18. Morowitz MJ, Denef VJ, Costello EK, Thomas BC, Poroyko V, Relman DA, Banfield JF. Strain-resolved community genomic analysis of gut microbial colonization in a premature infant. Proc Natl Acad Sci U S A. 2011;108(3):1128–33.View ArticlePubMedGoogle Scholar
  19. Brooks B, Firek BA, Miller CS, Sharon I, Thomas BC, Baker R, Morowitz MJ, Banfield JF. Microbes in the neonatal intensive care unit resemble those found in the gut of premature infants. Microbiome. 2014;2(1):1.View ArticlePubMedPubMed CentralGoogle Scholar
  20. Ley RE, Peterson DA, Gordon JI. Ecological and evolutionary forces shaping microbial diversity in the human intestine. Cell. 2006;124(4):837–48.View ArticlePubMedGoogle Scholar
  21. Walsh MC, Kliegman RM. Necrotizing enterocolitis: treatment based on staging criteria. Pediatr Clin N Am. 1986;33(1):179–201.View ArticleGoogle Scholar
  22. Moore HM, Kelly A, McShane LM, Vaught J. Biospecimen reporting for improved study quality (BRISQ). Transfusion. 2013;53(7):e1.View ArticlePubMedGoogle Scholar
  23. Walters W, Hyde ER, Berg-Lyons D, Ackermann G, Humphrey G, Parada A, Gilbert JA, Jansson JK, Caporaso JG, Fuhrman JA, et al. Improved bacterial 16S rRNA gene (V4 and V4-5) and fungal internal transcribed spacer marker gene primers for microbial community surveys. mSystems. 2016;1(1). https://msystems.asm.org/content/1/1/e00009-15.
  24. Caporaso JG, Lauber CL, Walters WA, Berg-Lyons D, Huntley J, Fierer N, Owens SM, Betley J, Fraser L, Bauer M, et al. Ultra-high-throughput microbial community analysis on the Illumina HiSeq and MiSeq platforms. ISME J. 2012;6(8):1621–4.View ArticlePubMedPubMed CentralGoogle Scholar
  25. Callahan BJ, McMurdie PJ, Rosen MJ, Han AW, Johnson AJ, Holmes SP. DADA2: high-resolution sample inference from Illumina amplicon data. Nat Methods. 2016;13(7):581–3.View ArticlePubMedPubMed CentralGoogle Scholar
  26. Mandal S, Van Treuren W, White RA, Eggesbo M, Knight R, Peddada SD. Analysis of composition of microbiomes: a novel method for studying microbial composition. Microb Ecol Health Dis. 2015;26:27663.PubMedGoogle Scholar
  27. Morton JT, Sanders J, Quinn RA, McDonald D, Gonzalez A, Vazquez-Baeza Y, Navas-Molina JA, Song SJ, Metcalf JL, Hyde ER, et al. Balance trees reveal microbial niche differentiation. mSystems. 2017;2(1). https://msystems.asm.org/content/2/1/e00162-16.
