- Research article
- Open Access
- Open Peer Review
Exploring the oral microbiota of children at various developmental stages of their dentition in the relation to their oral health
© Crielaard et al; licensee BioMed Central Ltd. 2011
- Received: 25 October 2010
- Accepted: 4 March 2011
- Published: 4 March 2011
An understanding of the relation of commensal microbiota to health is essential in preventing disease. Here we studied the oral microbial composition of children (N = 74, aged 3 - 18 years) in natural transition from their deciduous to a permanent dentition and related the microbial profiles to their oral health status. The microbial composition of saliva was assessed by barcoded pyrosequencing of the V5-V6 hypervariable regions of the 16 S rRNA, as well as by using phylogenetic microarrays.
Pyrosequencing reads (126174 reads, 1045 unique sequences) represented 8 phyla and 113 higher taxa in saliva samples. Four phyla - Firmicutes, Bacteriodetes, Proteobacteria and Actinobacteria - predominated in all groups. The deciduous dentition harboured a higher proportion of Proteobacteria (Gammaproteobacteria, Moraxellaceae) than Bacteroidetes, while in all other groups Bacteroidetes were at least as abundant as Proteobacteria. Bacteroidetes (mainly genus Prevotella), Veillonellaceae family, Spirochaetes and candidate division TM7 increased with increasing age, reflecting maturation of the microbiome driven by biological changes with age.
Microarray analysis enabled further analysis of the individual salivary microbiota. Of 350 microarray probes, 156 gave a positive signal with, on average, 77 (range 48-93) probes per individual sample.
A caries-free oral status significantly associated with the higher signal of the probes targeting Porphyromonas catoniae and Neisseria flavescens.
The potential role of P. catoniae and N. flavescens as oral health markers should be assessed in large-scale clinical studies. The combination of both, open-ended and targeted molecular approaches provides us with information that will increase our understanding of the interplay between the human host and its microbiome.
- Oral Health
- Saliva Sample
- Oral Health Status
- Permanent Dentition
- Oral Microbiota
The oral cavity is a complex ecological niche, as is reflected by its complex microbial community. Recent advances in sequencing technology, such as 454 pyrosequencing, have revealed an unexpectedly high diversity of the human oral microbiome: dental plaque pooled from 98 healthy adults comprised about 10000 microbial phylotypes . This is an order of magnitude higher than previously reported 700 oral microbial phylotypes as identified by cultivation or traditional cloning and sequencing .
Studies have revealed that the various sites in the oral cavity, such as the hard dental surfaces, mucosal sites, and anaerobic pockets, house unique microbial communities [3, 4]. The oral ecological system is dramatically influenced by chemical and physical fluctuations as a result of food and drink intake and oral hygiene measures. Nevertheless studies performed so far have revealed a relatively stable oral microbial community that shows fewer differences between individuals as compared to the skin or gastrointestinal microbiomes . The oral microbiota is intimately related to oral health. It is generally accepted that a shift in microbial composition is an important step in the progression of oral disease. However, there are few studies that have actually demonstrated this ecological shift.
For an individual, birth is a borderline between the sterile intrauterine life and the extrauterine existence with a continuous exposure to microorganisms . Microbiota are acquired via other individuals, animals and the local environment . The microbial community is further shaped by diet and personal oral hygiene.
Here we explored the effects of natural changes in the oral ecosystem during the transition from the deciduous to the permanent dentition of children on the microbial composition of their saliva. We started with an open-ended approach: we sequenced tagged 16 S amplicons of pooled saliva samples using 454 pyrosequencing technology. Then, by using a phylogenetic microarray that targets small subunit (16S) ribosomal DNA of the predominant oral microorganisms, we obtained individual profiles of each saliva sample. To assess the relation of the oral health status of each child with their microbial profile, we quantified the amount of certain oral pathogens and health-associated microorganisms by using a q-PCR technique and compared that with the obtained epidemiological data.
Distribution of children into four subgroups according to the stage of their dentition and the clinical findings.
Nr of children
Age in years
range, mean (s.d.)
