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Community ecology across bacteria, archaea and microbial eukaryotes in the sediment and seawater of coastal Puerto Nuevo, Baja California

  • Sabah Ul-Hasan ,

    Roles Conceptualization, Data curation, Formal analysis, Funding acquisition, Investigation, Methodology, Project administration, Validation, Visualization, Writing – original draft, Writing – review & editing;

    Affiliations Department of Molecular and Cell Biology, School of Natural Sciences, University of California Merced, Merced, CA, United States of America, Quantitative and Systems Biology Graduate Program, University of California Merced, Merced, CA, United States of America

  • Robert M. Bowers,

    Roles Conceptualization, Formal analysis, Methodology, Resources, Visualization, Writing – original draft, Writing – review & editing

    Affiliation Department of Energy, Joint Genome Institute, Walnut Creek, CA, United States of America

  • Andrea Figueroa-Montiel,

    Roles Conceptualization, Funding acquisition, Investigation, Methodology, Project administration, Resources, Writing – review & editing

    Affiliation Department of Biomedical Innovation, Centro de Investigación Científica y de Educación Superior de Ensenada (CICESE), Ensenada, Baja California, México

  • Alexei F. Licea-Navarro,

    Roles Funding acquisition, Investigation, Methodology, Project administration, Resources, Writing – review & editing

    Affiliation Department of Biomedical Innovation, Centro de Investigación Científica y de Educación Superior de Ensenada (CICESE), Ensenada, Baja California, México

  • J. Michael Beman,

    Roles Conceptualization, Funding acquisition, Methodology, Resources, Writing – review & editing

    Affiliation Department of Life and Environmental Sciences, School of Natural Sciences, University of California Merced, Merced, CA, United States of America

  • Tanja Woyke,

    Roles Conceptualization, Data curation, Investigation, Methodology, Project administration, Resources, Supervision, Writing – original draft, Writing – review & editing

    Affiliations Department of Molecular and Cell Biology, School of Natural Sciences, University of California Merced, Merced, CA, United States of America, Department of Energy, Joint Genome Institute, Walnut Creek, CA, United States of America

  • Clarissa J. Nobile

    Roles Funding acquisition, Investigation, Supervision, Writing – original draft, Writing – review & editing;

    Affiliation Department of Molecular and Cell Biology, School of Natural Sciences, University of California Merced, Merced, CA, United States of America


Microbial communities control numerous biogeochemical processes critical for ecosystem function and health. Most analyses of coastal microbial communities focus on the characterization of bacteria present in either sediment or seawater, with fewer studies characterizing both sediment and seawater together at a given site, and even fewer studies including information about non-bacterial microbial communities. As a result, knowledge about the ecological patterns of microbial biodiversity across domains and habitats in coastal communities is limited–despite the fact that archaea, bacteria, and microbial eukaryotes are present and known to interact in coastal habitats. To better understand microbial biodiversity patterns in coastal ecosystems, we characterized sediment and seawater microbial communities for three sites along the coastline of Puerto Nuevo, Baja California, Mexico using both 16S and 18S rRNA gene amplicon sequencing. We found that sediment hosted approximately 500-fold more operational taxonomic units (OTUs) for bacteria, archaea, and microbial eukaryotes than seawater (p < 0.001). Distinct phyla were found in sediment versus seawater samples. Of the top ten most abundant classes, Cytophagia (bacterial) and Chromadorea (eukaryal) were specific to the sediment environment, whereas Cyanobacteria and Bacteroidia (bacterial) and Chlorophyceae (eukaryal) were specific to the seawater environment. A total of 47 unique genera were observed to comprise the core taxa community across environment types and sites. No archaeal taxa were observed as part of either the abundant or core taxa. No significant differences were observed for sediment community composition across domains or between sites. For seawater, the bacterial and archaeal community composition was statistically different for the Major Outlet site (p < 0.05), the site closest to a residential area, and the eukaryal community composition was statistically different between all sites (p < 0.05). Our findings highlight the distinct patterns and spatial heterogeneity in microbial communities of a coastal region in Baja California, Mexico.


The identification and description of microbial biodiversity patterns is important for understanding the biological underpinnings of ecosystem function. This is particularly true for coastal microbial communities, as they play important roles in the regulation of biogeochemical cycling at the land-sea interface [1,2], and in the ecological dynamics of larger organisms through symbiosis and disease [3,4]. Coastal microbial communities are complex and spatially variable [57], consisting of all domains of life interacting with each other in the water column and sediment [8]. The heterogeneity of coastal microbial communities thus demands intensive sampling to improve our understanding of microbial ecology and the structure and function of coastal ecosystems. Many studies of coastal microbial communities, however, take place along waters of Western world countries or at somewhat subjective “exotic” locales [9]. This leaves large swaths of un-sampled/under-sampled coastlines around the world where microbial diversity–and its associated geochemical and physical diversity–is poorly characterized.

