ORIGINAL RESEARCH article
Sec. Plant Pathogen Interactions
Volume 9 - 2018 | https://doi.org/10.3389/fmicb.2018.01187
Dissecting Community Structure in Wild Blueberry Root and Soil Microbiome
- 1Department of Plant, Food, and Environmental Sciences, Dalhousie University, Truro, NS, Canada
- 2Department of Microbiology and Immunology, Dalhousie University, Halifax, NS, Canada
- 3Department of Pharmacology, Dalhousie University, Halifax, NS, Canada
A complex network of functions and symbiotic interactions between a eukaryotic host and its microbiome is a the foundation of the ecological unit holobiont. However, little is known about how the non-fungal eukaryotic microorganisms fit in this complex network of host–microbiome interactions. In this study, we employed a unique wild blueberry ecosystem to evaluate plant-associated microbiota, encompassing both eukaryotic and bacterial communities. We found that, while soil microbiome serves as a foundation for root microbiome, plant-influenced species sorting had stronger effect on eukaryotes than on bacteria. Our study identified several fungal and protist taxa, which are correlated with decreased fruit production in wild blueberry agricultural ecosystems. The specific effect of species sorting in root microbiome resulted in an increase in relative abundance of fungi adapted to plant-associated life-style, while the relative abundance of non-fungal eukaryotes was decreased along the soil-endosphere continuum in the root, probably because of low adaptation of these microorganisms to host–plant defense responses. Analysis of community correlation networks indicated that bacterial and eukaryotic interactions became more complex along the soil-endosphere continuum and, in addition to extensive mutualistic interactions, co-exclusion also played an important role in shaping wild blueberry associated microbiome. Our study identified several potential hub taxa with important roles in soil fertility and/or plant–microbe interaction, suggesting the key role of these taxa in the interconnection between soils and plant health and overall microbial community structure. This study also provides a comprehensive view of the role of non-fungal eukaryotes in soil ecosystem.
Plant health and development are fundamentally dependent on the interaction between host and its microbiome. Plants are no longer considered single organisms, but rather dynamic entities comprising both plants and microbiota with complex interactions and functions (Zilber-Rosenberg and Rosenberg, 2008; Vandenkoornhuyse et al., 2015). The recruitment of the plant microbiota suggests a gradual enrichment of soil microbial community (species sorting) through several habitats toward a defined subset of microorganisms occupying internal plant tissue, the endosphere (Vandenkoornhuyse et al., 2015). These habitats are distinguished by physical proximity to the plant and the level of host’s influence on microbial communities. These habitats, from least to most proximal, include bulk soil, the rhizosphere (the thin layer of soil surrounding roots), the rhizoplane (the root tissue surface colonized by microorganisms), and the endosphere.
Soil is the origin of the plant-associated microbiome and, while soil properties are determinants of root microbiome, the host plant significantly influences formation of rhizosphere and endophytic microbial communities. As the understanding of soil and plant microbiome progresses, there is a need to move the focus of the research from a simple description of community structure toward identification of the underlying mechanisms that define complexity of microbiota and link all members of soil community into single, stable, and functional entity (Fierer, 2017; Shade, 2017). As a result, the microbe–microbe and microbe–host interactions in plant microbiomes and their role in shaping root-associated microbial communities, as well as the potential of these interactions to affect host health have been the subject of several recent studies (Agler et al., 2016; Lareen et al., 2016; van Overbeek and Saikkonen, 2016; Busby et al., 2017; Yang et al., 2017; Zhang et al., 2017). The role of some microbial taxa (“hub” taxa) in shaping plant microbiomes in response to abiotic and host-derived factors has been recently proposed and verified (Agler et al., 2016). The hub taxa were defined as microbial groups, which are significantly more connected within the network than other groups based on centrality measurements, such as degree, betweenness centrality and closeness centrality. The strong plant–microbe interactions allow hub taxa to exert indirect effects on microbial communities by affecting the host and triggering plant species sorting preferences. In addition, hub taxa also directly inhibit or facilitate the growth of other microbes affecting overall interconnected communities (Agler et al., 2016).
Bacterial and fungal communities play an important role in soil and plant microbiomes (van Overbeek and Saikkonen, 2016) and in plant nutrient acquisition and stress adaptation (Vandenkoornhuyse et al., 2015). In addition to archaea, bacteria, and fungi, protists are highly abundant in soils and are represented by phylogenetically diverse group. Soil protists carry out a broad range of functions that affect soil fertility and plant health. These functions include modulating bacterial, fungal, algal, and nematode populations (Geisen, 2016; Geisen et al., 2015a), influencing soil nutrient cycling (Seppey et al., 2017), and exerting animal and plant-pathogenic effects (Geisen et al., 2015b). Protists play a central role in linking bacterial and fungal soil populations into a single and complex ecological network (Xiong et al., 2017) with prevalence of antagonistic interactions detected between the kingdoms and mutualistic interactions detected within the kingdoms (Agler et al., 2016). Protistan community structures are consistent within habitat types and geographic regions (Grossmann et al., 2016) and influenced by biotic and abiotic factors (Xiong et al., 2017; Yurgel et al., 2017). Despite their importance in soil ecosystems, protists remain the least characterized microorganisms in soil. In particular, plant-associated protistan communities and their roles in plant–microbiome interaction are not well understood.