Nr of caries-free children
Nr of children with caries
3-6, 4.4 (0.8)
5-11, 7.8 (1.6)
8-12, 10.1 (1.2)
11-18, 13.9 (2.4)
The deciduous dentition harboured a relatively high proportion of Proteobacteria compared to Bacteroidetes. In all other groups, the Bacteroidetes were found to be more abundant than Proteobacteria. In comparison to adult saliva , child saliva appears to have a higher proportion of Firmicutes and Actinobacteria and a lower proportion of Bacteroidetes, Fusobacteria, TM7 (Figure 1) and Spirochaetes at all stages of the dentition.
The higher proportion of Proteobacteria in the deciduous dentition than at any other stage was mainly due to a higher proportion of Gammaproteobacteria at this stage of dentition. The order Pseudomonadales with Pseudomonadaceae (genus Pseudomonas) and Moraxellaceae families (genus Acinetobacter, Moraxella and Enhydrobacter) contributed the most to this difference. At the deciduous dentition stage, about 8% of all reads in the healthy dentition and 4% of the reads in the group with untreated caries belonged to genus Acinetobacter while sequences belonging to this genus were nearly absent from all other stages (Additional file 1, Figure 2). Other groups that also showed a higher abundance in the deciduous dentition included the Enterobacteriaceae family and the genus Aggregatibacter within the Pasteurellaceae family.
No significant differences were observed with respect to species richness between the different sub-groups. Rarefaction curves however (Additional file 2) did show a decreased estimate in species richness in children with caries compared to healthy or treated group.
Individual phylogenic profiles of saliva
The oral microbiota were analyzed at an individual level using a taxonomic microarray based on discriminating regions of the small subunit (16S) ribosomal RNA gene. Of the 350 microarray probes, 156 gave a positive signal (signal/background ratio at least 3) in any of the samples analyzed, with, on average, 77 probes (range 48 - 93, s.d. 10.4) per individual sample (Additional file 3). All samples were positive for probes targeting the phyla Actinobacteria (genus Actinomyces and Rothia), Bacteroidetes (genus Prevotella and order Bacteroidales), Firmicutes (genus Streptococcus, Veillonella, Lactobacillus, Granulicatella) and Fusobacteria (genus Fusobacterium). All but one sample were positive for probes targeting the phylum Proteobacteria. Betaproteobacteria was the most prevalent class (genus Neisseria - in 97% of the samples), followed by Gammaproteobacteria (genus Haemophilus) and Epsilonproteobacteria (genus Campylobacter). Probes targeting candidate division TM7 were positive in 40% of the samples; the probes targeting the domain Archaea (Additional file 4: probe o1311, designed to target Crenarchaeota, Class Thermoprotei) were positive in 44% of the samples. The occurrence of Pseudomonas in the group of children with deciduous teeth was confined to one individual, and did not reflect a common feature of the oral microbiota of this group.
Analysis of specific microorganisms by quantitative PCR
The SAM and PCA analyses of the microarray profiles brought forward multiple probes targeting a group of several species within genus Porphyromonas - P. catoniae, P. gingivalis, P. macacae and P. gulae - as significantly associated with health. P. gingivalis is known as periodontal pathogen associated with destruction of periodontal tissue, and is phylogenetically closely related to P. catoniae. To evaluate the abundance of P. gingivalis in saliva, we used quantitative PCR. P. gingivalis could be detected in only 3 samples, at 1.3 × 102, 4.5 × 104 and 2.7 × 105 cells/ml saliva. Although probe o1503 was designed to specifically target P. gingivalis in our microarray it showed positive signal/background ratio in 98% of samples, indicating general Porphyromonas sensitivity. The pyrosequencing data confirmed the absence (or presence below the detection limit of the method) of P. gingivalis, P. gulae and P. macacae in our samples: the only Porphyromonas species identified was P. catoniae, and it belonged to relatively abundant taxa (1.2 - 5.2% of all reads). The q-PCR data of P. catoniae showed that saliva samples contained between 105 and 108 of P. catoniae cells/ml saliva. The number of P. catoniae cells correlated significantly with the signal of both Porphyromonas probes - o1503, the probe with the closest match for P. gingivalis, and o1506, the probe targeting P. catoniae (Spearman's correlation, p < 0.001; r = 0.618, p < 0.001; r = 0.580 respectively). Both Porphyromonas probes of the microarray hybridized thus with P. catoniae. The number of P. catoniae cells correlated negatively with the total number of decayed, missing and filled (DMFS & dmfs) surfaces (p = 0.024, r = -0.266) and, although less strongly, also with the number of surfaces with caries lesions (p = 0.047, r = -0.235).
