- Research article
- Open Access
Gut microbiota in two recently diverged passerine species: evaluating the effects of species identity, habitat use and geographic distance
BMC Ecology and Evolution volume 21, Article number: 41 (2021)
It has been proposed that divergence in the gut microbiota composition between incipient species could contribute to their reproductive isolation. Nevertheless, empirical evidence for the role of gut microbiota in speciation is scarce. Moreover, it is still largely unknown to what extent closely related species in the early stages of speciation differ in their gut microbiota composition, especially in non-mammalian taxa, and which factors drive the divergence. Here we analysed the gut microbiota in two closely related passerine species, the common nightingale (Luscinia megarhynchos) and the thrush nightingale (Luscinia luscinia). The ranges of these two species overlap in a secondary contact zone, where both species occasionally hybridize and where interspecific competition has resulted in habitat use differentiation.
We analysed the gut microbiota from the proximal, middle and distal part of the small intestine in both sympatric and allopatric populations of the two nightingale species using sequencing of bacterial 16S rRNA. We found small but significant differences in the microbiota composition among the three gut sections. However, the gut microbiota composition in the two nightingale species did not differ significantly between either sympatric or allopatric populations. Most of the observed variation in the gut microbiota composition was explained by inter-individual differences.
To our knowledge, this is the first attempt to assess the potential role of the gut microbiota in bird speciation. Our results suggest that neither habitat use, nor geographical distance, nor species identity have strong influence on the nightingale gut microbiota composition. This suggests that changes in the gut microbiota composition are unlikely to contribute to reproductive isolation in these passerine birds.
Vertebrates harbour taxonomically and functionally diverse microbial communities in their intestines, referred to as the gut microbiota [1, 2]. It has been shown that the composition of the gut microbiota can have profound effects on the host’s physiology and morphology, as well as behaviour [3,4,5,6,7,8]. Moreover, between-species divergence in the gut microbiota composition could play a role in the establishment of reproductive isolation between species and thus in generating species diversity [6, 9, 10]. Despite recent intensive research on variation in the gut microbiota composition within and between vertebrate species [1, 11,12,13,14] the factors that generate the gut microbial diversity are still not sufficiently understood, especially in non-mammalian taxa. Additionally, it is largelly unknown how often closely related species differ in the gut microbiota composition and thus how widespread the effect of the gut microbiota in speciation.
Variation in the gut microbiota composition may arise due to multiple factors including differences in the host’s diet [15,16,17,18], habitat [19,20,21] or geographical range [22,23,24]. In addition, host genes involved in the management of the gut microbiota can play important roles in structuring gut microbial communities [25,26,27]. All these factors as well as a stable and long-lasting transfer of the gut microbiota from parents to progeny may generate divergence in the gut microbiota composition between species. However, the importance of specific factors in shaping gut microbiota diversity seems to differ among different vertebrate lineages .
Between-species divergence in the gut microbiota composition can contribute to the origin of reproductive isolation by multiple ways. First, host-associated microbiota may be involved in assortative mating and thus the establishment of pre-mating reproductive barriers [6, 9]. Furthermore, interactions between the host genome and the microbiome, between different microbes of the same metagenome, or between different host's genes involved in the management of microbial communities can be disrupted in hybrids . This can cause gut microbiota dysbiosis in hybrid individuals, which can reduce their fitness and contribute to postzygotic isolation [10, 12, 13].
Here we studied the gut microbiota variation in two closely related passerine bird species, the common nightingale (Luscinia megarhynchos) and the thrush nightingale (Luscinia luscinia). The two species diverged approximately 1.8 Mya  and their breeding areas currently overlap in a secondary contact zone spanning across Europe , where they occasionally hybridize. Both species are migratory and differ in their wintering grounds in sub-Saharan Africa . They both preferentially occupy dense shrubby vegetation (often close to water bodies) and feed mostly on insects [31, 32]. In allopatric regions they inhabit the same habitats, while in the sympatric region their habitat use and diet have partially differentiated, presumably to reduce interspecific competition [32,33,34]. Common nightingales in sympatry occur more frequently in dry habitats and feed mostly on Coleoptera, whereas thrush nightingales in sympatry prefer wet habitats and feed more often on Diptera . Given that the gut microbiota composition can rapidly shift depending on habitat and prevailing diet [20, 35], the gut microbiota may have differentiated between the two nightingale species in sympatry.
Rarely-occurring interspecific hybrids between the common nightingale and thrush nightingale are viable, but their relative fitness compared to the parental species has not yet been evaluated thoroughly. Nevertheless, it is known that following Haldane’s rule, F1 hybrid females are sterile while F1 hybrid males are fertile [36,37,38]. It has been also documented that backcross hybrids are rarely present in the sympatric population  and that gene flow can occur between the two species [29, 40].
To elucidate the factors shaping the gut microbiota variation in nightingales, we analysed the gut microbiota profiles in sympatric and allopatric populations of both species using high-throughput sequencing of bacterial 16S rRNA. Unlike most studies on vertebrate gut microbiota based on the analyses of faecal samples as a proxy for intestinal samples, we analysed the microbiota along the whole small intestine to obtain a more complex view of the gut microbiota composition in the two nightingale species. First, we tested whether the gut microbiota composition differs between the two species and whether there are any bacteria exhibiting host species specificity, which would suggest that the gut microbiota could potentially contribute to the reproductive isolation between the two nightingale species. Second, we compared the level of interspecific differences in the gut microbiota composition in sympatry and in allopatry. A higher divergence in sympatry would imply a stronger effect of habitat use or diet, while a higher divergence in allopatry would indicate a stronger effect of geographical region on the gut microbiota divergence [41, 42]. Similar levels of divergence in sympatry and allopatry would suggest that the divergence in host genes involved in the management of the gut microbiota and/or long-term transfer of the gut microbiota from parents to progeny may cause a divergence of the gut microbiota between the two nightingale species. To our knowledge, this study is the first to focus on the gut microbiota composition in a pair of closely related avian species with incomplete reproductive isolation, and to examine its variation in sympatric and allopatric populations. Our findings could have important implications for understanding the factors affecting variation in the gut microbiota composition in birds and the possible role of gut microbiota divergence in avian speciation.
We sequenced metagenomic DNA extracted from three sections of the small intestine in 18 individuals of the common nightingale (Luscinia megarhynchos, hereafter CN) and 18 individuals of the thrush nightingales (Luscinia luscinia, hereafter TN). In both species, half of the individuals came from the sympatric region and half from the allopatric region. The three sections of the small intestine were: (1) the duodenum (the proximal part of the small intestine, hereafter DU), (2) the jejunum (the middle part of the small intestine, hereafter JE), and (3) the ileum (the distal part of the small intestine before caecal protuberances, hereafter IL). In total, 108 samples were sequenced (three gut samples for each of the 36 individuals).