Vaccinium angustifolium (wild blueberry) management is designed to bring agricultural field standards to natural wild blueberry habitats but retain these conditions close to natural (Hall et al., 1979; Eaton, 1988; Bell et al., 2009; Drummond et al., 2009). We recently used this system to study bacterial, fungal, and non-fungal eukaryotic communities and their responses to biotic and abiotic factors in a separate article. We found that soil bacteria and eukaryotes responded differently to biotic and abiotic factors: soil eukaryotes were more influenced by soil chemical characteristics, while bacteria more strongly responded to the presence of the plant (Yurgel et al., 2017). In this study, we employed wild blueberry managed and natural ecosystems to study interactions between plant and its microbiome focusing on root-associated bacterial and eukaryotic communities, which was mostly comprised by endophytic microorganisms. We evaluated how aggregate differences between forest and managed systems affect root microbiome and identified several eukaryotic taxa linked to field fruit production yield. We also analyzed the inter-kingdom correlations in soil and root-associated microbiota to identify the most connected (hub) microbial taxa in soil and root-associated communities. As a result, this study provides an integrative view on inter-kingdom soil and plant associated communities and identifies microbial taxa with potential importance in plant health and production.
Materials and Methods
The wild blueberry root samples, rhizosphere and bulk soil used in this study were collected in August 2015 (Yurgel et al., 2017). The sample collection, preparation, sequencing and initial bioinformatics analysis of the microbial communities from the rhizosphere and bulk soil was published previously (Yurgel et al., 2017). We included this sequencing data obtained from rhizosphere and bulk soil samples in this study as well for further analysis and comparison with the sequencing data obtained from root samples. Samples used in this study were collected across six managed blueberry fields and two forest sites adjacent to Nova Scotia Blueberry Institute (NSBI) fields at Debert and a commercial field situated near Collingwood Corner, Canada (Yurgel et al., 2017) (Supplementary Table S1). Three managed fields had a history of low yield fruit production and the other three had a history of high fruit yield production. After collecting rhizosphere soils from wild blueberry roots, MngRhizo and FrstRhizo samples (Yurgel et al., 2017), MngRoot and FrstRoot samples were stored in 50 ml sterile Falcon tubes at -86°C. A total of 15 roots from natural (FrstRoot) and 34 roots for manages (MngRoot) plants were collected (Supplementary Table S1).
Root Tissue Sample Preparation
For DNA isolation around 1 g of each root was placed into a 15 ml tube with 10 ml sterile water and sonicated for 60 s at 20°C in ultrasonic water-bath with 35 kHz frequency. Each root sample was then removed from the tube and placed into a new tube with 10 ml sterile water and sonicated for 60 s again. This step was repeated twice. The cleaned roots were cut into 5 mm pieces using sterile scissors and then placed into sterilized mortals. The samples were frozen in liquid nitrogen and ground into a fine powder using a sterile pestle. A total of 0.250 g ground root tissue was used for DNA isolation.
DNA Extraction and Sequencing
DNA extraction was carried out using the PowerSoil DNA Isolation Kit (MO BIO Laboratories, Carlsbad, CA, United States) according to the manufacturer’s protocol. The same DNA isolation kit was previously used for DNA extraction from rhizosphere and bulk soil (Yurgel et al., 2017). DNA quality and concentration were measured using a NanoDrop 1000 spectrophotometer (Thermo Scientific, Waltham, MA, United States). At least 50 ng (10 μL) of DNA sample were sent to the Dalhousie University CGEB-IMR1 for V6–V8 16S rRNA gene (16S; forward: ACGCGHNRAACCTTACC; reverse: ACGGGCRGTGWGTRCAA) and V4 18S rRNA gene (18S; forward: CYGCGGTAATTCCAGCTC; reverse: AYGGTATCTRATCRTCTTYG) library preparation and sequencing. Samples were multiplexed using a dual-indexing approach and sequenced using an Illumina MiSeq with paired-end 300 + 300 bp reads. All PCR procedures and Illumina sequencing details were as previously described (Comeau et al., 2016; Yurgel et al., 2017). All sequences generated in this study are available in the NCBI sequence read archive under the accession numbers PRJNA434066 (16S) and PRJNA434067 (18S).
Sequencing Data Processing
Sequence data processing and OTU picking were described in our earlier work (Yurgel et al., 2017). In short, the Microbiome Helper standard operating procedure was used to process and analyze the sequencing data (Comeau et al., 2017). Overlapping paired-end reads were stitched together using PEAR (v0.9.6) (Zhang et al., 2014). FASTX-Toolkit (v0.0.14) (Gordon and Hannon, 2010) was to filter out reads that had a quality score less than 30 at >10% of positions. In addition, we filtered out reads shorter than 400 bp that did not contain matching 59 and 39 sequences to the appropriate forward and reverse primers with BBMap (v35.85) (Bushnell, 2014). Chimeric reads were to screen out by running USEARCH (v6.1) (Edgar et al., 2011; Bushnell, 2014) with the options mindiv = 1.5 and minh = 0.2.
OTU (Operational Taxonomic Unit) Picking and Statistical Analyses
Following these filtering steps, we ran open-reference OTU picking using QIIME wrapper scripts (Caporaso et al., 2010). Specifically, SortMeRNA [v2.0-dev; (Kopylova et al., 2012)] was used for the reference OTU picking steps (with sortmerna_coverage = 0.8) and sumaclust (v1.0.00) (Mercier et al., 2013) for the de novo OTU picking steps (with 10% of the failures sub-sampled). We filtered out OTUs that contained fewer than 0.1% of the total sequences in order to compensate for MiSeq run-to-run bleed-through (see Comeau et al., 2016). Alpha-diversity (richness and Chao1) and beta-diversity (weighted UniFrac distance) (Lozupone et al., 2011) metrics were generated using QIIME. Variations in sample groupings explained by weighted UniFrac beta-diversity distances (Adonis tests, 999 permutations) were run in QIIME to calculate how sample groupings are related to microbial community structure. Analysis of taxonomic profiles and Principal Coordinate Analysis (PCoA) were performed using the STAMP software package (Parks et al., 2014). Corrected P-values (q-values) were calculated based on Benjamini–Hochberg FDR multiple test correction.
