Abstract
Molecular fingerprinting and sequencing based techniques have been widely used to characterize microbial communities. Terminal restriction fragment length polymorphism (T-RFLP) and 454-pyrosequencing were used to determine the microorganisms present in the different sections of the chicken gastrointestinal tract (GIT) (crop, jejunum, ileum and caeca). Broilers fed with diets differing in phosphorous (P) and calcium (Ca) as well as in phytase levels were used to study the microbiota of the upper and lower part of the GIT. A database with terminal restriction fragments (T-RF) of the most important organism present in the different gastrointestinal sections was constructed. The analysis revealed a distinct microbial assemblage on each section. Regardless of the diet, crop, jejunum and ileum were mainly colonized by Lactobacillaceae, and caeca were the most diverse site. The correlation between Lactobacillus crispatus and L. reuteri was positive in the crop, but negative in the jejunum. In crop samples, higher P and Ca levels led to a shift in the abundance of L. reuteri and L. crispatus to L. salivarius and L. taiwanensis whereas in the ileum supplementation of phytase favored L. salivarius and L. taiwanensis but resulted in decreased abundance of L. crispatus. Both methods were correlating significantly, being T-RFLP a reliable fingerprinting method to rapidly analyze large numbers of samples in a cost-effective and rapid manner. Results are easy to interpret with no need of deep bioinformatics knowledge and can be integrated with taxonomic information.
Introduction
The microbiota colonizing the gastrointestinal tract (GIT) of chickens plays an important role in shaping health and productivity of the host animal [1] and is also involved in protection from pathogens, detoxification, modulation of the immune system and breakdown of feed components [2]. Species within this complex ecosystem differ in their substrate preferences and growth requirements thus are affected by the chemical composition of the digesta that is determined by the GIT section as well as by the diet composition [3]. Dietary factors such as type and content of carbohydrates and proteins, and different feed additives (e.g. probiotics, organic acids and feed enzymes) have been recognized to alter the gut microbiota in chickens [4, 5]. Moreover, variation in supplementation of minerals such as calcium (Ca) and phosphorus (P) has been shown to modulate the microbiota of rats [6] and pigs [7].
Dietary P and Ca content also affects the composition of the microbial community in the GIT of broiler chickens [8, 9]. P in plant feedstuffs is mainly present as phytate-bound P and phosphate release from phytate involves the enzyme phytase and other phosphatases. Phytases are present in dietary plant feeds [10] and to a limited extent in the mucosa of chickens [11, 12]. Phytases also can be produced by different intestinal bacteria [13]. However, some part of dietary phytate remains non-digested in the intestine of broiler chickens. Therefore, to meet the animal’s P requirements, mineral P and microbial phytases are usually added to broiler diets. These supplements affect phytate hydrolysis and P availability in the GIT [14, 15]. Amongst changes of dietary or mucosal phytase activity this may be mediated by shifts within the bacterial community composition. Studies investigating the effect of mineral P and phytase supplementation on the microbiota of chickens are rare and restricted to the ileum and/or caeca [8, 9, 16]. However, the main activity of dietary phytases can be expected in the upper GIT [17] and bacteria with a high potential to degrade phytate were found in the upper GIT [13].
Culture-independent molecular-based methods have been developed for characterization of microbial communities in different habitats. Two major approaches are community fingerprinting and sequencing-based techniques [2]. A well-established molecular fingerprinting technique of 16S rRNA gene-based analysis of microbial communities within the GIT of chickens is the terminal restriction fragment length polymorphism (T-RFLP) [18–20]. Nevertheless, a significant shift towards high-throughput next-generation sequencing methods such as 454 pyrosequencing for microbial communities characterization, is evident in the last years [2]. Despite being more affordable than ever, generating large-scale, well-replicated microbial diversity investigations with next-generation sequencing methods remains an expensive and time-consuming option [21]. Thus, several studies aimed to compare microbial community structures using T-RFLP analysis and 454 pyrosequencing. Choe and colleagues detected different bacteria in biofilms from urinary catheters depending on the use of either T-RFLP or pyrosequencing [22]. Brugger and colleagues observed a different sensitivity of both methods for discrimination of different bacterial species in the nasopharyngeal space [23]. In contrast, in studies being conducted on soil, aquifer, human feces or rumen samples both methods correlated well and gave similar results regarding the most dominant members within microbial communities [21, 24–26]. Studies in which both T-RFLP and pyrosequencing were concurrently used for characterizing the microbiota of the chicken’s GIT are not available in literature. Nordentoft and colleagues used both methods to describe the microbiota of laying hens housed in different cage systems, but the approaches were applied in a more complementary than concurrently way [27]. Thus, the aim of the present study was to investigate the sensitivity of the fingerprinting method T-RFLP against 454 pyrosequencing to compare microbial communities along the GIT of broiler chickens fed with diets differing in mineral P and Ca levels as well as in supplementation of microbial phytase.
Material and Methods
Ethic statement
The animal experiment was carried out in the Agricultural Experiment Station of Hohenheim University, location Lindenhöfe in Eningen (Germany), in strict accordance with the German Animal Welfare legislation. All procedures regarding animal handling and treatments were approved by the Animal Welfare Commissioner of the University.