A surge in marine microbial community ecology research over the past decade has led to a wealth of new information on the dynamics between microorganisms and their surrounding environments [6]. As a result, the identification of spatial and temporal patterns of microbial diversity, and how this information correlates to biogeochemical cycling, has been vastly expanded [1017]. A recent commentary by Brussaard and colleagues, for example, highlights the growing roles that “big data” from microbial ecology and biogeochemistry studies play in understanding how microbial communities shape the biogeochemical cycling patterns of coasts and oceans [18]. Such information gathered over time provides a starting point to determining the causes and effects of microbial community disturbances [19]. While these discoveries are innovative by providing new insight into marine microbial ecosystems, much coastal microbial diversity remains uncharacterized [2022].

The majority of microbial biodiversity “omics” studies are overwhelmingly focused on bacterial communities using 16S rRNA amplicon sequencing, and are often limited to a specific environment type rather than considering multiple aspects of microbial ecosystems [23,24]. Coastal microbial communities present a dynamic assemblage to test taxa richness and diversity between two environment types: sediment solids and seawater liquids. As a result of its texture, soil is well known to host high microbial richness across domains [25] and, by extrapolation, this is also likely to be the case for sediment [26] since sediment also possesses a large surface area for microorganisms to attach [27]. The added value of using next-generation technology with these types of sampling studies is that it provides detailed information on taxa within a larger ecosystem framework.

Investigating the sediment and seawater at one coastal point using biological replicates is advantageous because it allows for the comparisons of species richness estimates and abundance profiles across sample types [28]. Taking these measurements into account, an ecological study of microbial mats, for example, observed that bacterial and archaeal mat biodiversity in intertidal, hypersaline, and hot spring environments was influenced by mat chemistry and spatial location, more so than by temporal changes [29]. These variations between locations can correspond to variations in function and/or recovery after perturbation [30], and thus emphasize the importance of simultaneously characterizing both richness and abundance measurements in microbial ecology studies.

While the Baja California coastline shares the same marine ecoregion with the United States [31], its microbial biodiversity is surprisingly understudied relative to the Southern Californian coastline [32]. The Southern California Bight ecoregion of Baja California experiences intense upwelling events that are predicted to increase with climate change [33,34], and thus undergoes substantial nutrient flux that could affect microbial composition [35]. The handful of existing microbial biodiversity next-generation sequencing studies on the Baja California coast are largely centered on the hypersaline environments throughout Guerrero Negro, which differ considerably from coastal environments in terms of community composition [3644]. We selected the coastal site of Puerto Nuevo in Baja California, which is close to the United States-Mexico border, for the following reasons. First, this region experiences strong upwelling events that are associated with nutrient fluxes. Such upwelling events also lead to marine organism habitat loss, and are increasing with climate change [33,34]. Second, this region shares overlapping coastal physical features with Southern California and is thus likely to share similarities in microbial ecosystems. Third, this location is unrepresented in terms of coastal microbial community sampling, thus its study would expand our existing knowledge of microbial diversity. With these reasons in mind, the primary goal of our study is to obtain information on coastal microbial diversity across domains and environment types in Puerto Nuevo to set the precedent for additional microbial ecology studies along the Baja California coastline.

Using high-throughput sequencing, we characterized the bacterial, archaeal, and eukaryal microbial diversity in the sediment and seawater of three sites along a 0.45 km range in Puerto Nuevo in Playas de Rosarito, Baja California. Our goals were to determine (1) the differences in coastal microbial community richness and/or abundance between seawater and sediment environment types, (2) the alpha diversity within a sampling site versus the beta diversity among a 0.45 km range, and (3) the shared versus unique patterns between bacterial, archaeal and eukaryal microbial communities.

Materials and methods

Study area and sampling

The necessary field permit for this study (permit # PPF/DGOPA-009/17) was issued from the Secretaría de Agricultura, Ganadería, Desarrollo Rural, Pesca y Alimentación (SAGARPA), complying with all relevant regulations.

The coastal Puerto Nuevo site is a fishing community near Playas de Rosarito that is frequently visited by tourists and covered in Zostera eel grass beds. We selected three sampling sites at low tide (~1 m in depth each) on the Puerto Nuevo coastline with gradient exposures to human impact along a 0.45 km range between 32.248 N, -116.948 E and 32.246 N, -116.944 E (Fig 1). We refer to the most North-facing site at point 0.0 km as the Sheltered (SH) site, the site at point 0.15 km as the Minor Outlet (MN) site, and the site at point 0.3 km as the Major Outlet (MJ) site. The SH site is facing a 5–7 m cliff at point 0.0 km, the MN site is near a small run off outlet or scour at point 0.15 km, and the MJ site is near a large run off outlet and residential area at point 0.3 km. Four replicates of surface seawater samples and sediment core samples were collected at each site according to previously described methods [45]. Salinity, temperature (°C), pH, ammonia (ppm), nitrite (ppm), and nitrate (ppm), were measured for each site using the API Saltwater Master Test Kit.

Fig 1. Location and metadata information of sampling sites.