Co-occurrence Network Construction and Analysis
The co-occurrence analysis was performed using the CCREPE (Compositionality Corrected by REnormalization and PErmutation) R package (Schwager, in press), which has previously been used to construct co-occurrence networks from microbial sequencing data (Gevers et al., 2014; Vazquez-Baeza et al., 2016). This network uses a novel similarity measure, the N-dimensional checkerboard score (NC-score) (Stone and Roberts, 1990), which is particularly appropriate to compositions derived from microbial community sequencing data. Microbes found in less than 5% of samples were removed from the analysis. The taxa represented by less than 1% of the reads in all samples were also removed. First, the co-occurrence and co-exclusion patterns in the samples were scored. The resulted were filtered to remove non-statistically significant relationships. We generated 12 networks based on strong correlations with p-values < 0.01, 0.001, 0.0001 and Bonferroni cut-offs at the genus, family and order levels. The data were loaded into Cytoscape 3.4.0 (Shannon et al., 2003) and used to calculated node statistics, such as degree, betweenness centrality, and closeness centrality. We used the Excel functions NORM.DIST to fit a normal distribution to degree, betweenness centrality or closeness centrality parameters to identify the values above which nodes can be considered outliers, corresponding to p < 0.1. Nodes with degree, betweenness centrality and closeness centrality above p-value = 0.1 for all three parameters in at least two out of four correlation networks based on p-values < 0.01, 0.001, 0.0001 and Bonferroni cut-offs were considered to be hub taxa. The networks were visualized with Cytoscape and were represented as graphs with microbial groups as vertices/nodes and the edges as interaction types.
Composition of Wild Blueberry Root Microbial Communities
A total of 5,569,830 high-quality 18S sequences and 595,992 high-quality 16S sequences were obtained from 49 root samples from plants from managed (MngRoot) and natural habitats (FrstRoot). The plant-derived OTUs Archaeplastida and Chloroplast were represented by 5,332,133 18S and 29,411 16S reads, respectively. For direct comparison of diversity and structure of microbial communities across environmental niches, the raw sequencing data from root samples from plans from managed (MngRoot) and natural habitats (FrstRoot) were combined with the raw sequencing data obtained from corresponding rhizosphere samples from plans from managed (MngRhizo) and natural habitats (FrstRhizo), and bulk soil samples from managed (MngBulk) and natural habitats (FrstBulk) (Yurgel et al., 2017) for processing, OTU picking and statistical analyses.
A total of 7,036,418 high-quality 18S sequences were obtained from root, rhizosphere (MngRhizo, FrstRhizo) and bulk (MngBulk, FrstBulk) samples. To remove plant-derived OTUs, 18S sequences annotated as Archaeplastida/Plantae and unassigned OTUs were filtered out. A total of 1,328,201 high-quality 18S sequences remained in the dataset. After normalization to a depth of 1,922 reads (the depth of the smallest dataset after the 8 lowest samples were removed), 253,704 reads were retained, including 80,724 high-quality 18S sequences representing root community from 42 samples. These reads were distributed among 1,731 OTUs across all environmental niches and among 996 OTUs across root samples at 97% identity (Figure 1A). Around 52% (896) of OTUs were shared among bulk soil, rhizosphere and root habitats, while only 1% of OTUs were specific to either bulk soil, rhizosphere or root niches. A significant proportion of OTUs (688 OTUs, ∼40%) was shared among only bulk and rhizosphere.
FIGURE 1. Venn diagram showing specific and shared OTUs across bulk, rhizosphere, and root niches. (A) 18S rRNA; (B) Bacteria16S rRNA.
Across all environmental niches 1,201 non-fungal OTUs including Alveolata (343 OTUs), Metazoa (286 OTUs), Cercozoa (283 OTUs), Hacrobia (120 OTUs), Stramenopiles (68 OTUs), and Nematoda (64 OTUs) were identified. The top 15 most relatively abundant root-associated eukaryotic classes (Figure 2A) represented ∼93% of all reads identified in the root samples and only 67 and 57% of all 18S reads identified in the bulk and rhizosphere samples, respectively. Around 92% of the total read identified in root samples were classified as Opisthokonts division. Of this, fungi were represented by 76% of the reads, including 72% of Ascomycota and 2% of Basidiomycota and Mucoromycota each (Figure 2A). Other fungal taxa identified in the study included Glomeromycota, Mucoromycotina, and Chytridiomycota. Most relatively abundant non-fungal root-associated eukaryotes included Metazoa, ringed worms Annelida (4%, 7 OTUs), Nematoda (2%, 12 OTUs), Arthropoda (1.4%, 6 OTUs), and Cercozoa (4%, 30 OTUs).
A total of 3,232,834 high-quality 16S sequences were obtained from root, rhizosphere and bulk samples. The reads annotated as Chloroplast were filtered, which resulting in a total of 3,186,706 high-quality 16S sequences remaining. The datasets were normalized to the depth of the smallest dataset, 7,136 reads, and 349,664 and 335,392 reads were retained in rhizosphere and bulk samples, respectively. The root community was represented by 349,664 high-quality 16S sequences across 49 samples. These reads were distributed among 8,058 OTUs across all environmental niches of which 6,802 OTUs were also found in root samples at 99% identity (Figure 1B). More than 80% (6,466 OTUs) were shared among three environmental habitats. Bulk, rhizosphere, and root-specific OTUs accounted for 1.5, 0.2, and 0.1% of total OTUs, respectively, and 14% of OTUs (1,120) were shared among bulk and rhizosphere. The top 15 most relatively abundant root associated bacterial classes represented ∼94% of all 16S rRNA reads identified in the root samples and ∼83 and 89% of all reads identified in the bulk and rhizosphere samples, respectively. The most abundant bacterial classes found in root samples were Proteobacteria (37%), including Alphaproteobacteria (23%) and Gammaproteobacteria (8%), Acidobacteria (26%), Actinobacteria (16%), Bacteroidetes Saprospirae (5%), Chloroflexi Ktedonobacteria (4%), and Verrucomicrobia Spartobacteria (2%) (Figure 2B).