To our knowledge, this is the first report on the oral microbiome of children assessed at the depth of next generation sequencing. This open-ended and high resolution approach provided us with the overview of the taxa present in saliva of children, next to our existing knowledge on the adult microbiome [1, 4]. Being aware of the current discussions on the artefacts that may be introduced by pyrosequencing [9, 10], we applied a stringent protocol for filtering sequences. Through a combined approach of pyrosequencing, as well as taxonomic microarray analysis, we showed that salivary microbiome of children is already complex by the age of 3, and it matures with increasing age. However, at the age of puberty it still differs from the adult microbiome. Although the analysis of the adult oral microbiome was performed on a different sequencing platform (GS20), and the forward primers differed from the ones used in this study, this is unlikely to account for the major differences we observed.
As in previous observations, the oral microbiome was shown to be relatively stable, despite the significant biological changes that occur during the eruption of teeth. However, some differences were observed, with the most striking difference between the deciduous dentition and the rest of the stages. The children in this youngest age group harboured groups of microorganisms that are not usually associated with healthy commensal oral microbiota (Pseudomonadaceae, Moraxellaceae, Enterobacteriaceae) at relatively higher proportions than older children. Although from our sequencing data it is not possible to draw any conclusions regarding the pathogenicity, it is known from literature that the Moraxellaceae family member Acinetobacter - the genus that contributed most to this difference - is considered to be a major nosocomial respiratory pathogen and has been reported at high prevalence in dental plaque and saliva of hospitalized individuals [11, 12]. Acinetobacter baumanii is infamous due to its multiple resistance to antibiotics [13, 14]. Studies on upper respiratory tract infections in children have found an association between recurrent tonsillopharyngitis and another member within Moraxellaceae family - Moraxella catarrhalis . The occurrence of Pseudomonas was shown to be confined to one individual.
In addition to the differences in their salivary microbiome, the children with deciduous teeth also had the highest amount of dental plaque among the four groups. Nevertheless, the prevalence and severity of inflammation of oral tissues (gingivitis and periodontitis) is low in healthy young children and gradually increases with increasing age [16, 17]. A classic example of age-related susceptibility to gingivitis was presented three decades ago by an experimental gingivitis study : after discontinued oral hygiene measures for 21 days, both, children and adults accumulated increasing amounts of dental plaque while signs of gingival inflammation were large in adults and remained negligible in children. This age-dependence has multiple natural reasons: the biological changes in tissues around the teeth during the eruption and exfoliation of teeth, the gradual development of the immune defence system and the endocrine system, all contributing to the maturation of the oral microbial communities . With increasing age the proportions of periodontal pathogens also increase [17, 20]. We confirmed the maturation of microbial composition by detecting increased proportions of Bacteroidetes (mainly genus Prevotella), Spirochaetes and candidate division TM7 with increasing age and found the highest abundance of these obligate anaerobes in the adult population .
Our microarray data suggested a positive association between the signal of the probe targeting Porphyromonas catoniae with caries-free status of children. Quantitative PCR confirmed that all children in our study harboured P. catoniae in their saliva, and that the amount of this species correlated negatively with the number of decayed, missing and filled surfaces in their oral cavity. So far there are no other reports supporting the health association of P. catoniae in relation to dental caries. It has however been shown that in periodontitis patients P. catoniae is specifically associated with shallow pockets and healthy sites and not the diseased, deep pockets . Another Porphyromonas species, P. gingivalis, one of the red complex organisms associated with periodontal disease , was found in only three samples by q-PCR. Other authors have also found P. gingivalis to be in low prevalence and abundance in children [20, 23].