After the filtering steps, which included (1) removing low-quality sequences, chimeric sequences, sequences not consistently present in both technical duplicates for a given sample, and non-bacterial sequences (including especially reads from coccidia parasites) and (2) excluding samples with less than 1000 reads after all the filtering steps above (see Material and Methods for details), we obtained a final dataset consisting of 57 samples. These included 22 samples from CN (DU = 6, JE = 6 and IL = 10, together representing 12 individuals) and 35 samples from TN (DU = 10, JE = 10 and IL = 15, together representing 16 individuals) (Additional file 1: Table S1). These samples were covered by a total of 276,676 reads. The mean sequencing depth per sample was 4035 (range = 1036–10,261) in CN and 5,369 (range = 1041–14,740) in TN. In total, 272 Operational Taxonomic Units (OTUs) were identified, and the average number of OTUs per sample was 8.33 (range: 1–46). Twelve bacteria phyla and 126 genera were detected in the gut microbiome of the two nightingale species (Fig. 1).
The most common bacterial phyla were Firmicutes (57.95% of relative abundance, dominated by the genera Catellicoccus, Candidatus Arthromitus and Clostridium sensu stricto), Proteobacteria (30.49%, dominated by the genera Escherichia/Shigella and Rickettsiella), Tenericutes (6.60%, dominated by the genera Mycoplasma and Ureaplasma), Actinobacteria (1.99%, dominated by the genera Actinoplanes and Kocuria) and Bacteroidetes (1.76%, dominated by the genus Candidatus Cardinium). The relative abundance of all other bacterial phyla was less than 1% (Fig. 1). Regarding the gut sections, Firmicutes and Proteobacteria were the dominant bacterial phyla in all three-gut sections (Fig. 1). The presence of Tenericutes, Bacteroidetes, Actinobacteria and Chlamydia was largely individually specific (Fig. 1).
Differences in microbial α-diversity among gut sections, between species and regions
As estimates of microbial α-diversity, describing the diversity of the microbiome in each sample, we used the Chao1 diversity index (accounting for undetected rare OTUs), the number of observed OTUs and the Shannon diversity index. For all three measures of α-diversity, the microbial diversity was highest in IL (Fig. 2, Table 1 and Additional file 1: Table S2a). We then used linear mixed models (LMMs) to test for the effects of the gut section (i.e. DU, JE, IL), the nightingale species (i.e. CN and TN), geographical region (i.e. allopatry and sympatry) and the species-region interaction on the respective α-diversity indexes. The effect of individual was included as a random effect.
LMMs revealed a significant effect of the gut section on α-diversity for the log-transformed Chao1 index (p = 0.002, Tables 1 and Additional file 1: Table S2a, Fig. 2b) and for the log-transformed number of observed OTUs (p = 0.004, Tables 1 and Additional file 1: Table S2a, Fig. 2a), but not for the Shannon index (Table 1 and Additional file 1: Table S2a, Fig. 2a). Pairwise post-hoc Tukey tests on Chao1 index and the number of observed OTUs showed that α-diversity was significantly higher in IL compared to the JE for the log-Chao1 (p = 0.048). All other pairwise comparisons were, however, insignificant (Fig. 2 and Additional file 1: Table S2b).
Generally, α-diversity estimates were higher in TN (mean ± standard error (se): Chao1: 9.34 ± 0.37, Shannon: 0.96 ± 0.12, number of observed OTUs: 9.11 ± 1.44) than in CN (mean ± se: Chao1: 6.41 ± 0.30, Shannon: 0.73 ± 0.11, observed OTUs 6.18 ± 0.89). However, α-diversity was higher in TN samples compared to CN samples only in sympatry, not in allopatry (Fig. 3). Nevertheless, when taking into account the inter-individual variability, the effect of the species identity on α-diversity was not significant (LMMs: p > 0.05, Table 1). The effects of the region and the interaction between species identity were also insignificant (LMMs: p > 0.05, Table 1).
Differences in microbial composition (β-diversity) among gut sections
As measures of microbial composition dissimilarity between samples (β-diversity), we calculated two types of distances: the binary Jaccard distance and the Bray–Curtis distance. The binary Jaccard distance accounts for the presence/absence of OTUs and is thus more sensitive to gut-microbiota changes driven by rare OTUs. The Bray–Curtis distance accounts for differences in the OTUs’ relative abundance and is thus less sensitive to rare OTUs.
We detected within-individual correlations in microbial composition among the three gut sections (Mantel test: p < 0.05 for both distances; range of correlation coefficients is 0.91–0.96 for Bray–Curtis distance and 0.32—0.70 for Jaccard distance; Additional file 1: Table S3). The db-RDA analysis revealed significant differences in the microbiota composition among the three-gut sections for the Jaccard distance (F2, 54 = 0.775, p = 0.035) but not for the Bray–Curtis distance (F2, 54 = 0.658, p = 0.13). However, the variation in the gut microbiota composition explained by differences among gut sections was very low both for the Jaccard distance (adjusted – R2 = 0.028) and Bray–Curtis distance (adjusted – R2 = 0.024) (Fig. 4a, b).
Differences in microbial composition between the two species in sympatry and allopatry
The db-RDA showed no significant effect of species identity or region on the gut microbiota composition (Table 2, model complete) although it revealed a weak but significant interaction between species and regions for both distance matrices (Bray–Curtis distance: p = 0.034 and Jaccard distance: p = 0.043, Table 2, model complete). This may suggest either that the species differ in microbial composition only in sympatry or allopatry, or that some differences within the species may exist between allopatric and sympatric regions. We thus tested these possibilities using db-RDA models focusing separately on each of them. However, the models did not reveal any significant differences in microbial composition between the species in sympatry (Bray–Curtis distance: p = 0.055; Jaccard distance p = 0.078; Table 2) nor in allopatry (Bray–Curtis distance: p = 0.071, Table 2; Jaccard distance p = 0.051; Table 2), although some subtle differences may exist both in sympatry and allopatry (Fig. 4c, d). Moreover, we found no significant differences in microbial composition between allopatric and sympatric regions of CN (Bray–Curtis distance: p = 0.098; Jaccard distance: p = 0.096; Table 2) despite TN showing significant differences in the gut microbiota composition between the two regions for the Bray–Curtis distance (p = 0.014; Table 2).
The nested.anova.dbrda function indicated that the variability in the gut microbiota composition explained by species and region was 14% for the Bray–Curtis distance and 11% for the Jaccard distance, while individual identity explained 79% (Bray Curtis distance) and 67% (Jaccard distance) of the variability in gut microbiota composition (see Table 3).