Transition of Microbial Communities From Rhizosphere to Root
Visualization of dissimilarity between eukaryotic communities across all environmental niches using Principal Coordinate Analysis (PCA) showed clear separation between soil bulk/rhizosphere (MngBulk, FrstBulk, MngRhizo, and FrstRhizo) and root (MngRoot and FrstRoot) communities (Supplementary Figure S1A). An analysis of the strength and statistical significance of sample groupings (Adonis test) indicated that niche (bulk, rhizosphere, and root) is associated with the structure of the eukaryotic community (R2 = 0.18, p < 0.001). Even stronger strength of sample groupings was detected when only rhizosphere and root niches were considered (R2 = 0.23, p < 0.001). Pairwise comparisons of Chao1 richness, Simpson evenness and Shannon diversity revealed a significant decrease in alpha-diversity of root eukaryotic communities compared to rhizosphere and bulk communities (Supplementary Figure S2A). Considering taxonomic groups, the relative abundance of a number of other eukaryotic taxa, such as Arthropoda, Dinophyceae, Prymnesiophyceae, Spirotrichea, and Urochordata (Figure 2A and Supplementary Figure S3A) was significantly lower in the root compared to rhizosphere. Only taxa represented by >50 and >250 18S and 16S reads, respectively, were considered. The relative abundance of fungi was decreased in rhizosphere compared to bulk soil, but increased in roots. In particular, the relative abundance of Pezizomycotina, which comprises most of the ascomycetous pathogens and mutualists, was significantly higher in root compared to rhizosphere. This included the classes Sordariomycetes, Leotiomycetes, containing many plant pathogens and mycorrhizal fungi, putative ericoid mycorrhizal fungi Lachnum (Glawe, 2008; Walker et al., 2011; Bizabani and Dames, 2015), and potential plant growth promoting dark septate endophyte Phialocephala (Rodriguez et al., 2009; Lukesova et al., 2015; Schlegel et al., 2016).
Similarly, to the analysis of eukaryotic comminutes, the PCoA showed clear separation between bulk, rhizosphere and root bacterial communities (Supplementary Figure S1B). The analysis of strength and statistical significance of sample groupings indicated that, niche (bulk, rhizosphere, and root) influenced the structure of the bacterial community (R2 = 0.26, p < 0.001). However, less strength of sample groupings was detected when only rhizosphere and root niches were considered (R2 = 0.17, p < 0.001). Similarly, to eukaryotic comminutes, Chao1 richness, Simpson evenness and Shannon diversity was significantly decrease in root associated bacterial communities compared to rhizosphere and bulk communities (Supplementary Figure S2B). Considering taxonomic groups, the relative abundances of several bacterial taxa, including Chthoniobacteriales, Acidobacteriales, Ellin6513, Solibacterales, and Syntrophobacteriales were significantly decreased in root compared to rhizosphere (Supplementary Figure S3B). The relative abundance of Ellin6513 was also decreased in rhizosphere compared to bulk soil. Conversely, the relative abundances of Saprospirales, Actinomycetales, Rhizobiales, and Xanthomonadales had increased relative abundances with proximity to plant, with the lower relative abundances in bulk soil and the highest in root (Supplementary Figure S3B).
Effect of Management and Field Production
Management had minor effect on root eukaryotes (Adonis test, R2 = 0.10, p < 0.05) and there were no differences in the relative abundances of eukaryotes detected between MngRoot and FrstRoot samples. However, when bulk, rhizosphere and root samples were analyzed together, arbuscular mycorrhizal fungi Glomeromycota (Davison et al., 2015) and grazers Nematoda were relatively more abundant and animal and fungal pathogen, Kickxellomycota (Spatafora et al., 2016), was relatively less abundant in forest compared to fields (Supplementary Figure S4A). Only taxa represented by >50 and >250 18S and 16S reads, respectively, were considered. Compared to eukaryotes, management has stronger effect on root bacterial communities (Adonis test, R2 = 0.14, p < 0.01). Bacterial orders Chthoniobacterales, Ellin6513, Solirubrobacterales, and Thermogemmatisporales had lower relative abundances, while orders Rhodospirillales and Solibacterales had higher relative abundances in FrstRoot compared to MngRoot samples (Supplementary Figure S4B). Additionally, differences in relative abundances of Chthoniobacterales, Ellin6513, Thermogemmatisporales, and Rhodospirillales were also detected between MngRhizo and FrstRhizo samples (Supplementary Figure S4B). When all niches from managed habitats were analyzed together, minor but statistically significant correlation between field fruit production and the structure of eukaryotic (Adonis test, R2 = 0.04, p < 0.05) but not bacterial communities (Adonis test, R2 = 0.02, p > 0.05) was detected. The fields with lower fruit yield had higher relative abundance of parasitic fungi Cryptomycotina (Letcher et al., 2017), gliding bacterivores/algaevores Glissomonadida (Cercozoa) (Howe et al., 2009) and Vampyrellida (Rhizaria) (Hess, 2017) (Supplementary Figure S5). Only taxa represented by >50 18S were considered.
Inter-Kingdom Correlation in Wild Blueberry Microbiomes
We generated a co-occurrence network by correlating relative abundances between microbial taxa found in ≥5% of samples from root, rhizosphere and bulks soil, with taxa grouped at the genus (Figure 3), family (Supplementary Figure S6A) and order levels (Supplementary Figure S6B). We used a Bonferroni cut-off to remove correlations with low p-values. These remaining correlations were used to construct a combined “edge-weighted spring embedded” co-occurrence network views in which positive correlations (blue) are pulling samples together forming clusters, while negative correlations (red) are pushing the samples apart.