P. catoniae (previously Oribaculum catoniae  and Bacteroides D26 ) are saccharolytic, Gram-negative anaerobic rods and the only non-pigmented species among Porphyromonas. Unlike other Porphyromonas species, P. catoniae belongs to early colonizers among obligate anaerobes: it has been detected in two month-old pre-dentate infants, and becomes a regular colonizer once the first teeth erupt [7, 26, 27]. P. catoniae differs from other Porphyromonas spp. in its frequent ability to produce ß-lactamase , an enzyme that inactivates ß-lactam antibiotics. Könönen et al  have hypothesized that this, on one hand, may offer a reservoir of resistance genes potentially transferable to pathogens, while on the other hand, this may allow commensal microorganism as P. catoniae to remain in the oral cavity after frequent ß-lactam antibiotic courses and prevent the overgrowth of opportunistic pathogens.
An interesting group to include in the study was the group of siblings. Fourteen sibling pairs, one set of three siblings (family number 9) as well as one set of four siblings (family number 8) participated in our study. From genotyping studies it is known that both vertical (from mother to child) and horizontal (among siblings and between spouses) transmission of oral microorganisms can occur, e.g., identical P. gingivalis genotypes among siblings were found in 26% of the sibships , while in two of the three families from which strains from siblings were available, a common Streptococcus mutans ribotype occurred in all family members . Recently even the transmission of S. mutans between unrelated children at public schools was reported . Besides microbial transmission, host genetic factors may influence the proportions of certain species in genetically related individuals, as has been estimated from the genetic contributions to the increased similarity of the microbiota of twins as compared with microbiota of unrelated people [32, 33]. In general, our study did not find higher similarity in saliva microbial profiles among siblings than among unrelated individuals. One exception was the family number 9, where profiles of all three siblings were highly similar (Pearson correlation 0.95-0.96) (Figure 4, Additional file 5). One should interpret our findings with caution though, since the individual saliva profiles in our study were biased by using targeted approach and our study was not designed to trace different genotypes. Only studies using an open-ended approach such as individually barcoded sample pyrosequencing  will allow full comparisons of individual microbiomes.
In conclusion, we have demonstrated that salivary microbiota of children aged 3 to 18 years is still in the process of maturation and that certain oral microorganisms may be associated with caries-free oral cavities. This study indicates the potential for further studies, preferably longitudinal clinical trials involving large study populations in revealing the panel of microorganisms as potential oral health markers. With that knowledge oral health professionals will be able to perform timely interventions in the oral ecosystem to prevent the shift from health to disease.
Study Population and Clinical Screening
Children aged 3-18 years, living in the area of Oss, the Netherlands, and being registered at the Youth Dental Care clinic (Jeugdtandverzorging Noordoost Noord-Brabant) participated in the study. Ethical approval was given by the independent Medical Ethics Committee of TNO. Inclusion criteria were good general health, no use of antibiotics in the last 6 months, no braces and written consent of the parents/caretakers of the child. The children were clinically examined in the dental clinic by one calibrated dental epidemiologist as a part of their regular dental check-up. The oral examination included a visual inspection of the oral mucosa, caries experience and plaque. The caries experience was expressed by the dmfs-index. This index was calculated by adding up the total number of decayed, missing and filled surfaces. Surfaces with early enamel lesions (white spots) were registered as sound. A tooth surface was registered as carious if caries lesion had reached dentin or if tooth enamel was undermined by underlying lesion resulting in at least a 0.25-mm-deep surface defect. The amount of dental plaque (plaque index) was assessed using criteria of Greene and Vermillion . In brief, six dental surfaces - buccal surface of both upper permanent or deciduous molars, labial surface of 11 and 31 (permanent dentition) or 51 and 71 (deciduous dentition), and lingual surface of 36 and 46 (permanent dentition) or 75 and 85 (deciduous dentition) - were inspected. If the selected tooth was missing, the contralateral tooth or the neighbouring tooth was assessed instead. Amount of plaque was determined visually by moving the probe along the tooth surface. The surface received score 0 if no plaque was visible, score 1 if plaque was present only at the cervical third of the surface, score 2 if plaque covered a cervical half of the surface, score 3 if plaque reached the incisal or occlusal surface of the tooth. A mean plaque index (average score per number of surfaces scored) was calculated per child.
Unstimulated saliva, as the representation of an average sample of the whole oral ecosystem [3, 4], was collected at the day of the dental check-up, at home, before breakfast and toothbrushing, by drooling into a DNA-free, sterile vial for 5 minutes. The parents were instructed to store the saliva refrigerated (4-7°C) and take the vial to the dental clinic, i.e., within 6 h after collection.