Generalized linear mixed models (GLMMs) identified one OTU belonging to Clostridium sensu stricto genus (Firmicutes phylum) that was significantly differentially represented in the two nightingale species in sympatry (Additional file 1: Table S4a). This OTU was more abundant in CN samples than in TN samples. No OTU was significantly differentially represented in the two species in allopatry (Additional file 1: Table S4b). The same OTU belonging to Clostridium sensu stricto was also differentially represented between sympatric and allopatric regions of CN as well as TN, although in TN the difference was no longer significant after correcting for multiple testing (Additonal file 1: Table S5a, b). For both species, Clostridium sensu stricto was more abundant in sympatry than in allopatry (Additional file 1: Table S5).
Microbial communities living in vertebrate gastrointestinal tracts may affect the fitness-related phenotypic traits of their hosts [3, 43], which in turn may induce selection on mechanisms that ensure the acquisition and maintenance of beneficial microbes. This selection pressure often results in long-lasting stable associations between the host and particular gut microbiota species. As different host species can be co-adapted with different gut bacteria, it is commonly assumed that the gut microbiota can be significantly involved in reproductive isolation between species . However, despite intensive research on various aspects of host gut microbiota interactions over the past decades, empirical evidence for the role of gut microbiota in speciation is still limited and comes mainly from invertebrate taxa . In this study, we examined the gut microbiota composition of two recently diverged songbirds, the common nightingale and the thrush nightingale, in their allopatric and sympatric populations. To our knowledge, this is the first attempt to assess the potential role of gut microbiota in bird speciation.
We found no significant differences in the gut microbiota composition between the two nightingale species, with less than 14% of the total gut microbiota variation being attributed to interspecific dissimilarities. Furthermore, differential abundance analyses identified only a single OTU from the genus Clostridium with a significantly different representation between the two nightingale species. Nevertheless, this OTU, as well as other highly prevalent OTUs (e.g. Candidatus Arthromitus) were detected in both host species, meaning that none of the OTUs exhibited species specificity. Consequently, our results do not provide support for the existence of species-specific gut microbiota components, and it is thus unlikely that the gut microbiota might be involved in reproductive isolation between the two nightingale species.
Generally, evidence for the role of the host’s microbiota in the origin of reproductive isolation is limited. In various arthropod taxa, bacterial endosymbionts are involved in cytoplasmic incompatibilities . In some arthropods, divergence in the gut microbiome between species can contribute to the mortality of hybrid individuals . It is, however, unclear whether this gut microbiota-induced hybrid lethality arises as a consequence of host vs. gut microbiota incompatibilities or incompatibilities among individual microbial species or the host genes involved in the management of the gut microbiota . In Drosophila, the divergence of host-associated microbiota causes assortative mating between different Drosophila lineages [6, 9], with observed changes in mating preferences caused by changes in levels of cuticular hydrocarbon sex pheromones induced by symbiotic bacteria . In vertebrates, there are a few studies showing phylogenetic co-divergences between hosts and particular bacterial species, typically comprising just a limited fraction of their gut microbiota [10, 12, 45]. Nonetheless, a possible contribution of this gut microbiota divergence to the origin of prezygotic or postzygotic reproductive isolation between species has not yet been demonstrated.
Changes in the host’s gut microbiota can be caused by environmental changes, for example by shifts in the host’s diet or habitat [16, 21, 46]. Such ecological niche shifts associated with changes in the gut microbiota could theoretically also strengthen the degree of reproductive isolation between species. Our previous research documented that sympatric populations of common and thrush nightingales in their secondary contact zone exhibited higher divergence in habitat use  and bill morphology  compared to allopatric populations. This was consistent with observed interspecific differences in the consumed diet in sympatry . We expected that the greater ecological niche divergence in nightingale sympatric populations would be associated with a higher dissimilarity of their gut microbiota in sympatric compared to allopatric populations. Nevertheless, our data did not support this expectation, as interspecific gut microbiota differences were comparable in both sympatric and allopatric populations. This result corresponds to previous research that revealed a surprisingly low effect of diet and other ecological traits on interspecific gut microbiota variation in a set of bird species with much contrasting ecology than the nightingale species studied here [28, 47]. However, the absence of gut microbiota divergence between the two nightingale species in sympatry might also be a result of interspecific gene flow, as the reproductive isolation between the two species is still incomplete[29, 38, 40].
Previous studies have shown a decrease in gut microbiota similarity with increasing geographic distance in various vertebrates [42, 48, 49], suggesting that physical distance could produce barriers to bacterial dispersal. In mammals, species living in allopatry have more dissimilar gut microbiota compositions compared to sympatric species even when controlling for the diet and phylogenetic distance . Our results, showing similar divergence in microbial communities between sympatric and allopatric populations of the two nightingale species, indicate that compared to mammals, geographical distance may not have such a strong effect on the gut microbiota composition in passerine birds. This is generally consistent with previous studies on birds that found no or only weak associations between the gut microbiota composition and geographic distance [47, 49,50,51]. Nevertheless, as our study area (spanning approximately 600 km; Fig. 5) covered only a part of the two nightingale species geographic range extents, we cannot rule out that some differences in the gut microbiota composition in nightingales may exist over larger geographical distances. The weak effect of geographical distance on bird gut microbiota may be related to the fact that many species, including both our nightingale species, migrate for thousands of km each year to their wintering grounds . Such migrations may be linked with higher dispersal in birds compared to non-migratory vertebrates . In nightingales, natal and breeding dispersal are not known, but our unpublished capture-recapture data on adult birds indicate a high level of fidelity in both species. Males older than one year typically hold the same territories over multiple years. One-year-old males are more dispersive and often settle away from the site of their first breeding, but their movements are generally limited to 15 km, and we have never recorded a translocation over 20 km. Nightingales also show a high degree of migration connectivity . Additionally, a wide variety of habitats and foods utilized during migration itself appears to influence the gut microbiota composition , which may also contribute to the weak effect of geographical distance on bird gut microbiota.
While the species identity and geographical region explained only a small amount of the variability of the gut microbiota composition in nightingales (together 14%), individual identity explained more than 79% of the variability. This finding is congruent with other studies on passerine birds, with the gut microbiota typically exhibiting pronounced inter-individual variation [23, 49, 54]. The relatively high inter-individual variability in the gut microbiota composition and the small effect of diet, habitat and species identity on the gut microbiota composition in birds might be related to physiological and morphological adaptations associated with flight, as similar patterns in gut microbiota variation has been observed in bats, which also exhibit reduced intestine sizes and complexity, at least compared to other mammalian clades .