FIGURE 3. Co-occurrence network generated by measuring abundance co-correlation between microbial taxa from root and rhizosphere and bulk soil. Correlation base network analysis showing potential interactions between bacterial, fungal, and protists genera. The size of the node is proportional to a taxon’s average relative abundance across all the samples. The lines connecting nodes (edges) represent positive (blue) or negative (red) co-occurrence relationship. The intensity of the color and the length of the edges represent the strength of correlation. The taxa shown in the figure are hub taxa, which were identified as those that were significantly more central based on the measurements of degree, betweenness centrality and closeness centrality (p > 0.1 based on normal distribution fit). The taxa in bold were found as hub taxa at least in two co-occurrence networks base on the abundances of microorganisms grouped at the genus, family or order levels.
For all three networks, three main microbial clusters were visually detected. Cluster A1 was mostly occupied by eukaryotes Metazoa, Hacrobia, Alveolata, and Radiolaria (Figure 3 and Supplementary Figures S6A,B), many of which have previously been associated with aquatic environments. These eukaryotes negatively correlated with a taxon in Glissomonadida from Clusters A3 and Pezizomycotina, which was scattered across network based on grouping at the genus level (Figure 3) or stood alone in the networks based on grouping at the family and order level (Supplementary Figures S6B). Bacterial taxa found in this cluster include Verrucomicrobia, Planctomycetes, and Candidatus Solibacter. The eukaryotes had the higher combined relative abundance in rhizosphere compared to bulk soil and root (Supplementary Figure S7A).
Clusters A2 was mostly represented by bacterial taxa from Alpha-, Beta-, and Gammaproteobacteria, Bacteroidetes, and Actinobacteria. This cluster had a strong negative correlation with Ascomycota and bacterial taxa from Clusters 3 (Figure 3 and Supplementary Figures S6A,B). Clusters A2 exhibited an increase in combined relative abundance with the shift from bulk to rhizosphere and from rhizosphere to root (Supplementary Figure S7A). Fungi, including potential pathogens, predators Cercozoa, Arthropoda, Nematoda, and Rotifers, and bacterial, Acidobacteria, Chloroflexi, and Verrucomicrobia were most abundant taxa belonging to Clusters 3 (Figure 3 and Supplementary Figures S6A,B). The combined relative abundances of both kingdoms in this cluster were negatively affected by proximity of the plant (Supplementary Figure S7A).
When Bonferroni cut-off p-values were used to select strong correlations, inter-kingdom correlations were represented by ∼21% of all correlations, with a higher proportion of positive correlations (∼68%) compared to negative ones (32%) (Figure 4A). Within each kingdoms, eukaryotic and bacteria correlations were represented by 42 and 37%, respectively. Within kingdoms, the positive and negative correlations were relatively evenly distributed (Figures 4B,C), with 48 and 43% of negative correlations within eukaryotes and within bacteria, respectively. The positive correlations between eukaryotic organisms exhibited a clear separation into two groups with low correlation strength (NC score < 0.58) and high correlation strength score (NC score < 0.65). All correlations with fungi were located in the group with low correlation strength (red colored bars in Figure 4B) with average NC score significantly lower than that of non-fugal correlations (p < 10-28).
FIGURE 4. Strength of correlation (NS-score) obtained by analysis of correlations between microbial genera using the CCREPE (Compositionality Corrected by REnormalization and PErmutation) R package. p-value Bonferroni cut-off was used to select strong correlations. Negative NS scores represent negative correlations. (A) Inter-kingdom (211) correlations; (B) Eukaryotic (375) correlations, red bars represent positive fungal/fungal and fungal/protists correlations; (C) Bacterial (422) correlations.
Co-occurrence Network in Bulk and Rhizosphere Soil Communities
Similarly, we generated co-occurrence sub-networks by considering bacterial and eukaryotic communities in (i) bulk and rhizosphere soil (soil-associated) (Figure 5) and (ii) rhizosphere and root (root-associated) microbiomes (Figure 6). Two microbial clusters were detected in the network considering the soil-associated microbiota (Figure 3). Cluster B1 was occupied by eukaryotes Metazoa, Hacrobia, Alveolata, and Radiolaria and bacteria Acidobacteria, Actinobacteria, Bacteroidetes, and Proteobacteria. These taxa were more abundant in rhizosphere compared to bulk soil (Supplementary Figure S7B). Eighty percent of eukaryotic and 86% of bacterial taxa, found in this cluster, were also found in the Clusters A1 and A2 in the network based on microbial communities across all environment niches (Figure 3). On average, the taxa found in Cluster B2 in the network considering the soil-associated microbiome were more abundant in bulk soil compared to rhizosphere and many of the taxa, found in this cluster (Figure 5) were also found in Cluster A3, considering microbial communities across all environment niches (Figure 3). Fungi were also a part of Cluster B2 in the network considering bulk and rhizosphere soil.
FIGURE 5. Co-occurrence network generated by measuring abundance co-correlation between microbial taxa from root and rhizosphere and bulk soil. Correlation base network analysis showing potential interactions between bacterial, fungal, and protists genera. The size of the node is proportional to a taxon’s average relative abundance across all the samples. The lines connecting nodes (edges) represent positive (blue) or negative (red) co-occurrence relationship. The intensity of the color and the length of the edges represent the strength of correlation. The taxa shown in the figure are hub taxa, which were identified as those that were significantly more central based on the measurements of degree, betweenness centrality and closeness centrality (p > 0.1 based on normal distribution fit). The taxa in bold were found as hub taxa at least in two co-occurrence networks base on the abundances of microorganisms grouped at the genus, family or order levels.