A 0.1-ml quantity of saliva sample was transferred to a sterile screw-cap Eppendorf tube with 0.25 ml of lysis buffer (AGOWA mag Mini DNA Isolation Kit, AGOWA, Berlin, Germany). Then 0.3 g zirconium beads (diameter, 0.1 mm; Biospec Products, Bartlesville, OK, USA) and 0.2 ml phenol were added to each sample. The samples were homogenized with a Mini-beadbeater (Biospec Products) for 2 min. DNA was extracted with the AGOWA mag Mini DNA Isolation Kit and quantified (Nanodrop ND-1000; NanoDrop Technologies, Montchanin, DE, USA).
PCR Amplification, Sample Pooling and Pyrosequencing
PCR amplicon libraries of the small subunit ribosomal RNA gene V5-V6 hypervariable region were generated for the individual samples. PCR was performed using the forward primer 785F (GGA TTA GAT ACC CBR GTA GTC) and the reverse primer 1061R (TCA CGR CAC GAG CTG ACG AC). The primers included the 454 Life Sciences Adapter A (forward primer) and B (reverse primer) fused to the 5' end of the 16 S rRNA bacterial primer sequence and a unique trinucleotide sample identification key per each sample group. This resulted in 12 distinctly labelled pools of samples - deciduous, early mixed, late mixed, and permanent dentition at healthy, treated or caries state. The amplification mix contained 2 units of Pfu Ultra II Fusion HS DNA polymerase and 1× PfuUltra II reaction buffer (Stratagene), 200 μM dNTP PurePeak DNA polymerase Mix (Pierce Nucleic Acid Technologies, Milwaukee, WI), and 0.2 μM of each primer. After denaturation (94°C; 2 min), 30 cycles were performed that consisted of denaturation (94°C; 30 sec), annealing (50°C; 40 sec), and extension (72°C; 80 sec). DNA was isolated by means of the MinElute kit (Qiagen, Hilden, Germany). The quality and the size of the amplicons were analyzed on the Agilent 2100 Bioanalyser with the DNA 1000 Chip kit (Agilent Technologies, Santa Clara, CA, USA) and quantified using Nanodrop ND-1000 spectrophotometer. The amplicon libraries were pooled in equimolar amounts and sequenced unidirectionally in the reverse direction (B-adaptor) by means of the Genome Sequencer FLX (GS-FLX) system (Roche, Basel, Switzerland).
Processing of the Pyrosequencing Data
GS-FLX sequencing data were processed as previously described . In brief, we trimmed sequences by removing primer sequences and low-quality data (sequences that did not have an exact match to the reverse primer, that had an ambiguous base call (N) in the sequence, or that were shorter than 50 nt after trimming). We then used the GAST algorithm  to calculate the percent difference between each unique sequence and its closest match in a database of 69816 unique eubacterial and 2779 unique archaeal V5-V6 sequences, representing 323499 SSU rRNA sequences from the SILVA database . Taxa were assigned to each full-length reference sequence using several sources including Entrez Genome entries, cultured strain identities, SILVA, and the Ribosomal Database Project Classifier . In cases where reads were equidistant to multiple V5-V6 reference sequences, and/or where identical V5-V6 sequences were derived from longer sequences mapping to different taxa, reads were assigned to the lowest common taxon of at least two-thirds of the sequences. Only sequences that were found at least 5 times were included in the analyses. This strict and conservative approach was chosen to preclude inclusion of sequences from potential contamination or sequencing artefacts.
Probe Design for the 16S rDNA Microarray
For the design of the taxonomic microarray literature inventory was made on the description of the normal oral microbiota [2, 3, 39–41]. The literature based inventory was compared to the 454 pyrosequencing data that were obtained in this study. While the majority of taxa observed by 454 sequencing were already included in the literature inventory, a number of taxonomic groups were found to be missing. These were included in the list. Based on the list, probes were designed using ARB . The probes were 20-22 nucleotides in size, with a predicted melting temperature of 60°C ± 5, and a GC level between 40 and 60%. The full list of oligonucleotides is provided in Additional file 4.