The gut microbiota composition in both nightingale species was dominated by the phyla Firmicutes (dominated by the genera Catellicoccus, Candidatus Arthromitus and Clostridium sensu stricto) and Proteobacteria (represented by the genera Escherichia/Shigella, Rickettsiella, and Pantoea) and was comparable with most passerines studies so far [55,56,57,58]. As we analysed the microbiota from three sections of the small intestine, our dataset also provides insight into gut microbiota variations along the digestive tract, which has been rarely studied in birds [51, 55]. We found significant differences in the microbiota composition among the three-gut sections in terms of the bacterial species’ presence/absence, but not in terms of the relative abundances of bacterial species. Nevertheless, the variation in the gut microbiota composition explained by differences among the gut sections was very low (2–3%). The three gut sections also differed in levels of microbial α-diversity, with the ileum—the most distal part of the small intestine—showing higher α-diversity compared to the duodenum and jejunum. The ileum typically maintains a more neutral pH and is responsible for absorption of the remaining products of digestion . We also detected significant within-individual correlations in microbial composition among the three gut sections. Generally, the gut microbiota profile of a particular gut section was more similar to any other gut section from the same individual than to the same gut section from a different individual, suggesting a considerable homogeneity in gut microbiota contents along the nightingale small intestine.
Our results suggest that neither the species identity, nor habitat, nor geographic distances have significant effects on the gut microbiota composition in the two nightingale species studied here. Instead, individual identity explains most of the observed variation in the gut microbiota composition. Our results are generally consistent with other studies in birds (e.g. ), and suggest that ecological factors, including diet and habitat, as well as geographical range do not have a strong influence on the avian gut microbiota composition. Altogether, this indicates that differences in gut microbiota in recently diverged bird species, especially if they are still connected by gene flow, might be usually too small to contribute to the origin of reproductive isolation. Differences in the gut microbiota composition between phylogenetically more distant avian species might arise at later stages of divergence, mostly as a consequence of the long-term independent evolution of species rather than the cause of speciation.
Study area and sampling
The sampling of common nightingales (Luscinia megarhynchos) and thrush nightingales (Luscinia luscinia) was carried out in Central Europe, in three regions (Fig. 5): an allopatric region for CN (south-western Poland), an allopatric region for TN (north-eastern Poland), and a sympatric region (central Poland) where the ranges of both species overlap and the species often locally co-occur . The allopatric region of CN was close to the sympatric region (Fig. 5); however, according to the Polish Breeding Bird Census data analysed in  as well as according to our long-term field observations, no TN individuals were recorded breeding in this area. Moreover, as the south-western edge of TN’s breeding range moved north-east recently (our unpublished observations), at the time of our sampling, CNs allopatric localities were not less than 100 km from the nearest breeding occurrence of TN. Both nightingale species were sampled in May 2018 at the beginning of the breeding season when territories were already established. Only male birds were caught using a mist net with a luring tape. We captured 9 CN and 9 TN males from allopatric regions and 9 CN and 9 TN males from the sympatric region. A list of the sampled birds, including their dates of sampling and GPS coordinates, is provided in Additional file 1: Table S1.
The birds were euthanized by standard cervical dislocation. Dissections started immediately; we removed the entire gastrointestinal tract from the body cavity, and gently separated intestines from the stomach. The whole gut tissue was then placed in a sterilized plastic tube (30 mL) with 99% ethanol, deep-frozen in liquid nitrogen and stored at − 80 °C until DNA extraction. The whole dissection procedure, starting with the euthanasia of the bird and finishing with the gut tissue being stored, did not exceed 8 min. All instruments used to dissect the birds (scissors, lancets) were repeatedly flame-sterilized to prevent cross-individual bacterial contamination of samples. The work with animals was approved by the General Directorate for Environmental Protection, Poland (permission no. DZP-WG.6401.03.123.2017.dl.3).
DNA extraction from the gut and 16S rRNA sequencing
From each individual’s gut, we dissected three samples (each ca. 0.5 cm long) from the small intestine using sterilized dissection tools. These sections were located in: (1) the duodenum (sampled from the proximal part of the small intestine), (2) the jejunum (sampled from the middle part of the small intestine) and (3) the ileum (the distal part of the small intestine before caecal protuberances). As the passerine colon is very short , we were unable to consistently dissect this gut part from all the intestine samples and thus the colon was not analysed in this study. Metagenomic DNA from each sample was extracted using the PowerSoil DNA isolation kit (MO BIO Laboratories Inc., USA). Both sample preparation and DNA extractions took place in a laminar flow cabinet. Sequencing libraries were prepared using a two-step PCR approach. The V3–V4 hypervariable region of bacterial 16S rRNA was amplified using universal primers S-D-Bact-0341-b-S-17 (CCTACGGGNGGCWGCAG) and S-D-Bact-0785-a-A-21 (GACTACHVGGGTATCTAATCC, ). Both forward and reverse primers were flanked by oligonucleotides compatible with Nextera adaptors (Illumina, USA). For the first PCR round, 5 μl of KAPA HIFI Hot Start Ready Mix (Kapa Biosystems, USA), 0.2 μM of each primer and 4.6 μl of DNA template were used (final reaction volume = 10 μl). PCR conditions were as follows: initial denaturation at 95 °C for 3 min followed by 30 cycles of 95 °C (30 s), 55 °C (30 s) and 72 °C (30 s), and a final extension at 72 °C (5 min). Dual-indexed Nextera sequencing adaptors were appended to the resulting PCR products during the second PCR. The second PCR reaction consisted of 10 μl of KAPA HIFI Hot Start Ready Mix, 5 μl of H2O, 2 μM of each primer and 1 μl of PCR product from the first PCR (final reaction volume = 20 μl) and the PCR program ran for 12 cycles with conditions being the same as during the first PCR. Products from the second PCR round were quantified by GenoSoft software (VWR International, Belgium) based on band intensities after electrophoresis on a 1.5% agarose gel, and mixed at equimolar concentration. The final library was cleaned up using SPRIselect beads (Beckman Coulter Life Sciences, USA). Products of desired size (520–750 bp) were extracted by PipinPrep (Sage Science Inc., USA) and sequenced on an Illumina Miseq (v3 kit, 300 bp paired-end reads). Technical PCR duplicates were sequenced for all individual DNA samples.
Bioinformatic processing of the sequence data and identification of microbial taxa
Samples were demultiplexed and primers were trimmed by skewer software . Using dada2 , we filtered out low-quality sequences (expected number of errors per read less than 1), denoised the quality-filtered fastq files and constructed an abundance matrix representing reads counts for individual haplotypes (Operational Taxonomic Units, OTUs) in each sample. Using uchime  and the gold.fna database (available at https://drive5.com/uchime/gold.fa), we identified chimeric sequences and removed them from the abundance matrix. Taxonomic assignation of haplotypes was conducted by the RDP classifier (80% confidence threshold ) and Silva reference database (v 132 ).