The three sampling sites are denoted in lime green (SH or sheltered), cyan (MN or Minor Outlet) and red (MJ or Major Outlet) circles. Sequenced samples based on seawater or sediment are displayed in the right-hand table columns for a total sequence output of 42 out of 48 samples submitted. The inset illustrates the approximate sampling location within Baja California, as denoted with a black circle. Chemical differences unique to sites are highlighted using colored boxes in the upper inset table and km refers to the distance in kilometers that MN and MJ are relative to SH.

Seawater samples (200 mL) were filtered on-site using sterile 60 mL syringes with 25 mm hydrophilic polyethersulfone 0.1-micron membrane filters (Supor-200 PES; Pall Laboratories) at an approximate rate of 15 mL/min. Filters were then transferred into individual, sterile 2 mL Eppendorf tubes, immediately frozen on dry ice, and stored at -80°C until further processing. For sediment cores, the tips of sterile 8.5 cm length x 1.5 cm diameter syringes were cut using sterile razor blades prior to being vertically inserted into the sediment. Sediment samples were then kept in their respective syringes and wrapped with Parafilm, immediately frozen on dry ice, and stored at -80°C until further processing. All samples were handled with sterile nitrile gloves both on- and off-site.

DNA extraction, PCR amplification for validation, and Illumina amplicon sequencing

DNA from the filters of 200 mL seawater samples was extracted using the QIAGEN DNeasy Blood & Tissue Kit (Qiagen, Valencia, CA, United States) following the manufacturer’s protocol. Filters were cut into 2 mm strips using sterilized scissors and the microbial content on the filter was homogenized using the Omni Bead Ruptor homogenizer (Omni International, Kennesaw, GA, United States) with a mixture of 0.1, 0.5, and 1.4 micron beads to maximize retrieval of DNA from all microbial domains. DNA from sediment samples was extracted from 0.5 g of field-moist sediment using the MoBio PowerSoil DNA Isolation Kit (MoBio, Carlsbad, CA, United States) following the manufacturer’s protocol. All extracted DNA from seawater and sediment samples was diluted to a final concentration of 5 ng per μL each.

Ribosomal RNA gene amplification was performed for all samples, including a variable 12 bp barcode sequence to ensure that samples were uniquely identifiable, following a standard protocol from the Department of Energy Joint Genome Institute (JGI) [46]. The V4-V5 region for 16S rRNA of bacteria and archaea (FW 515 F 5’- GTGYCAGCMGCCGCGGTAA-3’, RV 926R 5’- CCGYCAATTYMTTTRAGTTT-3’) and the V4 region for the 18S rRNA of eukaryotes (FW 5’- CCAGCASCYGCGGTAATTCC-3’, RV 5’- ACTTTCGTTCTTGATYRA-3’) were targeted, with sample validation amplifications to assess extraction quality [4751]. Stocks of 2x AccuStart II PCR SuperMix containing Taq DNA Polymerase (Quantabio, Beverly, MA, United States) and 10 mg/mL bovine serum albumin (BSA) (ThermoFisher Scientific, Waltham, MA, United States) were used during PCR amplification validation checks, conducted prior to amplicon sequencing. A final concentration of 1x SuperMix and 10 μg BSA was used for each 25 μL PCR reaction containing 10 ng DNA, 500 nM each for a given forward and reverse primer (1 μM total), and the remaining PCR reaction volume was made up to 25 μL with PCR grade nuclease-free water. The 16S rRNA region was amplified by denaturation at 94°C/3 min, followed by 30 cycles of denaturation 94°C/30 sec, annealing at 50°C/30 sec, elongation at 72°C/1 min, and a final elongation 72°C/10 min. The 18S rRNA region was amplified by denaturation at 94°C/3 min, followed by 30 cycles of denaturation 94°C/30 sec, annealing at 60°C/30 sec, elongation at 72°C/1.5 min, and a final elongation 72°C/10 min. After validation, 250 ng of extracted DNA in 50 μL total volume was used for plate-based next-generation 16S and 18S amplicon sequencing at the JGI using a KAPA Biosystem library qPCR kit and a Roche LightCycler 480 real-time PCR instrument with the same primers; a MiSeq Reagent kit using a 2x300 nt indexed protocol was used for sequencing on the Illumina MiSeq platform (Illumina, San Diego, CA, United States) [52]. Additional details for similar 16S and 18S sequencing protocols can be found on [53] and, respectively [54].

Sequence processing

Raw sequences were de-multiplexed and clustered into Operational Taxonomic Units (OTUs) using the iTagger v1.2 [49] and QIIME2 [55] pipelines for quality control and sequence analyses. Taxonomy was assigned by 97% identity or higher via the Silva database SSU for the 16S marker and SSU for the 18S r108 marker [46,49]. Identified and matched sequences were additionally filtered to remove mitochondrial DNA sequences. All remaining 16S and 18S rRNA gene sequences, with the sample having the lowest number of reads being 141944, were then rarefied at 1,000 reads per sample (23 output x 1,000 = 23,000 for 16S rRNA total rarefied reads and 21 output x 1,000 = 21,000 for 18S rRNA total rarefied reads; Fig 1 and S1 Fig). In sum, we submitted 24 samples for 16S and 18S sequencing (12 for seawater and 12 for sediment, containing 4 biological replicates per site), with an output of 23 datasets for 16S and 21 datasets for 18S.