Birds, diets and sampling
Samples for bacterial community analysis were obtained from an animal experiment described in detail by Zeller et al. [15]. In brief, a 2x3 factorial arrangement of dietary treatments was used. Two corn-soybean meal-based grower diets contained P only from plant sources (BD-) or additionally supplemented P from monocalcium phosphate (MCP), (BD+). Treatments consisted of the BD- and BD+ supplemented with 0, 500 or 12,500 FTU of an E. coli phytase/kg of feed.
Broiler chicken hatchlings (strain Ross 308) were allocated to floor pens, 20 birds each. Animals were fed with a commercial starter diet until 15 days of age; this diet contained 0.90% Ca, 0.65% tP, 22.0% crude protein, 6.8% ether extract, 12.6 MJ ME/kg, and 606 FTU/kg 3-phytase (EC 3.1.3.8, 4a E1600). At day 15 of age animals were switched to experimental diets. The six dietary treatments were randomly assigned to the pens (six pens per diet) and treatment diets were fed for 10 days and were offered for ad libitum consumption. Samples for microbial analysis were taken on day 25 of age from four chickens per pen and six pens per diet. Birds were euthanized by carbon dioxide asphyxiation following anesthesia in a gas mixture and different segments of the digestive tract were dissected to collect luminal digesta from the crop, jejunum (second half of the intestine between gizzard and Meckel’s Diverticulum), the distal two-thirds of the ileum (from Meckel´s Diverticulum until 2 cm before the ileocaecal junction) and the two caeca. Luminal digesta samples of each segment were pooled on a pen basis and stored at -80°C.
454 pyrosequencing of 16S rRNA gene amplicons
Extraction of genomic DNA from luminal digesta samples was carried out using the QIAamp DNA Stool Mini Kit (Qiagen, Hilden, Germany) according to the manufacturer’s instructions. The quality and purity of DNA extracts were determined spectrophotometrically (NanoDrop UV-Vis spectrophotometer 2000c, Thermo Fisher Scientific) and checked by agarose gel electrophoresis. DNA concentrations were measured fluorometrically by using the Qubit 2.0 fluorometer and Qubit dsDNA BR Assay Kit (Life Technologies, Darmstadt, Germany).
Three of the six DNA extracts per treatment and GIT section showing the best DNA quality and quantity were used for further analysis. The microbial community composition of a pooled DNA extract of the chosen replicates per treatment and section was amplicon pyrosequenced using 27F and 1492R [28] primers and Roche GS FLX++ technology (Eurofins Scientific).
Sequenced 16S rRNA gene amplicons were processed using Mothur software [29]. Sequences were quality filtered by excluding reads that had an average quality score lower than 20, a total length of less than 400 base pairs (bp), any primer or barcode mismatch, more than 10 homopolymer stretches and an N character. Sequences were sorted regarding their barcodes and primers and barcodes were trimmed from each read. Sequences were aligned and checked for chimeras using uchime and clustered into operational taxonomic units (OTU) at ≥ 97% similarity within Mothur [29]. Low abundance OTU (< 0.0004% of total reads) were removed. A total of 969 phylotypes were taxonomically assigned using the naïve Bayesian RDP classifier [30]. Sequences were submitted to European Nucleotide Archive under the study accession number PRJEB9198. All samples comprised more than 6.825 sequence reads, where the mean number of sequences per sample was 9.400±353, totaling 225.601 usable sequences reads.
T-RFLP profiling of 16S rRNA gene amplicons
16S rRNA gene fragments from the same pooled DNA samples as used for 454 pyrosequencing were amplified by polymerase chain reaction (PCR) using the universal bacterial primers 27F labeled at the 5′ end with 6-carboxyfluorescein (6-FAM) and 1492R [28]. PCR was performed in a total volume of 50 μl containing 10 μl of 5×PCR-Mastermix (Bio&SELL, Feucht, Germany), 0.4 μM of each primer (Biomers, Ulm, Germany), 2–15 μl of template DNA and nuclease free water (Qiagen). PCR from crop, jejunum and ileum samples were run in quadruplicates and for caecal samples in duplicates. An initial denaturation at 94°C for 4 min, followed by 30 cycles of denaturation at 94°C for 45 s, annealing at 58°C for 60 s, elongation at 72°C for 2 min and a final extension step at 72°C for 20 min was applied. Amplification products were purified using the Double Pure Kombi Kit (Bio&SELL) and fluorometrically quantified as described before.
70 ng of the purified PCR products were digested overnight using 5U of HaeIII (New England BioLabs, Frankfurt, Germany) as according to manufacturer instructions and digests were purified using Sephadex (illustra Sephadex G-50 Fine DNA Grade, GE Healthcare, Little Chalfont, UK).
Separation of fragments was carried out by capillary electrophoresis on a 3130 Genetic Analyzer (Applied Biosystems, Darmstadt, Germany) using an internal size standard (MapMarker X-Rhodamine Labeled 50–1500 bp, BioVentures, Murfreesboro, TN, USA). Fluorescent signals of terminal restriction fragments (T-RF) were extracted in the range of 50–1000 bp using the Gene Mapper V4.1 software (Applied Biosystems) and normalized according to Abdo and colleagues [31].