A large number of sequences from coccidian protozoa, an intracellular parasite present in the intestinal tract of vertebrates provoking Coccidiosis disease , were identified in TN samples (43% of the total number of reads) and in CN samples (38% of the total number of reads). These OTUs belonged to the genera Eimeria and Neospora (phylum: Apicomplexa). We removed all coccidian and other non-bacterial OTUs from the dataset. Furthermore, to eliminate PCR or sequencing artefacts that were not corrected by dada2, we removed all OTUs that were not consistently present in both technical duplicates for a given sample. Read counts for remaining OTUs were subsequently merged for the purpose of all later analyses. Finally, samples with less than 1,000 sequences after all the above filtering steps were discarded. In total, 19 samples from TN and 32 samples from CN were removed.
All statistical analyses were done using packages running under R Statistical Software version 3.4.3 (R Core Team 2015). To account for uneven sequencing depth among samples, a rarefied OTU table (n = 1,036 sequences per sample, which corresponds to the minimal per-sample sequencing depth) was used in all analyses, if not stated otherwise.
Estimation and comparison of microbial α-diversity
The three α-diversity estimates, including the Chao1 diversity index, the number of observed OTUs and the Shannon diversity index, were calculated using the phyloseq package . LMMs testing the effects of gut section, nightingale species and geographical region on the respective α-diversity indexes were performed in the package lme4 . To account for statistical non-independence (due to sampling of three gut sections for each individual), the effect of individual was included as a random effect. Differences between the gut sections were assessed based on Tukey post-hoc comparisons.
Dissimilarity of microbial composition (β-diversity) between samples
Two types of distances, the binary Jaccard distance and the Bray-Curtis distance, were calculated as measures of microbial composition dissimilarity between samples (β-diversity) using the vegan package .We used a Principal Coordinates Analysis (PCoA) based on the two distance matrices to visualize the differences in microbial composition among the three gut sections across both species. Associations between gut-microbiota composition and gut section were assessed by distance-based redundancy analyses (db-RDAs ) with the distance matrix as a response variable and the gut section identity (i.e. DU, JE and IL) as explanatory variables. The significance was assessed by a permutation-based ANOVA, with individual identity being considered as a block (i.e. ‘strata’) for permutation. Additionally, for individuals where all three-gut sections were available (n = 11, Additional file 1: Table S1), within-individual correlations of the microbial composition among the three-gut sections was evaluated using a Mantel’s test (R package ‘ade4’ ).
The effects of species identity (i.e. CN and TN) and region (i.e. sympatry and allopatry) on the gut-microbiota composition were assessed via db-RDA. The distance matrix was included as a response variable while nightingale species identity, region and their interaction were included as explanatory variables. The significance of explanatory variables in db-RDAs was assessed by a permutation-based ANOVA. In contrast to the analysis of the gut section, here explanatory variables associated with each individual (i.e. region, species identity) were reshuffled across blocks of individual‐specific samples during the permutation routine to account for the fact that multiple samples for each individual were analysed. To estimate the proportion of the variability explained by each factor on the gut microbiota composition, we used a nested analysis of variance via distance-based redundancy analysis (nested.anova.dbrda; package BiodiversityR ). The distance matrices were the response variable, while species identity, region and individual identity were explanatory variables (1000 permutations). To avoid any potential bias due to all three gut sections not being available for some individuals, we also ran this analysis on the subset of individuals (n=11) for which all three gut sections were available. The results were similar for both datasets and we thus present the results only for the whole dataset.
To identify specific OTUs whose abundances differed between the nightingale species in allopatric and sympatric regions, we used generalized linear mixed models with a negative binomial distribution . These analyses were performed on a subset of six OTUs (comprising 43% of all high quality reads) that were detected in at least five samples across both species and regions. The response variable was entered either as (i) the read counts for OTUs from the allopatric region or (ii) the read counts for OTUs from the sympatric region. The explanatory variable was the species identity, and individual identity was set as a random factor. Log-transformed total number of reads per sample was specified as the model offset. A false discovery rate method  was subsequently used to account for false discoveries due to multiple tests conducted on the given set of OTUs.
Availability of data and materials
Sequencing data are available from the European Nucleotide Archive under the study accession number: PRJEB43057. Metadata to the individual sequence samples are provided in the Supplementary Material Table S6. All other data are attached as a Supplementary Material.
Operational taxonomic unit
Linear mixed model
Principal coordinates analysis
Distance-based redundancy analyses
General mixed model
Analysis of variance
Polymerase chain reaction
Ley RE, Hamady M, Lozupone C, Turnbaugh PJ, Ramey RR, Bircher JS, et al. Evolution of mammals and their gut microbes. Science. 2008;320:1647–51. https://0-doi-org.brum.beds.ac.uk/10.1126/science.1155725.
Qin J, Li R, Raes J, Arumugam M, Burgdorf KS, Manichanh C, et al. A human gut microbial gene catalogue established by metagenomic sequencing. Nature. 2010;464:59–65. https://0-doi-org.brum.beds.ac.uk/10.1038/nature08821.
Kohl KD. Diversity and function of the avian gut microbiota. J Comp Physiol B. 2012;182:591–602. https://0-doi-org.brum.beds.ac.uk/10.1007/s00360-012-0645-z.
David LA, Maurice CF, Carmody RN, Gootenberg DB, Button JE, Wolfe BE, et al. Diet rapidly and reproducibly alters the human gut microbiome. Nature. 2014;505:559–63. https://0-doi-org.brum.beds.ac.uk/10.1038/nature12820.
Poulsen M, Hu H, Li C, Chen Z, Xu L, Otani S, et al. Complementary symbiont contributions to plant decomposition in a fungus-farming termite. Proc Natl Acad Sci. 2014;111:14500–5. https://0-doi-org.brum.beds.ac.uk/10.1073/pnas.1319718111.
Shropshire JD, Bordenstein SR. Speciation by symbiosis: the microbiome and behavior. MBio. 2016;7:1–11. https://0-doi-org.brum.beds.ac.uk/10.1128/mBio.01785-15.
Davidson GL, Cooke AC, Johnson CN, Quinn JL. The gut microbiome as a driver of individual variation in cognition and functional behaviour. Philos Trans R Soc B Biol Sci. 2018;373:20170286. https://0-doi-org.brum.beds.ac.uk/10.1098/rstb.2017.0286.
Suzuki TA, Martins FM, Phifer-Rixey M, Nachman MW. The gut microbiota and Bergmann’s rule in wild house mice. Mol Ecol. 2020;29:2300–11. https://0-doi-org.brum.beds.ac.uk/10.1111/mec.15476.
Sharon G, Segal D, Ringo JM, Hefetz A, Zilber-Rosenberg I, Rosenberg E. Commensal bacteria play a role in mating preference of Drosophila melanogaster. Proc Natl Acad Sci. 2010;107:20051–6. https://0-doi-org.brum.beds.ac.uk/10.1073/pnas.1009906107.
Moeller AH, Gomes-Neto JC, Mantz S, Kittana H, Segura Munoz RR, Schmaltz RJ, et al. Experimental evidence for adaptation to species-specific gut microbiota in house mice. mSphere. 2019;4:1–10. https://0-doi-org.brum.beds.ac.uk/10.1128/mSphere.00387-19.