Data analyses and statistics

Singleton and doubleton reads were removed before creating the two datasets per rRNA region (four in total). The four datasets include read abundance or presence-absence data, with 16S and 18S for each. The first dataset created was read abundance and the second was a conservative “presence = 1” or “absence = 0” assignment of rarefied reads (GitHub Supplemental-Results.Rmd code available at These metrics were then used to determine the biodiversity of each site (alpha diversity) and among sites (beta diversity). Abundant phyla and classes were classified and ranked into respective taxonomic groups. For diversity, we utilized Shannon’s and Simpson’s diversity indices based on read abundance. For abundance, we compared rarefied OTU reads of taxa by log fold. For richness, we assigned taxa as present or absent, then compiled taxa by phylogenetic group (i.e. phyla, class, order). For core taxa as indicators of the community, we took a DESeq2-like approach and compared taxa richness 16S or 18S across all samples versus sediment and seawater environment types versus SH, MN, and MJ site locations in order to define core taxa between three total categories: Puerto Nuevo core taxa, core taxa of environment type, and core taxa of location.

All statistical tests and visualizations were conducted in R [56] with all code and package citation information available at (S1S8 Tables). Changes in microbial community structure among sites were analyzed using permutational multivariate analysis of variance (PERMANOVA; [57]) with Bray-Curtis distances [58] for the abundance datasets and Jaccard indices [59] for the richness datasets. A Bonferroni p-value correction was used to determine pairwise differences between sites. Beta diversity differences in community structure and associated statistics were visualized using Venn diagrams and proportion of variance for principal components analysis (PCA) along two axes, grouped by environment type (sediment or seawater) versus location. For all univariate data, we used analysis of variance (ANOVA) to determine significant differences among sites, environment type, and site*environment type interactions. We used q-q plots and scale-location plots to inspect normality and homoscedasticity, respectively. Where significant differences were detected, Tukey’s Test of Honest Significant Differences was used to determine the range of differences among the sites and interactions.


Coastal Puerto Nuevo sample site metadata

We sampled four replicates of sediment and seawater from three sites within a 0.45 km range off the Puerto Nuevo coastline (Fig 1) and collected associated metadata at the interface where seawater meets sediment. The pH (7.9 ± 0.2), ammonia (0.08 ± 0.14 ppm) and nitrate (1.7 ± 2.9 ppm) levels, as well as temperature (15.8 ± 0.3°C) varied between sites during sampling in June 2016, whereas salinity (1.02 ± 0.00 psu), nitrite (0.0 ± 0.0 ppm), and depth (1.0 ± 0.0 m) were constant (S6 Table).

Microbial community diversity richness and abundance

A total of 14,137,026 raw reads were recovered from 23 of the 24 submitted seawater and sediment samples with median lengths of ~380 bp, publicly accessible upon free registration at the Joint Genome Institute Genome Portal, ID 502935 (S5 Table). 16S rRNA gene sequences were recovered for 11 of the 12 sediment samples (1,960,774 reads) and all of the 12 seawater samples (2,156,286 reads) for a total of 4,117,060 raw reads. 18S rRNA sequences were recovered for 9 of the 12 sediment samples (3,682,950 reads) and all of the 12 seawater samples (6,337,016 reads) for a total of 10,019,966 raw reads.

Shannon and Simpson diversity indices were produced from rarefied reads (S1 Fig), and all rarefied datasets passed the Shapiro-Wilk normality test (see GitHub Supplemental-Results.Rmd code available at The environment type (sediment or seawater) was found to be statistically significant for all 16S and 18S richness and abundance datasets (p < 0.005). Location was not statistically significant for any of the datasets, meaning that SH, MN or MJ did not significantly vary, although there was a correlation between environment type and site location observed for the 16S abundance dataset (p = 0.06). Focusing on environment type (sediment or seawater), analyses of reads by taking into account either raw or normalized sample mass indicated that microbial communities for sediment were orders of magnitude richer (approximately 500-fold) relative to those of seawater (Fig 2), regardless of how the data were analyzed. Taxa across domains are 2 fold richer and abundant in the sediment compared to seawater environment type. The sediment had 5.0x10^2 fold greater bacterial and archaeal taxa richness and 3.9x10^2 greater eukaryal taxa richness relative to seawater after normalization by mass. The sediment had 3.0x10^2 fold greater bacterial and archaeal taxa abundance and 2.7x10^2 greater eukaryal taxa abundance relative to seawater after normalization by mass.

Fig 2. Microbial community richness and abundance.

(a-b) Boxplot comparisons of rarefied bacterial and archaeal (16S) and eukaryal (18S) richness estimates for different environment types (sediment and seawater) and by sampling site (major outlet/MJ, minor outlet/MN, sheltered/SH), with a p value (p < 0.001) for environment type. (c-d) Boxplot comparisons of rarefied bacterial and archaeal (16S) and eukaryal (18S) abundance estimates for different environment types (sediment and seawater) and by sampling site (major outlet/MJ, minor outlet/MN, sheltered/SH), with a p value (p < 0.001) for environment type.