Microarrays for this study were produced in house, using the ArrayIt Nanoprint60 Microarray Robot. The 5'-amino-modifier-C6-linked oligonucleotides were diluted to a final concentration of 25 μM in a 50 mM Phosphate buffer (pH 7), and printed onto CodeLink Activated Slides. Following incubation at 80% humidity under ambient conditions, slides were blocked in a buffer of 0.1 M Tris Base and 50 mM ethanolamine (pH 9) for 45 minutes at 50°C while shaking in accordance with the manufacturer's recommendations. After that, the slides were rinsed twice in MilliQ purified water (MilliQ, Millipore), washed in 4 × SSC (600 mM sodium chloride/60 mM sodium citrate), 0.1% sodium dodecyl sulfate (SDS) for 30 minutes at 50°C, and washed in pre-warmed (50°C) MilliQ water. Following that, the slides were washed twice in MilliQ water at a room temperature, and dried under a stream of nitrogen. Slides were stored under nitrogen until use.
DNA Labelling and Hybridization
For taxonomic microarray analysis, 16 S rDNA was amplified by PCR as described above, using forward primers 8F (AGA GTT TGA TCH TGG YTC AG) and 8F-bif (TGG CTC AGG ATG AAC GCT G) and reverse primer 1061R (TCA CGR CAC GAG CTG ACG AC). Following PCR amplification, DNA was amplified by random Klenow amplification with the BioPrime DNA Amplification kit (Invitrogen) according to the manufacturer's recommendations. Klenow-amplified DNA was passed through an Illustra AutoSeq G-50 column (GE Healthcare G50) for purification and concentrated in a speedvac. Following, the DNA was labelled by Terminal Transferase coupling of Cy3-dUTP (Promega). Following Illustra AutoSeq G-50 column purification, and vacuum concentration, the labelled DNA was dissolved in 40 μl Easyhyb hybridization buffer (Roche), and denatured for 2 min at 95°C. Printed slides were pre-hybridized in 0.45 μm-filtered pre-hybridization buffer [1% BSA, 5 × SSC, and 0.1% SDS] at 42°C for 45 min with rotation, then washed twice with MilliQ purified water, dried with nitrogen, and pre-warmed at 42°C. The microarrays were placed in the ProPlate multi-array system (Grace Bio-Labs). The hybridization mixture was then pipetted in the individual wells, and incubated in a hybridization chamber for four hours. Following hybridization, slides were then thoroughly washed sequentially in 1 × SSC, 0.2% SDS for 10 sec at 37°C, 0.5 × SSC for 10 sec at 37°C, and twice in 0.2 × SSC for 10 min at room temperature. Slides were dried with nitrogen and scanned using a Scanarray Express 680013 Microarray Analysis System (Perkin Elmers Life Analytical Sciences Inc.). Images were obtained and quantified with ImaGene 4.2 software (Biodiscovery).
To validate microarray performance, a number of tests were performed. These included: 1) Replicated analysis of samples to test robustness of microarray data; 2) Spiking DNA of underrepresented species to a complex mixture followed by microarray analysis; 3) performing a direct comparison between qPCR and microarray data, and 4) performing a direct comparison between sequencing and microarray data.
Technical replicates were included to verify robustness of data. In the examples described below, three replicates were compared. Two were analyzed on slides of the same printing series - sMF02-11, and one was analyzed on an older slide series (sMF02-9). The Pearson correlation (r) between the three microarray analyses was high, and varied between 0.91 and 0.93, and was independent of the slide series. For comparison, correlation between different saliva samples ranged from 0.4 to 0.7.
To test the performance of the microarray with the complex oral microbial community, we performed a spiking experiment. For this, DNA was isolated from saliva samples of a healthy adult donor as well as from pure cultures of Lactobacillus casei (ATCC 334). Following, DNA was quantified, and pure culture DNA was added to saliva DNA at levels ranging between 0.01 and 1% of the total community. Then the DNA was labelled, and used to hybridize the microarray. A clear signal was detected in all spiked samples for the L. casei spot on the microarray in a dose responsive manner. At the family level, also a significant dose responsive increase in microarray spot intensity was detected (with lower sensitivity).