Grond K, Sandercock BK, Jumpponen A, Zeglin LH. The avian gut microbiota: community, physiology and function in wild birds. J Avian Biol. 2018;49:e01788. https://0-doi-org.brum.beds.ac.uk/10.1111/jav.01788.
Wang J, Kalyan S, Steck N, Turner LM, Harr B, Künzel S, et al. Analysis of intestinal microbiota in hybrid house mice reveals evolutionary divergence in a vertebrate hologenome. Nat Commun. 2015;6:6440. https://0-doi-org.brum.beds.ac.uk/10.1038/ncomms7440.
Brucker RM, Bordenstein SR. Speciation by symbiosis. Trends Ecol Evol. 2012;27:443–51. https://0-doi-org.brum.beds.ac.uk/10.1016/j.tree.2012.03.011.
Brucker RM, Bordenstein SR. The hologenomic basis of speciation: gut bacteria cause hybrid lethality in the genus Nasonia. Science. 2013;341:667–9. https://0-doi-org.brum.beds.ac.uk/10.1126/science.1240659.
Hicks AL, Lee KJ, Couto-Rodriguez M, Patel J, Sinha R, Guo C, et al. Gut microbiomes of wild great apes fluctuate seasonally in response to diet. Nat Commun. 2018;9:1786. https://0-doi-org.brum.beds.ac.uk/10.1038/s41467-018-04204-w.
Keenan SW, Engel AS, Elsey RM. The alligator gut microbiome and implications for archosaur symbioses. Sci Rep. 2013;3:2877. https://0-doi-org.brum.beds.ac.uk/10.1038/srep02877.
Lewis WB, Moore FR, Wang S. Changes in gut microbiota of migratory passerines during stopover after crossing an ecological barrier. Auk. 2017;134:137–45. https://0-doi-org.brum.beds.ac.uk/10.1642/AUK-16-120.1.
Michel AJ, Ward LM, Goffredi SK, Dawson KS, Baldassarre DT, Brenner A, et al. The gut of the finch: uniqueness of the gut microbiome of the Galápagos vampire finch. Microbiome. 2018;6:167. https://0-doi-org.brum.beds.ac.uk/10.1186/s40168-018-0555-8.
Loo WT, Dudaniec RY, Kleindorfer S, Cavanaugh CM. An inter-island comparison of Darwin’s finches reveals the impact of habitat, host phylogeny, and island on the gut microbiome. PLoS ONE. 2019;14:e0226432. https://0-doi-org.brum.beds.ac.uk/10.1371/journal.pone.0226432.
Teyssier A, Rouffaer LO, Saleh Hudin N, Strubbe D, Matthysen E, Lens L, et al. Inside the guts of the city: Urban-induced alterations of the gut microbiota in a wild passerine. Sci Total Environ. 2018;612:1276–86. https://0-doi-org.brum.beds.ac.uk/10.1016/j.scitotenv.2017.09.035.
Phillips JN, Berlow M, Derryberry EP. The Effects of landscape urbanization on the gut microbiome: an exploration into the gut of urban and rural White-crowned sparrows. Front Ecol Evol. 2018;6:1–10. https://0-doi-org.brum.beds.ac.uk/10.3389/fevo.2018.00148.
Gaona O, Cerqueda-García D, Moya A, Neri-Barrios X, Falcón LI. Geographical separation and physiology drive differentiation of microbial communities of two discrete populations of the bat Leptonycteris yerbabuenae. Microbiologyopen. 2020;9:1113–27. https://0-doi-org.brum.beds.ac.uk/10.1002/mbo3.1022.
Grond K, Santo Domingo JW, Lanctot RB, Jumpponen A, Bentzen RL, Boldenow ML, et al. Composition and drivers of gut microbial communities in arctic-breeding shorebirds. Front Microbiol. 2019;10:2258. https://0-doi-org.brum.beds.ac.uk/10.3389/fmicb.2019.02258.
Gillingham MAF, Béchet A, Cézilly F, Wilhelm K, Rendón-Martos M, Borghesi F, et al. Offspring microbiomes differ across breeding sites in a panmictic species. Front Microbiol. 2019;10:1–16. https://0-doi-org.brum.beds.ac.uk/10.3389/fmicb.2019.00035.
Org E, Parks BW, Joo JWJ, Emert B, Schwartzman W, Kang EY, et al. Genetic and environmental control of host-gut microbiota interactions. Genome Res. 2015;25:1558–69. https://0-doi-org.brum.beds.ac.uk/10.1101/gr.194118.115.
Suzuki TA, Phifer-Rixey M, Mack KL, Sheehan MJ, Lin D, Bi K, et al. Host genetic determinants of the gut microbiota of wild mice. Mol Ecol. 2019. https://0-doi-org.brum.beds.ac.uk/10.1111/mec.15139.
Kubinak JL, Stephens WZ, Soto R, Petersen C, Chiaro T, Gogokhia L, et al. MHC variation sculpts individualized microbial communities that control susceptibility to enteric infection. Nat Commun. 2015;6:8642. https://0-doi-org.brum.beds.ac.uk/10.1038/ncomms9642.
Song SJ, Sanders JG, Delsuc F, Metcalf J, Amato K, Taylor MW, et al. Comparative analyses of vertebrate gut microbiomes reveal convergence between birds and bats. MBio. 2020;11:1–14. https://0-doi-org.brum.beds.ac.uk/10.1128/mBio.02901-19.
Storchová R, Reif J, Nachman MW. Female heterogamety and speciation: reduced introgression of the Z chromosome between two species of nightingales. Evolution (N Y). 2010;64:456–71. https://0-doi-org.brum.beds.ac.uk/10.1111/j.1558-5646.2009.00841.x.
Sorjonen J. Mixed singing and interspecific territoriality - consequences of secondary contact of two ecologically and morphologically similar nightingale species in europe. Ornis Scand. 1986;17:53. https://0-doi-org.brum.beds.ac.uk/10.2307/3676753.
Cramp S, Brooks DJ. Handbook of the birds of Europe, the Middle East and North Africa. The birds of the western Palearctic, vol. VI. Warblers. Oxford University. 1992.
Sottas C, Reif J, Kreisinger J, Schmiedová L, Sam K, Osiejuk TS, et al. Tracing the early steps of competition-driven eco-morphological divergence in two sister species of passerines. Evol Ecol. 2020. https://0-doi-org.brum.beds.ac.uk/10.1007/s10682-020-10050-4.
Reif J, Reifová R, Skoracka A, Kuczyński L. Competition-driven niche segregation on a landscape scale: evidence for escaping from syntopy towards allotopy in two coexisting sibling passerine species. J Anim Ecol. 2018;87:774–86.