In addition, each DNA extract used for that pool was processed separately as previously described and analyzed by T-RFLP as single replicate (n = 3), to give a better insight of bacterial community for each dietary treatment.
Cloning and sequencing of 16S rRNA gene amplicons for identification of T-RFs
DNA extracts of all six treatments were pooled per GIT section (crop, ileum, caeca) and amplified as described above except that the forward primer was not fluorescently labeled. PCR products were purified with the MinElute PCR Purification Kit (Qiagen) and cloned using the TA Cloning Kit TOP10F (Life Technologies). Ninety-six clones per section were screened by amplified ribosomal DNA restriction analysis (ARDRA) using the restriction enzyme AflIII (BioLabs) and sequenced on an ABI 3370xl Genetic Analyzer (Applied Biosystems, Weiterstadt, Germany). Clones were taxonomically assigned using the naïve Bayesian RDP classifier [30]. Finally, 25 different clones for crop, 24 for ileum and 47 for caeca were chosen for sequencing and clones of interest were analyzed by T-RFLP as previously described. Sequences were submitted to GenBank under the accession number KP780094-KP780131.
Statistical analysis
Two multivariate data-sets comprising the relative abundance of each T-RF and the percentage distribution of each phylotype across each sample were analyzed using PRIMER (v.6.1.6, PRIMER-E, Plymouth Marine Laboratory, UK) [32]. Sample-similarity matrices were generated using the Bray-Curtis coefficient [33] and the bacterial community structures were explored by principal coordinate analysis (PCoA) [32]. Clusters were superimposed over the PCoA plot to represent the percentage similarity within a group of samples. A similarity profile permutation test (SIMPROF) was used to seek for statistically significant clusters [34]. Statistical comparisons between different gut sections and diets were made using analysis of similarity (ANOSIM) with 999 permutations [32]. The RELATE routine in Primer 6 [32] was used to quantify the pattern match between the two resemblance matrices generated from the pooled T-RFLP and 454-pyrosequencing samples. Rho values were considered significant if less than 5% of 9999 randomly permutated were greater than the real rho value. Phylotype richness and diversity were explored using univariate measures through PRIMER [32]. Pielou’s evenness (J') is an equitability measure, which expresses how evenly the sequence reads are distributed among the OTUs and was calculated as J' = H'/H'max = H'/logS. Shannon diversity (H’) was calculated as H' = -Σi pi ln(pi), where pi is the relative abundance of the ith OTU. Pearson correlation coefficient (999 permutations) was used to measure the occurrence of a pair of species sharing the same niche in relative proportions using PRISM 6 (GraphPad Software, CA). Positive and negative correlations were considered significantly different if p < 0.05.
Draftsman plots charting the relative abundance of one species-of-interest against another were used to visualize negative and positive correlations between species [35].
Results
Microbial community structure along the GIT of broilers
The total number of OTUs and T-RFs detected in digesta samples regarding each dietary treatment and GIT section as well as Shannon diversity and Pielou’s evenness values are given in S1 Fig and S1 Table. The values showed a low diversity of the samples from jejunum and ileum, medium diversity for crop samples and a high diversity for caeca samples.
Exploring the global bacterial community structure using PCoA revealed a clear separation of bacterial communities found in caecal samples compared to those from crop, jejunum and ileum irrespective of the methodological approach (Fig 1A, 1B and 1C). Further variation of samples was associated with a shift of the bacterial community composition from crop samples to those from the small intestine. Pyrosequencing results showed a second distinct cluster with 50% similarity formed by most of the crop samples and a third one with jejunum and ileum samples (Fig 1A). T-RFLP PCoA of pooled samples showed a cluster with 50% similarity of crop samples without supplementation of MCP and all jejunum and ileum samples. Crop samples supplemented with MCP clustered together at 50% similarity (Fig 1B). Similar results were observed for T-RFLP of single replicates (Fig 1C).
Fig 1. Principle coordinate analysis (PCoA) depicting the shifts in bacterial communities among the gastrointestinal tract of broilers fed with different diets varying in supplementation of monocalcium phosphate: BD- (open circles) and BD+ (close circles) and different levels of phytase: 0 (black), 500 (red), 12,500 (blue) FTU/kg feed, as detected by 454-pyrosequencing (A) and T-RFLP of pooled samples (B) and single replicates (C).
Clusters represent samples sharing more than 50% similarity of their bacterial communities.
ANOSIM was used to test for significant differences in the bacterial community across all the sections. A significant difference of global bacterial profiles along the different sections of broiler’s GIT was observed for all three types of analyses (454 pyrosequencing: R = 0.756, p = 0.001; T-RFLP pooled: R = 0.716, p = 0.001; T-RFLP single: R = 0.641, p = 0.001). An effect of MCP or phytase addition to the diet was not detected, in any of the cases.