FIGURE 6. Co-occurrence network generated by measuring abundance co-correlation between microbial taxa from root and rhizosphere. Correlation base network analysis showing potential interactions between bacterial, fungal, and protists genera. The size of the node is proportional to a taxon’s average relative abundance across all the samples. The lines connecting nodes (edges) represent positive (blue) or negative (red) co-occurrence relationship. The intensity of the color and the length of the edges represent the strength of correlation. The taxa shown in the figure are hub taxa, which were identified as those that were significantly more central based on the measurements of degree, betweenness centrality and closeness centrality (p > 0.1 based on normal distribution fit). The taxa in bold were found as hub taxa at least in two co-occurrence networks base on the abundances of microorganisms grouped at the genus, family or order levels.
Co-occurrence Network in Rhizosphere and Root Communities
The network considering abundance co-correlation in the root-associated microbiome exhibited striking complexity (Figure 6). One strongly interconnected cluster (Cluster C1) and C4 loosely interconnected clusters were detected in the network. The Cluster C1 was mostly occupied by eukaryotes, some of which had been primarily associated with aquatic environments. Aquatic bacteria Planctomycetes and Acidobacteria were also found in the cluster. The Cluster C1 had negative correlation with Bradyrhizobiaceae and Pezizomycotina - the major taxa comprising Cluster C2. Both kingdoms from Cluster C1 were more abundant in rhizosphere compared to root (Supplementary Figure S7C) and reverse tendency was detected in Cluster C2. Cluster C3 included predators Filosa Sarcomonadea, Metazoa (Arthropoda, Nematoda, and Rotifera) and Alveolata and several potential parasitic fungi. Clusters C4 and C5 were mostly represented by bacteria.
Identification of Hub Taxa in Microbial Networks
For identification of hub microbes, we generated co-occurrence networks based on strong correlations with p-values < 0.01, 0.001, 0.0001 and Bonferroni cut-offs for microbial taxa grouped at genus, family or order levels. 12 networks were generated for each of 3 types of communities: (i) across all environmental niches, (ii) associated with bulk and rhizosphere soil, and (iii) associated with rhizosphere and plant root. The multiple p-values were used since it has been previously shown that the strength of cut-offs affects network structure (Kurtz et al., 2015). Similarly, in our analysis we found differences in the parameters of the nodes from the networks based on different p-value cut-offs. For each network, we identified nodes with significantly higher degree, betweenness centrality or closeness centrality based on normal distribution fit with p < 0.1 for all three parameters using at least two out of four correlation cut-offs. These nodes were considered as potential outliers.
Several potential outliers were identified in the networks considering microbial communities across all environmental niches and based on different grouping of the taxa (Supplementary Table S2). The bacterial genera Bradyrhizobiaceae and Pedosphaerales and the fungi Pezizomycotina, Geoglossomycetes, and Leotiomycetes were highly connected (Figure 3). Combined together, these four microbial taxa were directly connected to 30 eukaryotic and 34 bacterial taxa, which represented 67% of all nodes in network based on correlations with p-values with Bonferroni cut-offs. Bradyrhizobium and Pedosphaerales were supported at all taxonomic levels (Figure 3 and Supplementary Figures S6A,B) and were directly connected to 21 (43%) eukaryotic and 29 (62%) bacterial taxa grouped at genera level, based on correlations with p-values with Bonferroni cut-offs. In the co-occurrence network considering the soil-associated microbiome and based on the microbial taxa grouped at genera level, eukaryotic taxa Dinophyceae, Telonemia, Maxillopoda, and Appendicularia and bacterial taxa Acidobacteriaceae, Caulobacteraceae, and Pedosphaerales were highly connected. Acidobacteriaceae, Caulobacteraceae were also found as hub taxa at least in one other co-occurrence networks based on different grouping (Supplementary Table S3 and Figure 5). Considering the root-associated microbiome, Bradyrhizobiaceae, Actinomycetales, Solibacterales, Pedosphaerales, and the fungi Pezizomycotina Leotiomycetes were identified as hub taxa in at least two co-occurrence networks (Supplementary Table S4 and Figure 6).
The concept of holobiont encompasses a complex network of functions and symbiotic interactions between host–plant and its microbiome. Over the past several years an understanding the bacterial and fungal communities as components of the holobiont and their role in plant nutrient acquisition and resistance to biotic and abiotic stresses has progressed significantly (Vandenkoornhuyse et al., 2015). However, a full comprehension of plant holobiont concept is missing an explanation of how the non-fungal eukaryotic microorganisms fit in this complex network of plant–microbiome interactions. To elucidate the role of soil eukaryotes and prokaryotes in plant-associated microbiome we investigated wild blueberry root microbiomes containing 996 eukaryotic and 6,802 bacterial OTUs, respectively. This community was mostly comprised by endophytes with possible minor proportion of root-epiphytic microorganisms. The microbiome was combined with previously identified bulk soil and rhizosphere microbiomes (Yurgel et al., 2017) resulting in a total of 530 fungal, 1201 non-fungal eukaryotic, and 8058 bacterial OTUs across all environmental niches. This comprehensive dataset enabled us to evaluate the role of non-fungal eukaryotes in shaping the interactions between blueberry plants and soil microbes.
Similar to previous reports (Leach et al., 2017), fungi were the most abundant eukaryotic taxa in the wild blueberry root microbiome. These fungi included a number of potential mycorrhizal fungal taxa, such as Pezizomycotina, Glomeromycota, Mucoromycotina, and Chytridiomycota (Kohout et al., 2012; Davison et al., 2015; van der Heijden et al., 2015; Orchard et al., 2017), putative ericoid mycorrhizal fungi Lachnum (Walker et al., 2011; Bizabani and Dames, 2015; Zhang et al., 2016), and potential plant growth promoting endophyte Phialocephala (Rodriguez et al., 2009; Lukesova et al., 2015; Schlegel et al., 2016). We were able to identify 30, 12, 7, and 6 individual OTUs belonging to Cercozoa, Nematoda, Annelida, and Arthropoda, respectively. In total these microorganisms were represented by ∼12% of the high quality 18S reads and were the most abundant non-fungal eukaryotes in the root microbiome.