Sottas C, Reif J, Kuczyński L, Reifová R. Interspecific competition promotes habitat and morphological divergence in a secondary contact zone between two hybridizing songbirds. J Evol Biol. 2018;31:914–23. https://0-doi-org.brum.beds.ac.uk/10.1111/jeb.13275.
Xue Z, Zhang W, Wang L, Hou R, Zhang M, Fei L, et al. The bamboo-eating giant panda harbors a carnivore-like gut microbiota, with excessive seasonal variations. MBio. 2015;6:1–12. https://0-doi-org.brum.beds.ac.uk/10.1128/mBio.00022-15.
Stadie C. Erdsanger I; Nachtigall und Sprosser. Eur Vogelwelt Vogelwelt. 1991;3:130–89.
Reifová R, Kverek P, Reif J. The first record of a female hybrid between the Common Nightingale (Luscinia megarhynchos) and the Thrush Nightingale (Luscinia luscinia) in nature. J Ornithol. 2011;152:1063–8.
Mořkovský L, Janoušek V, Reif J, Rídl J, Pačes J, Choleva L, et al. Genomic islands of differentiation in two songbird species reveal candidate genes for hybrid female sterility. Mol Ecol. 2018;27:949–58. https://0-doi-org.brum.beds.ac.uk/10.1111/mec.14479.
Reifová R, Reif J, Antczak M, Nachman MW. Ecological character displacement in the face of gene flow: evidence from two species of nightingales. BMC Evol Biol. 2011;11:138. https://0-doi-org.brum.beds.ac.uk/10.1186/1471-2148-11-138.
Janoušek V, Fischerová J, Mořkovský L, Reif J, Antczak M, Albrecht T, et al. Postcopulatory sexual selection reduces Z-linked genetic variation and might contribute to the large Z effect in passerine birds. Heredity. 2019;122:622–35. https://0-doi-org.brum.beds.ac.uk/10.1038/s41437-018-0161-3.
Moeller AH, Suzuki TA, Lin D, Lacey EA, Wasser SK, Nachman MW. Dispersal limitation promotes the diversification of the mammalian gut microbiota. Proc Natl Acad Sci. 2017;114:13768–73. https://0-doi-org.brum.beds.ac.uk/10.1073/pnas.1700122114.
Linnenbrink M, Wang J, Hardouin EA, Künzel S, Metzler D, Baines JF. The role of biogeography in shaping diversity of the intestinal microbiota in house mice. Mol Ecol. 2013;22:1904–16. https://0-doi-org.brum.beds.ac.uk/10.1111/mec.12206.
Hird SM. Evolutionary biology needs wild microbiomes. Front Microbiol. 2017;8:1–10. https://0-doi-org.brum.beds.ac.uk/10.3389/fmicb.2017.00725.
Lindsey ARI, Rice DW, Bordenstein SR, Brooks AW, Bordenstein SR, Newton ILG. Evolutionary genetics of cytoplasmic incompatibility genes cifA and cifB in prophage WO of Wolbachia. Genome Biol Evol. 2018;10:434–51. https://0-doi-org.brum.beds.ac.uk/10.1093/gbe/evy012.
Trevelline BK, Sosa J, Hartup BK, Kohl KD. A bird’s-eye view of phylosymbiosis: weak signatures of phylosymbiosis among all 15 species of cranes. Proc R Soc B Biol Sci. 2020;287:20192988. https://0-doi-org.brum.beds.ac.uk/10.1098/rspb.2019.2988.
Youngblut ND, Reischer GH, Walters W, Schuster N, Walzer C, Stalder G, et al. Host diet and evolutionary history explain different aspects of gut microbiome diversity among vertebrate clades. Nat Commun. 2019;10:2200. https://0-doi-org.brum.beds.ac.uk/10.1038/s41467-019-10191-3.
Kropáčková L, Těšický M, Albrecht T, Kubovčiak J, Čížková D, Tomášek O, et al. Codiversification of gastrointestinal microbiota and phylogeny in passerines is not explained by ecological divergence. Mol Ecol. 2017;26:5292–304. https://0-doi-org.brum.beds.ac.uk/10.1111/mec.14144.
Suzuki TA, Worobey M. Geographical variation of human gut microbial composition. Biol Lett. 2014;10:20131037. https://0-doi-org.brum.beds.ac.uk/10.1098/rsbl.2013.1037.
Hird SM, Carstens BC, Cardiff SW, Dittmann DL, Brumfield RT. Sampling locality is more detectable than taxonomy or ecology in the gut microbiota of the brood-parasitic Brown-headed Cowbird (Molothrus ater). PeerJ. 2014;2:e321. https://0-doi-org.brum.beds.ac.uk/10.7717/peerj.321.
Banks JC, Cary SC, Hogg ID. The phylogeography of Adelie penguin faecal flora. Environ Microbiol. 2009;11:577–88. https://0-doi-org.brum.beds.ac.uk/10.1111/j.1462-2920.2008.01816.x.
Hird SM, Sánchez C, Carstens BC, Brumfield RT. Comparative gut microbiota of 59 neotropical bird species. Front Microbiol. 2015. https://0-doi-org.brum.beds.ac.uk/10.3389/fmicb.2015.01403.
Pigot AL, Tobias JA. Dispersal and the transition to sympatry in vertebrates. Proc R Soc B Biol Sci. 2015;282:20141929. https://0-doi-org.brum.beds.ac.uk/10.1098/rspb.2014.1929.
Hahn S, Amrhein V, Zehtindijev P, Liechti F. Strong migratory connectivity and seasonally shifting isotopic niches in geographically separated populations of a long-distance migrating songbird. Oecologia. 2013;173:1217–25. https://0-doi-org.brum.beds.ac.uk/10.1007/s00442-013-2726-4.
Kropáčková L, Pechmanová H, Vinkler M, Svobodová J, Velová H, Těšičký M, et al. Variation between the oral and faecal microbiota in a free-living passerine bird, the great tit (Parus major). PLoS ONE. 2017;12:e0179945. https://0-doi-org.brum.beds.ac.uk/10.1371/journal.pone.0179945.
Bodawatta KH, Sam K, Jønsson KA, Poulsen M. Comparative analyses of the digestive tract microbiota of new guinean passerine birds. Front Microbiol. 2018;9:1–13. https://0-doi-org.brum.beds.ac.uk/10.3389/fmicb.2018.01830.
Lewis WB, Moore FR, Wang S. Characterization of the gut microbiota of migratory passerines during stopover along the northern coast of the Gulf of Mexico. J Avian Biol. 2016;47:659–68. https://0-doi-org.brum.beds.ac.uk/10.1111/jav.00954.
García-Amado MA, Shin H, Sanz V, Lentino M, Martínez LM, Contreras M, et al. Comparison of gizzard and intestinal microbiota of wild neotropical birds. PLoS ONE. 2018;13:e0194857. https://0-doi-org.brum.beds.ac.uk/10.1371/journal.pone.0194857.