Throughout the four GIT sections investigated, bacteria from eight different phyla were identified by 454 pyrosequencing with Firmicutes, Proteobacteria and Bacteroidetes being the most abundant ones and represented by 867, 34 and 26 out of 969 OTUs, respectively. Firmicutes dominated in all four GIT sections. In jejunum samples more than 99.8% of the sequences found were affiliated to this phylum. Proteobacteria were observed in the crop and in the ileum in relative abundances lower than 27% and together with Firmicutes more than 97% of total bacterial community was covered. In caecal samples a considerable contribution of Bacteroidetes (>18%), Tenericutes and Proteobacteria (1–5%) to the bacterial community composition was observed. At family level digesta samples from crop, jejunum and ileum were mainly colonized by species belonging to Lactobacillaceae family while phylotypes belonging to Ruminococcaceae, Bacteroidaceae, uncultured Clostridiales, and Streptococcaceae (circa 80% of total community; Fig 2) were detected in caeca.
Fig 2. Microbiota taxonomy of GIT of chicken fed with different diets using pyrosequencing data.
Relative abundance of bacterial families within the crop, jejunum, ileum and caeca. Diets differed in supplementation of monocalcium phosphate (BD-/BD+) and phytase (0, 500, 12,500 FTU/kg feed).
The most abundant OTUs, with their relative abundance on each section per diet are listed in Table 1 and S2 Table. The phylotypes contributing significantly to the observed differences between GIT sections were closely related to Lactobacillus crispatus, L. salivarius, L. taiwanensis, Bacteroides fragilis, L. aviarius, Shigella flexneri, Aeromonas sharmana and L. vaginalis. Sequencing of clone libraries showed a similar phylogenetic picture (Table 2). While L. salivarius-type phylotypes were the most abundant species found in the crop (>46%), sequences obtained from the small intestine mainly represented L. crispatus-type species (>81% for jejunum, >77% for ileum). In the crop this phylotype was detected on a relative average abundance of 19% and was less abundant in caeca (<0.4%). A similar trend for both lactobacilli were found by T-RFLP, where T-RF designated to L. salivarius decreased from crop to caeca and T-RF designated to L. crispatus made up 36% in the crop, 78% in the small intestine and only 2% in the caeca. The second important phylotype occurring in the small intestine, L. aviarius (>7% of all OTU), was also of minor importance in crop and caeca (<0.2% of all OTU). Differences between both sections of the small intestine were mainly explained by the decreased abundance of L. crispatus- and the increased abundance of Shigella flexneri-type species in the ileum when compared to the jejunum. Moreover, a continuous drop of the abundance of L. taiwanensis- and L. vaginalis-type phylotypes could be detected from crop to caeca significantly contributing to observed differences between sections. This was confirmed by T-RFLP analysis showing a decrease of T-RF designated to L. taiwanensis and L. vaginalis/L. reuteri from the crop to the ileum. Sequences being most abundant in caecal samples (>2.5%) showed a very low abundance in the upper GIT (<0.07%) and were classified as B. fragilis-, Alistipes finegoldii-, Pseudoflavonifractor capillosus- and B. ovatus-type species. The first three mentioned phylotypes could be identified by T-RFLP (Table 2) and three further T-RFs 195, 308, 315 with more than 2.5% abundance contributed to significant differences between caecal samples and those of the upper GIT but could not be identified by cloning. More clones were obtained from the caeca samples, however they showed a low identity with sequences available on the database and were not taken into consideration in this work. Mantel test showed a significant correlation between the results obtained with 454 pyrosequencing and T-RFLP of pooled samples (R = 0.92, p = 0.001). Moreover, SIMPER analysis for T-RFLP of the three single replicates per treatment revealed the same species contributing to differences between crop, jejunum, ileum and caeca as for T-RFLP of pooled samples.
Table 1. List of the 30 most abundant OTUs found among the GIT of broilers detected by 454-pyrosequencing, their average abundance in different sections and sequence similarity to closest reference strains in GenBank.