Microbial community composition

In total, the Puerto Nuevo microbial community composition during the time of sampling was comprised of 3 domains: Archaea, Bacteria, and Eukarya. For prokaryotes, there were 50 phyla, 130 classes, 240 orders, 441 families, and 859 genera represented. For eukaryotes, there were 30 phyla, 56 classes, 130 orders, 165 families, and 317 genera represented. Microbial communities revealed specific taxonomic assemblages associated with sediment versus seawater samples collected from the same sites (Figs 3 and 4, Table 1). Similar to OTU richness and abundance, PERMANOVA statistics indicated that microbial community composition differed by environment type (p = 0.001, f = 68.06 for prokaryote 16S and f = 25.09 for eukaryote 18S).

Fig 3. Microbial phyla by richness and abundance.

Top phyla by richness differ by environment type, with some abundance specificity by site location. (a-b) The top 10 bacterial and archaeal as well as eukaryal phyla across biological replicates of site locations for both seawater (SEA) and sediment (SED) environment types from most to least richness in the sediment in order of highest relative abundance to lowest. (c-d) The top 20 bacterial and archaeal as well as eukaryal classes, demonstrating variation in abundance by environment type and site location from a gray-scale gradient of white (0) to black (100). Common or rare phyla and classes can be additionally viewed by comparison of OTU tables.

Fig 4. Microbial community composition and beta-diversity.

Venn diagrams of percentage overlapping OTUs for bacterial and archaeal as well as eukaryal microbial communities based on richness, with site location colors corresponding to Fig 1. Statistically significant variation by PERMANOVA and pairwise comparison tests is shown in color whereas similarities (no variation) are shown as gray-scale.

Table 1. Shared (core) and unique core taxa for environment type and location.

Bacterial Proteobacteria and eukaryal Florideophycidae displayed higher richness in seawater, whereas Bacterial Bacteroides and Planctomycetes and eukaryal Ciliophora and Annelida had higher richness in sediment; richness of all other archaeal-, bacterial-, and eukaryal phyla did not differ substantially between environment types (Fig 3, S2 Fig). Cytophagia (bacterial) and Chromadorea (eukaryal) were abundant classes specific to the sediment environment, whereas Cyanobacteria and Bacteroidia (bacterial) and Chlorophyceae (eukaryal) were specific to the seawater environment. A further breakdown of taxa richness by pairwise comparisons revealed that the microbial community taxa richness was the same across domains and locations for sediment (p > 0.1, f < 1.25). For seawater, archaeal and bacterial community composition (p = 0.017, f = 2.09 for 16S seawater subset; MJ-SH p = 0.084 / f = 2.45 and MJ-MN p = 0.021 / f = 2.80) was distinct for the MJ site and all sites were distinct for eukaryal community composition (p = 0.003, f = 2.28 for 18S seawater subset; MJ-SH p = 0.054 / f = 2.06, MJ-MN p = 0.031 / f = 2.69, SH-MN p = 0.025 / f = 2.02) (Fig 4, S3 Fig).

Investigation of the Puerto Nuevo ‘core’ taxa–those consistently found across environment types (sediment or seawater) and locations–resulted in 47 genera and 50 unique OTU identifications (Table 1, S7 and S8 Tables). For prokaryotic domains, only Bacteria were part of the Puerto Nuevo core taxa–no core Archaea were observed. Across the two domains (Bacteria and Eukarya), 13 phyla were observed. Actinobacteria, Cyanobacteria, and Phyla 1002968 were core phyla specific to the seawater environment, whereas Chlorobi, Arthropod, Ciliophora, and Phyla 1003810 were specific to the sediment environment. Proteobacteria, Orchophta, Dinoflagellata, and Bacteroides were core phyla shared between both environment types. Three bacterial classes and one eukaryal class were core to seawater, and four bacterial classes and three eukaryal classes were specific to sediment. Bacterial Alphaproteobacteria, Flavobacteriia, and Gammaproteobacteria and eukaryal Diatomea and Dinophyceae were shared core classes between sediment and seawater. Three genera were core taxa specific to the SH and MJ site locations, with two of the three genera specific to other categories (Puerto Nuevo core community taxa and sediment core community taxa). No core taxa were specific to the MN site location.


Microbial communities in the coastal Baja California region are understudied relative to Western coastal regions, and community dynamics among multiple domains within Baja California were unknown prior to this study. We characterized sample diversity within (alpha diversity) and between (beta diversity) coastal microbial communities by examining bacteria, archaea and microbial eukaryotes in both the sediment and seawater of Puerto Nuevo, Baja California. Our findings support the hypotheses that: (1) the variation in diversity is greater in coastal sediment microbial communities than seawater microbial communities along a 0.45 km range and (2) prokaryotic and eukaryotic microbial communities exhibit similar composition patterns in coastal sediment but different composition patterns in seawater. Our findings that coastal communities differ among sample sites and between environment type (sediment, seawater) are consistent with global patterns of microbial biodiversity; for example, studies on the Baltic Sea coastline and the coral reef systems of Indonesia find similar patterns as our study [60,61]. Furthermore, our observed differences for bacterial, archaeal, and eukaryal microorganisms between sites within a small 0.45 km range illustrate the necessity for future studies to expand geographical and temporal sampling in this region to better understand the microbial ecology and biodiversity patterns of Puerto Nuevo, Baja California.