Berlow M, Kohl KD, Derryberry EP. Evaluation of non-lethal gut microbiome sampling methods in a passerine bird. Ibis (Lond 1859). 2020;162:911–23. https://0-doi-org.brum.beds.ac.uk/10.1111/ibi.12807.
Zhang Y, Simon SE, Johnson JA, Allen MS. Spatial microbial composition along the gastrointestinal tract of captive Attwater’s prairie chicken. Microb Ecol. 2017;73:966–77. https://0-doi-org.brum.beds.ac.uk/10.1007/s00248-016-0870-1.
Klindworth A, Pruesse E, Schweer T, Peplies J, Quast C, Horn M, et al. Evaluation of general 16S ribosomal RNA gene PCR primers for classical and next-generation sequencing-based diversity studies. Nucleic Acids Res. 2013;41:e1–e1. https://0-doi-org.brum.beds.ac.uk/10.1093/nar/gks808.
Jiang H, Lei R, Ding S-W, Zhu S. Skewer: a fast and accurate adapter trimmer for next-generation sequencing paired-end reads. BMC Bioinform. 2014;15:182. https://0-doi-org.brum.beds.ac.uk/10.1186/1471-2105-15-182.
Callahan BJ, McMurdie PJ, Rosen MJ, Han AW, Johnson AJA, Holmes SP. DADA2: High-resolution sample inference from Illumina amplicon data. Nat Methods. 2016;13:581–3. https://0-doi-org.brum.beds.ac.uk/10.1038/nmeth.3869.
Edgar RC, Haas BJ, Clemente JC, Quince C, Knight R. UCHIME improves sensitivity and speed of chimera detection. Bioinformatics. 2011;27:2194–200. https://0-doi-org.brum.beds.ac.uk/10.1093/bioinformatics/btr381.
Wang Q, Garrity GM, Tiedje JM, Cole JR. Naïve bayesian classifier for rapid assignment of rRNA sequences into the new bacterial taxonomy. Appl Environ Microbiol. 2007;73:5261–7. https://0-doi-org.brum.beds.ac.uk/10.1128/AEM.00062-07.
Quast C, Pruesse E, Yilmaz P, Gerken J, Schweer T, Yarza P, et al. The SILVA ribosomal RNA gene database project: improved data processing and web-based tools. Nucleic Acids Res. 2013;41:D590–6. https://0-doi-org.brum.beds.ac.uk/10.1093/nar/gks1219.
Knight A, Ewen JG, Brekke P, Santure AW. The evolutionary biology, ecology and epidemiology of Coccidia of Passerine birds. Adv Parasitol. 2018;99:35–60. https://0-doi-org.brum.beds.ac.uk/10.1016/bs.apar.2018.01.001.
McMurdie PJ, Holmes S. Phyloseq: an R package for reproducible interactive analysis and graphics of microbiome census data. PLoS ONE. 2013;8:e61217.
Bates D, Mächler M, Bolker B, Walker S. Fitting linear mixed-effects models using lme4. J Stat Softw. 2015. https://0-doi-org.brum.beds.ac.uk/10.18637/jss.v067.i01.
Oksanen AJ, Blanchet GF, Friendly M, Kindt R, Legendre P, Mcglinn D, et al. The vegan package. Community Ecol Packag. 2016;10:631–7.
Legendre P, Andersson MJ. Distance-based redundancy analysis: testing multispecies responses in multifactorial ecological experiments. Ecol Monogr. 1999;69:1–24.
Dray S, Dufour A-B. The ade4 package: implementing the duality diagram for ecologists. J Stat Softw. 2007;22:1–20. https://0-doi-org.brum.beds.ac.uk/10.18637/jss.v022.i04.
Kindt R, Coe R. Tree diversity analysis: a manual and software for common statistical methods for ecological and biodiversity studies. World Agroforestry Centre; 2005.
Brooks ME, Kristensen K, van Benthem KJ, Magnusson A, Berg CW, Nielsen A, et al. GlmmTMB balances speed and flexibility among packages for zero-inflated generalized linear mixed modeling. R J. 2017;9:378. https://0-doi-org.brum.beds.ac.uk/10.32614/RJ-2017-066.
Benjamini Y, Hochberg Y. Controlling the false discovery rate: a practical and powerful approach to multiple testing. J R Stat Soc. 1995;57:289–300.
We acknowledge the CF Genomics of CEITEC supported by the NCMG research infrastructure (LM2018132 funded by MEYS CR) for their support with obtaining scientific data presented in this paper. Computational resources were supplied by the project ‘e-Infrastruktura CZ’ (e-INFRA LM2018140) provided within the program Projects of Large Research, Development and Innovations Infrastructures. Access to computing and storage facilities owned by parties and projects contributing to the National Grid Infrastructure MetaCentrum, provided under the programme ‘Projects of Large Infrastructure for Research, Development, and Innovations’ (LM2010005), is greatly appreciated. We also thank Manon Poignet and Lucie Baránková for their assistance in the field and members of the population and speciation genetics group for their useful comments on the previous versions of this manuscript.
This work was supported by the student grant of the Grant Agency of Charles University [462/2017 to C.S.], a grant of the Czech Science Foundation [18–14325S to R.R. and T.A.] and the Charles University grant [PRIMUS/19/SCI/008 to R.R.].
Ethics approval and consent to participate
The work with animals was approved by the General Directorate for Environmental Protection, Poland (permission no. DZP-WG.6401.03.123.2017.dl.3).
Consent for publication
The authors declare that they have no competing interests.
Springer Nature remains neutral with regard to jurisdictional claims in published maps and institutional affiliations.
A list of sampled nightingale individuals with information about their species, geographical region, date of sampling and GPS coordinates. Table S2. α-diversity in the three gut sections across both nightingale species (a) and pairwise post-hoc Tukey tests of differences in α-diversity between specific gut sections (b) Table S3. Within-individual correlations in the microbial composition among the three-gut sections. Table S4. Differences in representation of particular OTUs between the two nightingale species in sympatry (a) and in allopatry (b). Table S5. Differences in representation of particular OTUs between sympatric and allopatric region in the common nightingale (a) and in the thrush nightingale (b). Table S6. Metadata to the individual sequence samples that are available from the European Nucleotide Archive under the study accession number: PRJEB43057.
About this article
Cite this article
Sottas, C., Schmiedová, L., Kreisinger, J. et al. Gut microbiota in two recently diverged passerine species: evaluating the effects of species identity, habitat use and geographic distance. BMC Ecol Evo 21, 41 (2021). https://0-doi-org.brum.beds.ac.uk/10.1186/s12862-021-01773-1
- Gut microbiome
- Reproductive isolation
- Habitat use