| OTU | Average abundance (%) | Closest reference strain (Genbank accession no.) | RDP a score | |||
|---|---|---|---|---|---|---|
| Crop | Jejunum | Ileum | Caeca | |||
| 1 | 19.29 | 81.93 | 77.67 | 0.34 | Lactobacillus crispatus (AF257097) | 0.92 |
| 2 | 46.47 | 3.42 | 4.94 | 0.04 | Lactobacillus salivarius (AF089108) | 0.92 |
| 3 | 18.21 | 6.13 | 1.04 | 0.02 | Lactobacillus taiwanensis (EU487512) | 0.91 |
| 4 | 0.02 | <0.01 | 0.07 | 16.86 | Bacteroides fragilis (CR626927) | 0.96 |
| 5 | 0.11 | 7.29 | 7.95 | 0.12 | Lactobacillus aviarius (M58808) | 0.87 |
| 6 | 0.17 | 0.03 | 5.60 | 1.80 | Escherichia/Shigella flexneri (X96963) | 0.89 |
| 7 | 0.01 | 0 | 0.03 | 4.15 | Paenibacillus amylolyticus (D85396) | 0.42 |
| 8 | 0.01 | <0.01 | <0.01 | 3.43 | Alistipes finegoldii (AY643083) | 0.90 |
| 9 | <0.01 | 0 | <0.01 | 2.92 | Pseudoflavonifractor capillosus (AY136666) | 0.76 |
| 10 | 3.75 | 0.13 | 0.09 | 0 | Lactobacillus vaginalis (AF243177) | 0.90 |
| 11 | <0.01 | 0 | 0.04 | 2.77 | Bacteroides ovatus (AB050108) | 0.80 |
| 12 | 3.77 | 0.01 | 0.03 | 0 | Aeromonas sharmana (DQ013306) | 0.82 |
| 13 | <0.01 | 0 | <0.01 | 2.59 | Pseudoflavonifractor capillosus (AY136666) | 0.67 |
| 14 | <0.01 | 0 | <0.01 | 2.11 | Clostridium orbiscindens (Y18187) | 0.82 |
| 15 | 0 | 0 | <0.01 | 1.82 | Bacillus thermocloacae (Z26939) | 0.43 |
| 16 | <0.01 | 0 | <0.01 | 1.63 | Bacteroides thetaiotaomicron (AE015928) | 0.91 |
| 17 | <0.01 | 0 | <0.01 | 1.57 | Oscillibacter valericigenes (AB238598) | 0.60 |
| 18 | 0.01 | 0 | 0.02 | 1.40 | Eubacterium desmolans (L34618) | 0.78 |
| 19 | <0.01 | 0 | <0.01 | 1.17 | Clostridium termitidis (FR733680) | 0.46 |
| 20 | <0.01 | 0 | 0.01 | 1.13 | Clostridium bolteae (AJ508452) | 0.71 |
| 21 | <0.01 | 0 | <0.01 | 1.11 | Clostridium spiroforme (X75908) | 0.86 |
| 22 | 0.01 | 0 | <0.01 | 1.14 | Clostridium leptum (AJ305238) | 0.39 |
| 23 | <0.01 | 0 | 0 | 1.03 | Phascolarctobacterium faecium (X72865) | 0.69 |
| 24 | 1.13 | 0.08 | 0.06 | <0.01 | Lactobacillus reuteri (L23507) | 0.73 |
| 25 | 0 | 0 | 0 | 0.99 | Spiroplasma chinense (AY189126) | 0.39 |
| 26 | 0 | 0 | 0 | 0.89 | Anaerotruncus colihominis (AJ315980) | 0.60 |
| 27 | 0.01 | 0 | <0.01 | 0.86 | Oscillibacter valericigenes (AB238598) | 0.60 |
| 28 | <0.01 | 0 | <0.01 | 0.82 | Butyricicoccus pullicaecorum (EU410376) | 0.44 |
| 29 | <0.01 | 0 | <0.01 | 0.87 | Eubacterium tortuosum (L34683) | 0.55 |
| 30 | <0.01 | 0 | <0.01 | 0.89 | Clostridium methylpentosum (Y18181) | 0.56 |
| Total | 93 | 99 | 98 | 54 | ||
aRibosomal database project
Table 2. Predicted and observed terminal restriction fragments (T-RFs) in base pairs (bp) of clones of interest detected in clone libraries and associated T-RFs obtained from T-RFLP of pooled samples after digestion with HaeIII.
| Clone | Genbank accecssion no. | Closest reference strain (Genbank acc. no.) | RDP score | Predicted T-RF a | Observed T-RF | Pseudo-T-RF I b | Pseudo-T-RF II b | Observed T-RF pooled samples |
|---|---|---|---|---|---|---|---|---|
| K11 | KP780124 | Lactobacillus reuteri (L23507) | 0.83 | 67 | 62 | 336 | 62 | |
| K1 | KP780095 | Lactobacillus vaginalis (AF243177) | 0.95 | 66 | 62 | 62 | ||
| C14 | KP780096 | Faecalibacterium prausnitzii (AJ413954) | 0.80 | 185 | 183 | 317 | 332 | 183 |
| C26 | KP780098 | Clostridium amygdalinum (AY353957) | 0.80 | 237 | 234 | 235* | ||
| C37 | KP780099 | Pseudoflavonifractor capillosus (AY136666) | 0.81 | 239 | 236 | 236 | ||
| C6 | KP780102 | Clostridium lactatifermentans (AY033434) | 0.85 | 242 | 241 | 241 | ||
| K5 | KP780121 | Lactobacillus crispatus (AF257097) | 0.98 | 243 | 243 | n.o. | ||
| I3 | KP780103 | Lactobacillus crispatus (AF257097) | 1 | 246 | 244 | 244 | ||
| C44 | KP780104 | Bacteroides ovatus (AB050108) | 0.87 | 261 | 260 | 267 | 260 | |
| C74 | KP780105 | Bacteroides fragilis (CR626927) | 0.96 | 263 | 262 | 851 | 261* | |
| C110 | KP780131 | Helicobacter pullorum (AY631956) | 0.95 | 270 | 267 | 266* | ||
| C64 | KP780109 | Clostridium saccharolyticum (Y18185) | 0.80 | 273 | 271 | 271 | ||
| C75 | KP780128 | Eubacterium desmolans (L34618) | 0.82 | 275 | 275 | n.o. | ||
| K3 | KP780111 | Lactobacillus salivarius (AF089108) | 0.96 | 279 | 277 | 321 | 276* | |
| I46 | KP780125 | Lactobacillus aviarius (M58808) | 0.90 | 280 | 277 | 276* | ||
| K17 | KP780120 | Lactobacillus salivarius (AF089108) | 0.96 | 278 | 278 | 323 | 278 | |
| K44 | KP780113 | Hordeum vulgare subsp. vulgare (EF115541) | 0.99 | 295 | 293 | 293 | ||
| K62 | KP780114 | Lactobacillus salivarius (AF089108) | 0.94 | 323 | 321 | 321 | ||
| K9 | KP780115 | Lactobacillus salivarius (AF089108) | 0.96 | 323 | 323 | 322* | ||
| K12 | KP780116 | Lactobacillus taiwanensis (EU487512) | 0.97 | 332 | 330 | 331* | ||
| K13b | KP780119 | Lactobacillus reuteri (L23507) | 0.85 | 336 | 333 | 333 | ||
| C11 | KP780117 | Bacteroides thetaiotaomicron (AE015928) | 0.98 | 383 | 381 | 338 | 339 | 381 |
| C7 | KP780118 | Alistipes finegoldii (AY643083) | 0.98 | 913 | 919 | 333 | 919 |
aPredicted from in silico digest with HaeIII by using REPK (v.1.3) [59]
bSecondary peaks produced by some clones in addition to the main peak.