The finding that the sediment environment type exhibits higher bacterial richness when compared to seawater is consistent with previous literature investigating bacterial diversity in and along the Pacific [45,62,63], with less being known in this regard for archaeal and eukaryal microorganisms. These results could be explained by the physical nature of the sediment environment type, allowing for an increase in the formation of microbial mats and biofilms by providing a surface for microorganisms to attach. In addition, the sediment is composed of minerals, and as such it supports the electric coupling of complex microbial redox reactions, which may serve important roles in biogeochemical cycling and the maintenance of ecological homeostasis [64]. In general, sediment is a stratified solid gradient that provides niche stability to microorganisms, whereas seawater is a dynamic liquid that is constantly in flux. These two environment types, however, are not mutually exclusive; the seawater environment type is a necessary contributor to refreshing the microbial populations within coastal environments [65], including the sediment. We note that we used different extraction kits for seawater and sediment. While we did include a blank as a control for the seawater extraction kit and observed little to no detectable DNA in the blank sample, there is always the possibility of different levels of bias from the sequencing results of the DNA samples extracted using different extraction methods. Nonetheless, we observed some overlap of core taxa between seawater and sediment across sites (Table 1), which suggests an interaction between these communities. Additionally, we observed consistency in microbial community composition between sites, which is particularly interesting for sediment samples, since sediment samples often display microspatial heterogeneity [66,67]. Overall, our study provides the framework for future studies to examine the microbial composition and taxa preferences between and among multiple environment types at a particular location site, and is a starting point for understanding the underlying functional implications that these preferences may play within specific ecosystems.

We observed distinct core taxa present for coastal Puerto Nuevo with three eukaryal genera specific to the sediment core taxa of one or more sampling sites (Table 1). Interestingly, Nitzschia and Unknown 1001105 were core genera (found in the sediment) that distinguish the Sheltered (SH) and Major Outlet (MJ) sites from the Minor Outlet (MN) site. Nitzschia has been found in regions with observed elevated nitrogen levels [68], and is a known toxin-producing diatom in marine and freshwater environments. Licmophora is another diatom which, unlike Nitzschia, is negatively impacted by human nitrogen pollutants [69] and could be in competition with Nitzschia. Interestingly, Licmophora is found in both the sediment and seawater whereas Nitzschia is only observed in the sediment (Table 1). Both Nitzschia and Licmophora were the only genera that showed up multiple times as distinguished core taxa for Puerto Nuevo microbial communities, be it sediment or seawater specific communities, or sampling site specific communities. Further investigation into the metabolomic profiles of these genera in relation to detailed biogeochemistry in the environments they are found may reveal novel information into the significance of these taxa in Puerto Nuevo and other coastal microbial communities.

We observed that different patterns of microbial taxa primarily depend on the environment type rather than the sampling site (Figs 3 and 4, Table 1). Akin to sediment hosting greater microbial biodiversity than seawater, we found a common pattern with previous literature in that beta diversity appears to be more important than alpha diversity in determining microbial community composition across environment types [70,71]. Many soil microbial ecology studies agree that drivers of microbial beta diversity vary across space. In specific reference to coastal and marine microbial communities, Barberán and Casamayor (2010) found that the significance of beta diversity and its drivers vary by phylum when specifically investigating bacterial Actinobacteria, Alphaproteobacteria, Bacteroidetes, Betaproteobacteria, Cyanobacteria, and Gammaproteobacteria [72]. This seems to be a common observation, affirmed by current studies in vastly different coastal microbial communities [73,74]. Puerto Nuevo sediment microbial communities within a 0.45 km range do not significantly differ between sites or domains (16S and 18S), whereas seaweater eukaryal microbial communities do demonstrate heterogeneity for all sites, and bacterial and archaeal microbial communities specifically differ for the Major Outlet site (Fig 4). Explanation for these results may be rooted in the physical dynamics of coastal seawater compared to sediment. Indeed, several studies demonstrate how the microbial community composition of aquatic and marine environments depend on scale [60,75,76], and while we did not explicitly test for scale, we observed statistically significant community composition variation to exist even for small 0.45 km ranges. Moreover, our study is consistent with previous studies observing the mixing of marine and terrestrial communities, where coasts are unique interfaces for comparing the two interacting environments. While more studies comparing coastal seawater and sediment are needed, especially for microbial eukaryotes, a recent study [77] on a coastal environment of Southern China found similar patterns as we have found in this study for Puerto Nuevo in that the environment type and geographic location impacted the community composition, a finding that is analogous to previous studies focused exclusively on bacterial communities [28,60,73,76,78,79]. Another recent study in China’s coastal waters reported on the biogeography of microbial eukaryotes [80], further adding to our knowledge of microbial community composition studies.