  28. Mann HB, Whitney DR. On a test of whether one of two random variables is stochastically larger than the other. Ann Math Statist. 1947;18(1):50–60.View ArticleGoogle Scholar
  29. Student. The probable error of a mean. Biometrika. 1908;6:1–25.View ArticleGoogle Scholar
  30. Fisher RA. On the interpretation of χ2 from contingency tables, and the calculation of P. J Royal Stat Soc. 1922;85(1):87–94.View ArticleGoogle Scholar
  31. Omar RZ, Wright EM, Turner RM, Thompson SG. Analysing repeated measurements data: a practical comparison of methods. Stat Med. 1999;18(13):1587–603.View ArticlePubMedGoogle Scholar
  32. Vrieze SI. Model selection and psychological theory: a discussion of the differences between the Akaike information criterion (AIC) and the Bayesian information criterion (BIC). Psychol Methods. 2012;17(2):228–43.View ArticlePubMedPubMed CentralGoogle Scholar
  33. Breiman L. Bagging predictors. Mach Learn. 1996;24(2):123–40.Google Scholar
  34. Halinski RS, Feldt LS. The selection of variables in multiple regression analysis. J Educ Meas. 1970;7(3):151–7.View ArticleGoogle Scholar
  35. Mela CF, Koppale PK. The impact of colinearity on regression analysis: the asymmetric eVect of negative and positive correlations. J Appl Econ. 2002;34:667–77.View ArticleGoogle Scholar
  36. Durbin J, Watson GS. Testing for serial correlation in least squares regression. Biometrika. 1971;58(1):1–19.Google Scholar
  37. Andreopoulos B, An A, Wang X, Schroeder M. A roadmap of clustering algorithms: finding a match for a biomedical application. Brief Bioinform. 2009;10(3):297–314.View ArticlePubMedGoogle Scholar
  38. La Rosa PS, Warner BB, Zhou Y, Weinstock GM, Sodergren E, Hall-Moore CM, Stevens HJ, Bennett WE Jr, Shaikh N, Linneman LA, et al. Patterned progression of bacterial populations in the premature infant gut. Proc Natl Acad Sci U S A. 2014;111(34):12522–7.View ArticlePubMedPubMed CentralGoogle Scholar
  39. Greenwood C, Morrow AL, Lagomarcino AJ, Altaye M, Taft DH, Yu Z, Newburg DS, Ward DV, Schibler KR. Early empiric antibiotic use in preterm infants is associated with lower bacterial diversity and higher relative abundance of Enterobacter. J Pediatr. 2014;165(1):23–9.View ArticlePubMedPubMed CentralGoogle Scholar
  40. Aagaard K, Ma J, Antony KM, Ganu R, Petrosino J, Versalovic J. The placenta harbors a unique microbiome. Sci Transl Med. 2014;6(237):237ra265.View ArticleGoogle Scholar
  41. Dominguez-Bello MG, Costello EK, Contreras M, Magris M, Hidalgo G, Fierer N, Knight R. Delivery mode shapes the acquisition and structure of the initial microbiota across multiple body habitats in newborns. Proc Natl Acad Sci U S A. 2010;107(26):11971–5.View ArticlePubMedPubMed CentralGoogle Scholar
  42. Cong X, Xu W, Janton S, Henderson WA, Matson A, McGrath JM, Maas K, Graf J. Gut microbiome developmental patterns in early life of preterm infants: impacts of feeding and gender. PLoS One. 2016;11(4):e0152751.View ArticlePubMedPubMed CentralGoogle Scholar
  43. Stout MJ, Zhou Y, Wylie KM, Tarr PI, Macones GA, Tuuli MG. Early pregnancy vaginal microbiome trends and preterm birth. Am J Obstet Gynecol. 2017;217:356–e1.View ArticlePubMedPubMed CentralGoogle Scholar
  44. Kindinger LM, Bennett PR, Lee YS, Marchesi JR, Smith A, Cacciatore S, Holmes E, Nicholson JK, Teoh TG, MacIntyre DA. The interaction between vaginal microbiota, cervical length, and vaginal progesterone treatment for preterm birth risk. Microbiome. 2017;5(1):6.View ArticlePubMedPubMed CentralGoogle Scholar
  45. van de Wijgert JH, Jespers V. The global health impact of vaginal dysbiosis. Res Microbiol. 2017;168:859–64.View ArticlePubMedGoogle Scholar