n.o.—not observed
*Observed T-RF in T-RFLP of pooled samples was assumed to represent the respective clone as run-to-run variability of fragment size is expected to be ±1bp [60].
For detection of pairs of species sharing the same niche in relative proportions Person correlations were calculated (S3 Table). In crop samples L. salivarius was negatively correlated with L. crispatus, L. vaginalis and L. reuteri, however the last 3 species were positively correlated with each other (Fig 3, S3 Table). In the jejunum L. crispatus and L. reuteri were negatively correlated (Fig 3). Moreover, a higher abundance of L. crispatus was accompanied by a lower abundance of L. taiwanensis in this section (S3 Table). The resulting positive correlation between L. taiwanensis and L. reuteri observed in the jejunum was also found in the ileum. The negative correlation of L. salivarius and L. vaginalis detected in the crop was also observed in the ileum (S3 Table).
Fig 3. Draftsman plot showing the relative abundance (%) of one species-of-interest against another.
(A) Positive correlation in crop and (B) negative correlation in jejunum between L. crispatus and L. reuteri in all six dietary treatments.
Effect of diet on the microbial community structure within single sections of the GIT in broilers
The bacterial community structure within single sections of the GIT did not show significant effects of MCP or phytase supplementation in case of analyzing pooled samples with 454 pyrosequencing or T-RFLP (p>0.05) (S2 Fig). However, at family level results of 454 pyrosequencing indicated a higher abundance of Flavobacteriaceae in the crop digesta when no MCP was added to the diet (Fig 2, S4 Table). Moreover, supplementation of phytase led to an increasing abundance of Aeromonadaceae and Flavobacteriaceae and a decreasing abundance of Lactobacillaceae in the crop. No effect of MCP or phytase was detected in the jejunum. However, in the ileum, supplementation of phytase seemed to favour the abundance of Enterobacteriaceae while decreasing Lactobacillaceae in diets without MCP. The opposite was found in diets with MCP. In caecal samples Enterobacteriaceae were less prevalent and unclassified Clostridiales and Bacteroidaceae were more abundant when MCP was supplemented. In the absence of MCP, the addition of phytase led to a lower abundance of Erysipelotrichaceae and Lactobacillaceae and to a higher abundance of Bacteroidaceae.
PCoA for T-RFLP of single replicates revealed that more than 70% of total variation between bacterial community structures in crop samples are explained by PCo1 indicating a strong effect of MCP (Fig 4). This was also confirmed by ANOSIM (R = 0.291, p = 0.009). However, no effect of phytase was detected in crop samples. In the digesta of the jejunum no effects of MCP or phytase on bacterial community structures was found. In the case of the ileum a significant shift of the bacterial community composition with addition of phytase was observed as more than 55% of total variation was explained by PCo1 (Fig 4). This was also confirmed by ANOSIM (R = 0.229, p = 0.001). For caecal samples no significant effect of both dietary factors were observed but a possible trend for a change in the bacterial community structure with addition of phytase became evident by PCoA (Fig 4) as well as by ANOSIM (R = 0.136, p = 0.06).
Fig 4. PCoA ordination of the bacterial assembly of single replicates within each section of GIT.
Broilers were fed with different diets varying in supplementation of monocalcium phosphate: BD- (open circles) and BD+ (close circles) and different levels of phytase: 0 (black), 500 (red), 12,500 (blue) FTU/kg feed, and samples analyzed by T-RFLP: Crop (A), Jejunum (B), Ileum (C) and Caeca (D).