It has been previously shown that bacteria belonging to the three main phyla, Proteobacteria, Actinobacteria, and Bacteroidetes, are the most abundant taxa in plant rhizosphere and endosphere, while the phylum Acidobacteria is often excluded from these compartments (Hacquard et al., 2015; Leach et al., 2017). Similarly, Alphaproteobacteria and Gammaproteobacteria, Actinobacteria, and Bacteroidetes were among the five most abundant bacterial taxa in wild blueberry roots and were enriched along the soil-endosphere continuum. Although Acidobacteria was the second most abundant phylum in root microbiome, its abundance was significantly decreased in roots compared to rhizosphere. The exclusion of Acidobacteria from endophytic compartment has been reported in other plant microbiomes (Bulgarelli et al., 2013).
Transition of Microbiome Along the Soil-Endosphere Continuum
Bulk soil microbiome serves as a foundation for plant-associated microbiome (Shakya et al., 2013; Schreiter et al., 2014). In agreement with this notion, more than 52% of eukaryotic and 80% of bacterial OTUs identified in this study are found in all three environmental niches while only 1% of OTUs were unique to root associated microbiome. Rhizosphere is the first habitat with a strong plant influence on microbial communities. However, the transition from root surface to interior provides the strongest species sorting effect, demanding microbial specialization necessary for invasion and survival inside plant tissue and, as a result, a significant decrease in community diversity (Hacquard et al., 2015; Vandenkoornhuyse et al., 2015). Our data also indicated a significant decrease in bacterial and eukaryotic diversity in root microbiome compared to rhizosphere and bulk soil, probably as a result of this specialization process.
As previously reported in the wild blueberry rhizosphere samples, plant-influenced species sorting has a stronger effect on bacteria than on eukaryotes (Yurgel et al., 2017). Here, we detected the opposite species sorting effect in the root microbiome. A lower proportion of eukaryotic OTUs than bacterial OTUs were shared between all three environments. Moreover, the 15 most abundant eukaryotes in the root were at significantly lower relative abundance in the other two environments, which was not the case for the most abundant bacteria in the roots. In agreement with this finding, niche (rhizosphere vs. root) correlated with 23% of eukaryotic and 17% of bacterial community variation. The specific effect of species sorting in root microbiome due to host resulted in an increase in relative abundance of fungi adapted to plant-associated life-style, such as Lachnum, Phialocephala, and Sordariomycetes, as well as lichen-forming fungi Lecanorales, Cetradonia linearis and Cladonia. In contrast, the relative abundances of microscopic animals, protists and algae were decreased along the soil-endosphere continuum in the root, probably because of strong impact of host defense system on community establishment and low adaptation of non-fungal eukaryotes to host-plant defense responses.
The Link Between Field Fruit Production and Community Structure
Since we did not have detailed information about fruit yield in the managed fields used as sampling sites, we assigned each field with high or low fruit yield parameter, based on the assessment of field production by blueberry growers. Our data showed minor but statistically significant correlation between field fruit production and the structure of eukaryotic community. More specifically, we found that parasitic fungi Cryptomycotina (Letcher et al., 2017), gliding bacterivores/algaevores Glissomonadida (Cercozoa) (Howe et al., 2009) and Vampyrellida (Rhizaria) (Hess, 2017) were more abundant in the fields with low fruit yield across all three environmental niches. The presence of these microorganisms might directly or indirectly affect plant health through the disease development or/and depletion of microbial taxa with beneficial effect on plant development and production. However, more detailed studies are required to verify this hypothesis, which include disease survey of the fields and increase of the number of sampling sites for better resolution of differences in the structure of microbiomes.
Previously we showed that the aggregate difference in forest vs. managed systems influenced bacterial communities in blueberry rhizospheres, but had less effect on eukaryotic communities (Yurgel et al., 2017). A similar tendency of stronger effect of management on bacterial communities compared to eukaryotic communities was detected in blueberry roots. The main factors involved in the differentiation of microbial community between managed and natural habitats might include previous pruning of the plants, use of soil-applied fertilizers and pest management practices, which resulted in higher growth rates and fruit production of managed stands compared to forest stands (Yurgel et al., 2017).
Community Correlation Networks
To further evaluate the rules guiding the assembly of plant-associated microbiota, we generated bacterial and eukaryotic community correlation networks, which incorporated different levels of host–plant influence. In this model the combined bulk and rhizosphere communities (soil-associated microbiome) were considered to be under lower plant influence compared to combined rhizosphere and root communities (root-associated microbiome). The combination of microbial communities across all environmental niches in a single correlation networks provided a complementary view of microbe–microbe and plant–microbe interaction in a broader ecological setting. Previous studies showed that the bacterial network is more complex in root-associated microbiome than in bulk soil (Cordero and Datta, 2016; Shi et al., 2016). We also found that microbial network, comprising both bacterial and eukaryotic microorganisms became more complex along the soil-endosphere continuum. Only two visually well-defined clusters emerged in the soil-associated co-occurrence network, while four loosely and one tightly associated cluster emerged in the root-associated co-occurrence network.
The existence of extensive mutualistic interactions among plant-associated microorganisms is a well-known concept (Hallam and McCutcheon, 2015). Previously within kingdoms of plant-associated microorganisms, more positive than negative correlations were detected, while more negative than positive correlation were detected between microbes from different kingdoms (Agler et al., 2016). Our data showed a more even distribution of positive and negative correlations within kingdoms suggesting that co-exclusion or competition also plays an important role in shaping plant associated microbiomes. A previous study of inter-kingdom correlations showed that soil protists formed distinct clusters that link a range of bacterial and fungal taxa (Xiong et al., 2017). In all networks constructed in this study, tightly associated clusters comprising both bacterial and eukaryotes organisms were identified. Moreover, a higher proportion of positive correlations compared to negative ones was detected between microbes from different kingdoms, which emphasizes the importance of mutualistic interactions in inter-kingdom networks.