Direct Comparison between qPCR and Microarray Data
A third method for validating microarray data was by cross comparing species levels established by quantitative PCR with the results obtained using the microarray. In the current study, this was performed for Porphyromonas catoniae in saliva samples obtained from the children. During the study, 74 saliva samples were analyzed. The q-PCR data of P. catoniae showed that saliva samples contained between 105 and 108 of P. catoniae cells/ml saliva. The fluorescence intensity for the P. catoniae probes on the microarray ranged between 0 and 110. The number of P. catoniae cells correlated significantly with the signal of both Porphyromonas probes - o1503 and o1506. The Spearman's correlations were p < 0.001; r = 0.618 and p < 0.001; r = 0.580, respectively.
Direct Comparison between Sequencing and Microarray Data
To enable a direct comparison between microarray and sequencing data, both data sets were coupled by using the probe and sequence data. For this, a string search was used to identify matching probe sequences within the 454 pyrosequencing data. For 26 probes a direct match was identified. This relatively low number of matching probe sequences is due to the fact that the pyrosequencing data span the V5-V6 region, while the majority of probes were defined in the V2, V3 and V4 region of the 16 S ribosomal gene. We then calculated the Pearson correlation between the microarray and 454 sequencing data. Good (r = 0.85) to excellent (p > 0.9) correlation was found for probes corresponding to relatively abundant taxa (>0.1% of all reads; signal/background fluorescence value >20). The correlation for less abundant species was weak. No false positive probes were found. Only two probes (o1402 and o1445) were classified as false negatives.
Targeting of specific microorganisms by quantitative PCR
Quantitative PCR was performed on the Applied Biosystems 7500 Fast Real-Time PCR System. The total microbial load was determined using the universal primer set described by Nadkarni et al . The P. catoniae and P. gingivalis primer-probe sets were designed using Primer Express (Applied Biosystems). To quantify P. catoniae, the primer-probe set of P. catoniae-16S-F (CGG TTG CCA TCAG GTA ATG C), P. catoniae-16S-R (CAC CTT CCT CAC GCC TTA CG) and P. catoniae-16S-probe (TCC GTA GAG ACT GCC G), a minor-groove binding probe (MGB) labeled with 6-carboxy-fluorescein (FAM) was used. The P. gingivalis primer-probe set was composed of P. gingivalis-16S-F (GCG CTCA ACG TTC AGC C), P. gingivalis-16S-R (CAC GAA TTC CGC CTG C) and the FAM labeled minor-groove binding (MGB) probe P. gingivalis-16S-probe (CAC TGA ACT CAA GCC CGG CAG TTT CAA). Quantitative PCR was performed using the Diagenode Universal Mastermix, in accordance with the manufacturer's recommendations. Standard controls included a serial dilution series of purified genomic DNA of P. gingivalis ATCC BAA-308 and P. catoniae ATCC 51270.
To identify the probes that contribute significantly to the different response variables (oral health status, the stage of dentition), we performed the Significance Analysis of Microarrays (SAM analysis) - a non-parametric statistical technique for finding significant differences between microarray data that are grouped based on experimental conditions . To reduce the dimensions of the array data we performed the principal component analysis (PCA). Similarities among individual sample profiles were calculated using the sample distance matrix. The SAM and PCA analyses were performed using the MeV software package, as part of the TM4 microarray software suite . The sample distance matrix was calculated using Pearson correlation coefficient and visualized using hierarchical clustering with the average linkage method. Independent samples T-test, Pearson and Spearman correlations were calculated using SPSS (Version 17.0). Abundances of probes that showed significant differences in SAM and contributed most to the PCA were tested by ANOVA, Games-Howell post-hoc test using SPSS (Version 17.0).
We thank Louise Nederhoff, Mieke Havekes and Norbert Sedee for excellent technical assistance. We thank Jeugdtandverzorging Noordoost Noord Brabant for facilitating sample collection. Susan Huse was supported on a subcontract to Mitchell L. Sogin from the Woods Hole Center for Oceans and Human Health, funded by the National Institutes of Health and National Science Foundation (NIH/NIEHS1 P50 ES012742-01 and NSF/OCE 0430724). We also thank the ACTA Research Institute, the Dutch Ministry for Economic Affairs, GABA International, Leaf Holland BV and FrieslandCampina for financial support.
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