SIMPER analysis for T-RFLP of single replicates indicated a higher abundance of L. reuteri/L. vaginalis- (T-RF 62) and L. crispatus-type species (T-RF 244) in crop samples in the absence of MCP whereas for diets with addition of MCP L. salivarius- (T-RF 278 and 321) and L. taiwanensis-type phylotypes (T-RF 331) seemed to be more abundant. For the ileum increased abundances of species affiliated to L. salivarius (T-RF 278, 321 and 322) and L. taiwanensis (T-RF 331) with supplementation of phytase was shown whereas for diets without phytase L. crispatus-type species (T-RF 243 and 244) were favored.
Discussion
In the last decade 454-pyrosequencing became one of the most used method to depict microbial communities from a vast set of habitats [21, 36, 37]. However, it is still a costly technique if a large amount of samples needs to be analyzed. T-RFLP is an established fingerprinting technique that can characterize microbial communities rapidly and cost-efficiently [21]. To identify phylotypes by T-RFLP, clones with known sequences were used for an in silico and experimental restriction digestion. This enabled the assignment of different species and revealed the well-known problem of pseudo-T-RFs, which were shown for 12 of the clones here. These pseudo-T-RFs were probably caused by a partial amplicon digestion [38, 39]. Further work should be done in order to identify three unknown T-RFs detected in the caeca samples in abundances higher than 2.5%, which were not covered by existing clone libraries. Several studies with different sample sources have shown that T-RFLP is a suitable method that coupled with sequencing information gives a reliable insight into community profile [40–42]. Results from the present study confirmed that 454 pyrosequencing and T-RFLP have a strong correlation and revealed similar global results analyzing the 16S rRNA gene. As previously demonstrated with soil [21], nasopharyngeal [23] and rumen [24] samples, pyrosequencing had a better insight into the bacterial community. Nevertheless, T-RFLP was also able to distinguish the different sections of the GIT in broiler chickens and the same dominant species per sample were detected as those detected by pyrosequencing.
Independently of the diet, lactobacilli were the dominant colonizers of the crop, where a negative correlation between L. salivarius and L. crispatus was observed. In presence of in-feed antimicrobials L. crispatus increased its prevalence [43]. L. salivarius was highly abundant in the crop samples, its abundance decreased in the jejunum and ileum while L. crispatus became the most abundant microorganism. Previous studies have shown that L. crispatus inhibits the adhesion of avian pathogenic Escherichia coli [44]. Also, it has high amylase activity, which is a favorable effect on animal performance and feed conversion ratio [45]. Abbas Hilmi and colleagues have shown that L. reuteri was the most abundant lactobacillus species in the crop of 1-week old chicken decreasing its abundance in 5-week old chicken depending on the diet [46]. In the current study this microorganism was not the most abundant in the crop but its abundance decreased in diets supplemented with MCP. In addition, it showed a positive correlation with L. crispatus in the crop, but the opposite was found in the jejunum where a negative correlation was observed. In the present study, lactobacilli were detected in abundances lower than 1% in the caeca, which is in accordance with some published studies [43, 47, 48]. The caeca is the highest diverse section of the chicken GIT (9–12 fold more) and is mainly colonized by unknown or uncultured microorganisms. A great number of OTUs could not be assigned at the genus level. This might be related to the fact that most of our knowledge regarding intestinal samples came from human studies leaving other hosts not so well characterized and with absence of important information [49, 50].
Results from in vitro studies with ruminal bacteria have shown that microbes require a minimum of P for optimal fermentation [51]. Moreover, it was demonstrated that bacterial P and Ca assimilation and metabolic activity depend on P and Ca availability in the large intestine of pigs [52]. In the present study, a significant effect of dietary MCP or phytase was obtained by T-RFLP analysis of single replicates. In crop samples, a shift within Lactobacillales from L. salivarius- and L. taiwanensis- to L. reuteri/L. vaginalis- and L. crispatus-type phylotypes, when no MCP was added, was detected. Palacios and colleagues isolated phytase-producing lactobacilli from different sections of the GIT of broiler chickens [13]. L. reuteri, isolated from the gizzard, showed one of the highest phytate-degrading activity (600–1700 U/g protein at pH 5.0 and 7.2) [13]. Several L. crispatus strains isolated from crop and caeca of broiler chickens have also been shown to possess phytase activity [45]. The ability of utilizing phytate-bound P may explain the higher abundance of both species when animals were fed with phytate-rich diets without MCP. However, L. salivarius-type species isolated from the small intestine [13] and feces [53] of broiler chickens also had high phytate-degrading activities. Either these strains differ from those strains in the crop in their ability to degrade phytate or other factors such as changes in physicochemical properties of the digesta, play a role for the occurrence of L. salivarius-type species. Differences in pH and production of short chain fatty acids were observed in the crop of 42-day-old broiler chickens fed with low compared to adequate contents of P and Ca in diets [9]. Moreover, free Ca++ ions have been shown to considerably improve the attachment of L. salivarius isolated from the chicken GIT to immobilized chicken mucus in vitro [54] whereas the positive effect of Ca++ ions on in vitro adhesion of a L. reuteri isolate from pig feces to piglet jejunal epithelial cells was much lower than for other Lactobacillus sp. [55].