  46. Collado MC, Rautava S, Aakko J, Isolauri E, Salminen S. Human gut colonisation may be initiated in utero by distinct microbial communities in the placenta and amniotic fluid. Sci Rep. 2016;6:23129.View ArticlePubMedPubMed CentralGoogle Scholar
  47. Urbaniak C, Angelini M, Gloor GB, Reid G. Human milk microbiota profiles in relation to birthing method, gestation and infant gender. Microbiome. 2016;4:1.View ArticlePubMedPubMed CentralGoogle Scholar
  48. Patel SH, Vaidya YH, Patel RJ, Pandit RJ, Joshi CG, Kunjadiya AP. Culture independent assessment of human milk microbial community in lactational mastitis. Sci Rep. 2017;7(1):7804.View ArticlePubMedPubMed CentralGoogle Scholar
  49. Costello EK, Stagaman K, Dethlefsen L, Bohannan BJ, Relman DA. The application of ecological theory toward an understanding of the human microbiome. Science. 2012;336(6086):1255–62.View ArticlePubMedPubMed CentralGoogle Scholar
  50. Gupta VK, Paul S, Dutta C. Geography, ethnicity or subsistence-specific variations in human microbiome composition and diversity. Front Microbiol. 2017;8:1162.View ArticlePubMedPubMed CentralGoogle Scholar
  51. Kramer BW, Ikegami M, Moss TJ, Nitsos I, Newnham JP, Jobe AH. Antenatal betamethasone changes cord blood monocyte responses to endotoxin in preterm lambs. Pediatr Res. 2004;55(5):764–8.View ArticlePubMedGoogle Scholar
  52. Kumar P, Venners SA, Fu L, Pearson C, Ortiz K, Wang X. Association of antenatal steroid use with cord blood immune biomarkers in preterm births. Early Hum Dev. 2011;87(8):559–64.View ArticlePubMedPubMed CentralGoogle Scholar
  53. Fuenfer MM, Herson VC, Raye JR, Woronick CL, Eisenfeld L, Ingardia CJ, Block CF, Krause PJ. The effect of betamethasone on neonatal neutrophil chemotaxis. Pediatr Res. 1987;22(2):150–3.View ArticlePubMedGoogle Scholar
  54. Kavelaars A, van der Pompe G, Bakker JM, van Hasselt PM, Cats B, Visser GH, Heijnen CJ. Altered immune function in human newborns after prenatal administration of betamethasone: enhanced natural killer cell activity and decreased T cell proliferation in cord blood. Pediatr Res. 1999;45(3):306–12.View ArticlePubMedGoogle Scholar
  55. Cortese R, Lu L, Yu Y, Ruden D, Claud EC. Epigenome-microbiome crosstalk: a potential new paradigm influencing neonatal susceptibility to disease. Epigenetics. 2016;11(3):205–15.View ArticlePubMedPubMed CentralGoogle Scholar
  56. Sokal MM, Koenigsberger MR, Rose JS, Berdon WE, Santulli TV. Neonatal hypermagnesemia and the meconium-plug syndrome. N Engl J Med. 1972;286(15):823–5.View ArticlePubMedGoogle Scholar
  57. Mehta R, Petrova A. Intrapartum magnesium sulfate exposure attenuates neutrophil function in preterm neonates. Biol Neonate. 2006;89(2):99–103.View ArticlePubMedGoogle Scholar
  58. Gregory KE, Samuel BS, Houghteling P, Shan G, Ausubel FM, Sadreyev RI, Walker WA. Influence of maternal breast milk ingestion on acquisition of the intestinal microbiome in preterm infants. Microbiome. 2016;4(1):68.View ArticlePubMedPubMed CentralGoogle Scholar
  59. Sekirov I, Tam NM, Jogova M, Robertson ML, Li Y, Lupp C, Finlay BB. Antibiotic-induced perturbations of the intestinal microbiota alter host susceptibility to enteric infection. Infect Immun. 2008;76(10):4726–36.View ArticlePubMedPubMed CentralGoogle Scholar
  60. Hourigan S, Ta A, Chettout N, Clemency N, Klein E, Baveja R, Provenzano M, Heberling C, Subramanian P, Hasan NA, et al. Differences in the stool and skin microbiome, virulence factor and antimicrobial resistance genes in a private room versus a shared space neonatal intensive care unit. Gastroenterology. 2017;152(5 Supple 1):S213–4.View ArticleGoogle Scholar

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© The Author(s). 2018

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