Overall, our study is consistent with other studies, while providing new information on microbial diversity for Puerto Nuevo. For example, studies in other locations [81,81,82] found that Chlorobi, a photosynthesizing bacterial phylum that is known to contribute to sulfur cycling, is generally present in the sediment. Our results also indicated that Chlorobi are present in the sediment of Puerto Nuevo. Also consistent with other studies in other locations, the photosynthesizing Cyanobacteria have been observed to exist preferentially in seawater [8385], and we find this to be the case in Puerto Nuevo as well. In addition, Alphaproteobacteria and Gammaproteobacteria, which have been observed to be common phyla across multiple environment types in other regions [72,74,86,87], were also found in the sediment and seawater of Puerto Nuevo. While we do see archaea representative of abundant or rich taxa (Fig 3), we did not find any archaeal groups in the core taxa of Puerto Nuevo (Table 1). The lack of archaea in the core taxa of Puerto Nuevo is a novel finding in terms of marine microbial composition, and suggests that future studies should incorporate the inclusion of microbial eukaryotes in microbial community composition studies, as our results indicate that there is stronger co-occurrence between bacteria and microbial eukaryotes than between archaea and other domains.


In this investigation, we have expanded our understanding of microbial diversity and community composition in a near-shore marine environment of Baja California–a coastal region that has been generally understudied. Our analysis of coastal microbial communities just North of Puerto Nuevo, Baja California, which combined 16S and 18S rRNA gene sequencing approaches of coastal seawater and sediment, identified strong relationships between sampling sites and environment types consistent with previous studies. Our findings also highlight the differences of small scale (0.45 km) beta diversity, and demonstrate the significance of integrating multi- domain, environment type, and sampling sites into microbial composition studies to provide ecological context to microbial biodiversity potentially impacted by human-induced climate change and development.

Supporting information

S1 Table. Taxa corresponding to 16S OTU data.

Assigned prokaryotic taxonomy for 16S OTUs.


S2 Table. Taxa corresponding to 18S OTU data.

Assigned microbial eukaryotic taxonomy for 18S OTUs.


S3 Table. Rarefied 16S reads for sediment and seawater samples.

16S reads, rarefied to 1000, for coastal Puerto Nuevo sediment and seawater samples.


S4 Table. Rarefied 18S reads for sediment and seawater samples.

18S reads, rarefied to 1000, for coastal Puerto Nuevo sediment and seawater samples.


S5 Table. Metadata for amplicon reads.

Metadata and number of raw reads for 16S and 18S OTU sequences.


S6 Table. Metadata for site locations.

Metadata for coastal Puerto Nuevo site locations.


S7 Table. Output table for 16S core taxa.

Full output table for 16S core taxa found along coastal Puerto Nuevo.


S8 Table. Output table for 18S core taxa.

Full output table for 18S core taxa found along coastal Puerto Nuevo.


S1 Fig. Metrics and rarefaction curves on read abundance.

Read abundance histograms of prokaryotic 16S (a) and eukaryotic 18S (d) Simpson’s diversity, histograms of prokaryotic 16S (b) and eukaryotic 18S (e) Shannon’s diversity, and rarefaction curves of all prokaryotic 16S (c) and eukaryotic 18S (f) operational taxonomic units versus number of reads.


S2 Fig. Top 20 phyla per site location.

Boxplots display top 20 (a) bacterial and archaeal 16S phyla and (b) eukaryal 18S phyla by richness.


S3 Fig. Microbial community variations per site location.

Principal component analysis (PCA) plots of PC1 x PC2 show variation versus similarity of microbial communities between site locations for (a) bacterial and archaeal 16S in the sediment and (b) seawater and (c) eukaryal 18S in the sediment and (d) seawater.



We thank researchers at the Scientific Research Center and Higher Education of Ensenada (CICESE) and researchers Christa Pennacchio, Nicholas C. Dove, Franz Krah, Dr. Jesse Wilson, Dr. Megha Gulati, Dr. Stephen C. Hart, Jorge Montiel, Lisa J. Cohen, Michael E. Malloy, and Jessica M. Blanton.