An effect of MCP on the bacterial community composition in the ileum or caeca of broilers was not detected by T-RFLP analysis in the present study whereas results on bacterial counts and fermentation products reported previously indicated shifts within the microbial community in these sections when feeding diets low or adequate in P and Ca [8, 9]. These different findings may result from differences in diet formulations, methodical approaches used for microbial community analysis or animal’s age.
A significant effect of phytase on the bacterial community composition was only observed in the ileum being restricted to L. salivarius-, L. taiwanensis- and L. crispatus-type phylotypes. Changes in concentrations of different inositol phosphate isomers resulting from effects of phytase on phytate degradation were reported in a companion study [15]. Phytate can also exert anti-nutritional effects through formation of complexes with proteins and or minerals. Hence, supplementation of phytase is associated with positive effects on the availability of different nutrients in digesta through increased phytate breakdown [5]. However, the enzyme mechanism that caused an increase in the abundance of the L. salivarius- and L. taiwanensis-type species and the decrease of L. crispatus is unknown. An effect of phytase on the abundance of L. reuteri was not found in the ileum. This is in accordance with previous findings in pig ileum samples [56]. However, total counts of lactobacilli in the ileum of broilers were increased upon supplementation of 500 or 5000 U [8, 9].
The possible trend for a change in the bacterial community structure with addition of phytase in caeca detected in the present study is in accordance with results of previous studies that showed changes in lactobacilli and Escherichia coli counts (8) or production of short chain fatty acids [9] in caeca of broilers when adding phytase to diet.
Studies on the bacterial community composition in the jejunum of broiler chickens as affected by diet are rare. Geier and colleagues demonstrated an effect of indigestible carbohydrates on the composition of the Lactobacillus community in the jejunum of 25-day-old broiler chickens [57]. However, Torok et al. detected no effect of a non-starch polysaccharide-degrading enzyme on the jejunal bacterial community composition in 22-day-old broiler chickens [58]. Likewise, no effect of the MCP or phytase on the bacterial community composition in the jejunum could be observed in the present study.
Conclusions
This is the first study showing that 454 pyrosequencing and T-RFLP can be used for analysis of the microbiota in broiler GIT. Results of both methods were highly correlated and revealed similar global results on bacterial communities found in crop, jejunum, ileum and caeca. Thus, we conclude that T-RFLP can be used as a reliable fingerprinting method to rapidly analyze large numbers of samples. Moreover, our results provide comprehensive taxonomic information on the bacterial community that is present in different sections of chicken’s GIT. To the best of our knowledge, we are the first having used such a high number of animals (72) to analyze the chicken’s microbiota considering the upper as well as the lower part of the GIT. Furthermore, this is the first report on effects of MCP and phytase on the microbiota in different sections of chicken’s GIT. Our data revealed a strong dietary effect on lactobacilli in crop and ileum samples. Shifts on different bacterial groups within the microbiota were also observed at family level. Hence, it can be concluded that MCP as well as phytase are modulators of the gut microbiota in chickens.
Supporting Information
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Comparison of PCoA plots for T-RFLP of pooled and 454-pyrosequencing results and samples per dietary treatment. Diets varied in supplementation of monocalcium phosphate: BD- (open circles) and BD+ (close circles) and different levels of phytase: 0 (black), 500 (red), 12,500 (blue) FTU/kg feed.
(TIFF)
(DOCX)
(DOCX)
(DOCX)
Diets differed in supplementation of monocalcium phosphate (BD-/BD+) and phytase (0, 500, 12,500 FTU/kg feed).
(DOCX)
Acknowledgments
The authors would like to thank Sabine Kleinsteuber, Ingo Fetzer and Frank Rasche for helpful discussions about the application and analysis of T-RFLP and pyrosequencing.
Data Availability
All relevant data are within the paper and its Supporting Information files. All sequences of clones were submitted to GenBank under the accession number KP780094-KP780131. Sequences obtained by 454 sequencing were submitted to European Nucleotide Archive under the study accession number PRJEB9198.
Funding Statement
This study was funded by the Ministerium für Wissenschaft, Forschung und Kultur des Landes Baden-Württemberg. MR and LEH received the funding. The funders had no role in study design, data collection and analysis, decision to publish, or preparation of the manuscript.
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Associated Data
This section collects any data citations, data availability statements, or supplementary materials included in this article.
Supplementary Materials
(TIFF)
Comparison of PCoA plots for T-RFLP of pooled and 454-pyrosequencing results and samples per dietary treatment. Diets varied in supplementation of monocalcium phosphate: BD- (open circles) and BD+ (close circles) and different levels of phytase: 0 (black), 500 (red), 12,500 (blue) FTU/kg feed.
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(DOCX)
(DOCX)
(DOCX)
Diets differed in supplementation of monocalcium phosphate (BD-/BD+) and phytase (0, 500, 12,500 FTU/kg feed).
(DOCX)
Data Availability Statement
All relevant data are within the paper and its Supporting Information files. All sequences of clones were submitted to GenBank under the accession number KP780094-KP780131. Sequences obtained by 454 sequencing were submitted to European Nucleotide Archive under the study accession number PRJEB9198.