Identification of Hub Taxa in the Microbial Networks
Across all environmental niches bacteria, Bradyrhizobium and Pedosphaerales, and fungi, Pezizomycotina Geoglossomycetes, and Leotiomycetes, were identified as hub taxa, suggesting an important role of these microorganisms in wild blueberry soil ecosystem.
Hub Taxa in Plant-Associated Microbiome
Bradyrhizobium, Pedosphaerales, and Leotiomycetes, were also hubs in the network considering root-associates microbiome. The ability of some highly interconnected microbial taxa to link host factors to plant microbiome variation has been recently tested (Agler et al., 2016). Bradyrhizobium genus is one of the most ubiquitous microorganisms in soils from across the world and plays a critical role in soil fertility. These bacteria have been used as a model organism to study the impact of environmental factors on soil microbiota (Shah and Subramaniam, 2017). The organisms from the Bradyrhizobium genus are able to promote plant growth by producing the plant growth promoting compounds indole-3-acetic acid and 1-amino-cyclopropane-1-carboxylic acid deaminase as well as fixating nitrogen inside plant tissues (Piromyou et al., 2017). The genus Leotiomycetes contains many plant pathogens and mycorrhizal fungi (Glawe, 2008; Walker et al., 2011; Bizabani and Dames, 2015) and therefore might have a profound effect on soil and plant health and, as a result also an effect on the microbiomes associated with these niches. Actinobacteria Actinomycetales, and Acidobacteria Solibacterales were also identified as hubs in root-associated microbiome. Actinobacteria is one of the most abundant taxa in plant rhizosphere and endosphere (Hacquard et al., 2015; Leach et al., 2017) and play a major role soil fertility and plant health. Actinomycetes are capable to improve the availability of nutrients and minerals in soils, suppress some pathogens and promote plant health (Bhatti et al., 2017).
Hub Taxa in Soil-Associated Microbiome
In the network considering abundance co-correlation in soil-associated microbiome, non-fungal eukaryotic taxa Dinophyceae, Telonemia, Maxillopoda, and Appendicularia and bacterial taxa Acidobacteriaceae, Caulobacteraceae, and Pedosphaerales were identified as hubs. Acidobacteria, is one of the most abundant bacterial taxa in soils, especially in acidic conditions predicted to be involved in soil nutrient cycling (Kielak et al., 2016). Ecological interactions Acidobacteria with Proteobacteria (Kielak et al., 2016) and with soils protists (Xiong et al., 2017) had been reported. While recently it was shown that Dinophyceae is an important member of soil protistan communities (Bates et al., 2013; Yurgel et al., 2017), little is known about the role of Telonemia, Maxillopoda, and Appendicularia in soil microbiome. Therefore, our findings emphasize the complexity of soil ecology and the need for more research aimed to understand the inter-kingdom interactions in soil and plant-associated communities.
Our analyses of eukaryotic and bacterial communities associated with wild blueberry ecosystems allowed us to better understand the plant-influenced species sorting effect on soil bacteria and fungi and gain insights into the effect of this process on non-fungal eukaryotes. This study also extends our knowledge about the effect of aggregate difference in forest vs. managed systems on microbial communities and identified several eukaryotic taxa that are potentially linked to the decrease in fruit production in wild blueberry agricultural ecosystems. Our data indicated that bacterial and eukaryotic interactions become more complex along the soil-endosphere continuum and included extensive mutualistic inter-kingdom. We also identified several potential hub taxa with important roles in soil fertility and/or plant–microbe interaction and indicated the potential role of these taxa in the interconnection between soils and plant health and overall microbial community structure.
SY and ML obtained funding. SY and DP designed the study and collected the samples. SY and AD processed the samples and performed the data pre-possessing. SY performed the bioinformatics analyses and wrote the manuscript. GD assisted with the bioinformatics analyses. SY, ML, and DP analyzed and discussed the results. SY, GD, ML, and DP participated in the production and the final version of the manuscript.
This work was supported by Nova Scotia Research Acceleration Grant RA2016-005, Discovery Grant from Natural Sciences and Engineering Research Council of Canada and Wild Blueberry Producers Association of Nova Scotia to SY. Additional support was provided to ML through the Strategic Research Initiatives Fund from Dalhousie University and a Discovery Grant from the Natural Sciences and Engineering Research Council of Canada.
Conflict of Interest Statement
The authors declare that the research was conducted in the absence of any commercial or financial relationships that could be construed as a potential conflict of interest.
The Supplementary Material for this article can be found online at: https://www.frontiersin.org/articles/10.3389/fmicb.2018.01187/full#supplementary-material
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Keywords: bacterial communities, eukaryotic communities, plant–microbe interaction, Vaccinium angustifolium, community networks
Citation: Yurgel SN, Douglas GM, Dusault A, Percival D and Langille MGI (2018) Dissecting Community Structure in Wild Blueberry Root and Soil Microbiome. Front. Microbiol. 9:1187. doi: 10.3389/fmicb.2018.01187
Received: 15 February 2018; Accepted: 16 May 2018;
Published: 06 June 2018.
Edited by:Davide Bulgarelli, University of Dundee, United Kingdom
Reviewed by:Richard Allen White III, RAW Molecular Systems (RMS) LLC, United States
Silvia Proietti, Università degli Studi della Tuscia, Italy
Copyright © 2018 Yurgel, Douglas, Dusault, Percival and Langille. This is an open-access article distributed under the terms of the Creative Commons Attribution License (CC BY). The use, distribution or reproduction in other forums is permitted, provided the original author(s) and the copyright owner are credited and that the original publication in this journal is cited, in accordance with accepted academic practice. No use, distribution or reproduction is permitted which does not comply with these terms.
*Correspondence: Svetlana N. Yurgel, email@example.com