  1. 1. Bauer JE, Cai W-J, Raymond PA, Bianchi TS, Hopkinson CS, Regnier PAG. The changing carbon cycle of the coastal ocean. Nature. 2013;504: 61–70. pmid:24305149
  2. 2. Wallenstein MD, Myrold DD, Firestone M, Voytek M. Environmental Controls on Denitrifying Communities and Denitrification Rates: Insights from Molecular Methods. Ecol Appl. 16: 2143–2152. pmid:17205893
  3. 3. Ghaisas S, Maher J, Kanthasamy A. Gut microbiome in health and disease: Linking the microbiome–gut–brain axis and environmental factors in the pathogenesis of systemic and neurodegenerative diseases. Pharmacol Ther. 2016;158: 52–62. pmid:26627987
  4. 4. McFall-Ngai MJ. The Importance of Microbes in Animal Development: Lessons from the Squid-Vibrio Symbiosis. Annu Rev Microbiol. 2014;68: 177–194. pmid:24995875
  5. 5. Bowen JL, Weisman D, Yasuda M, Jayakumar A, Morrison HG, Ward BB. Marine Oxygen-Deficient Zones Harbor Depauperate Denitrifying Communities Compared to Novel Genetic Diversity in Coastal Sediments. Microb Ecol. 2015;70: 311–321. pmid:25721726
  6. 6. Fuhrman JA, Cram JA, Needham DM. Marine microbial community dynamics and their ecological interpretation. Nat Rev Microbiol. 2015;13: 133. pmid:25659323
  7. 7. Hollibaugh JT, Gifford SM, Moran MA, Ross MJ, Sharma S, Tolar BB. Seasonal variation in the metratranscriptomes of a Thaumarchaeota population from SE USA coastal waters. ISME J. 2014;8: 685–698. pmid:24132081
  8. 8. Moulton OM, Altabet MA, Beman JM, Deegan LA, Lloret J, Lyons MK, et al. Microbial associations with macrobiota in coastal ecosystems: patterns and implications for nitrogen cycling. Front Ecol Environ. 2016;14: 200–208.
  9. 9. Petro C, Starnawski P, Schramm A, Kjeldsen KU. Microbial community assembly in marine sediments. Aquat Microb Ecol. 2017;79: 177–195.
  10. 10. Haskell William Z., Prokopenko Maria G., Hammond Douglas E., Stanley Rachel H. R., Sandwith Zoe O. Annual cyclicity in export efficiency in the inner Southern California Bight. Glob Biogeochem Cycles. 2017;31: 357–376.
  11. 11. He Y, Sen B, Zhou S, Xie N, Zhang Y, Zhang J, et al. Distinct Seasonal Patterns of Bacterioplankton Abundance and Dominance of Phyla α-Proteobacteria and Cyanobacteria in Qinhuangdao Coastal Waters Off the Bohai Sea. Front Microbiol. 2017;8. pmid:28868051
  12. 12. Jessup CM, Kassen R, Forde SE, Kerr B, Buckling A, Rainey PB, et al. Big questions, small worlds: microbial model systems in ecology. Trends Ecol Evol. 2004;19: 189–197. pmid:16701253
  13. 13. Kaestli M, Skillington A, Kennedy K, Majid M, Williams D, McGuinness K, et al. Spatial and Temporal Microbial Patterns in a Tropical Macrotidal Estuary Subject to Urbanization. Front Microbiol. 2017;8. pmid:28751882
  14. 14. Kavagutti VS. Biotic factors drive bacterioplankton community in a tropical coastal site of the equatorial atlantic ocean. 2016; Available:
  15. 15. Kirchman DL. Growth Rates of Microbes in the Oceans. Annu Rev Mar Sci. 2016;8: 285–309. pmid:26195108
  16. 16. Prosser JI, Bohannan BJM, Curtis TP, Ellis RJ, Firestone MK, Freckleton RP, et al. The role of ecological theory in microbial ecology. Nat Rev Microbiol. 2007;5: 384–392. pmid:17435792
  17. 17. Whitton BA, Potts M. The Ecology of Cyanobacteria: Their Diversity in Time and Space. Springer Science & Business Media; 2007.
  18. 18. Brussaard CPD, Bidle KD, Pedrós-Alió C, Legrand C. The interactive microbial ocean. In: Nature Microbiology [Internet]. 20 Dec 2016 [cited 8 Apr 2018]. pmid:27995930
  19. 19. Hunt DE, Ward CS. A network-based approach to disturbance transmission through microbial interactions. Front Microbiol. 2015;6. pmid:26579091
  20. 20. Angell JH, Peng X, Ji Q, Craick I, Jayakumar A, Kearns PJ, et al. Community Composition of Nitrous Oxide-Related Genes in Salt Marsh Sediments Exposed to Nitrogen Enrichment. Front Microbiol. 2018;9. pmid:29483902
  21. 21. Galloway JN, Dentener FJ, Capone DG, Boyer EW, Howarth RW, Seitzinger SP, et al. Nitrogen Cycles: Past, Present, and Future. Biogeochemistry. 2004;70: 153–226.
  22. 22. Gradoville Mary R., Bombar Deniz, Crump Byron C., Letelier Ricardo M., Zehr Jonathan P., White Angelicque E. Diversity and activity of nitrogen‐fixing communities across ocean basins. Limnol Oceanogr. 2017;62: 1895–1909.
  23. 23. Cowan MK. Microbiology: a systems approach; Fifth Edition. [Internet]. McGraw-Hill; 2018. Available:
  24. 24. Röling WFM, Ferrer M, Golyshin PN. Systems approaches to microbial communities and their functioning. Curr Opin Biotechnol. 2010;21: 532–538. pmid:20637597
  25. 25. Kuzyakov Y, Blagodatskaya E. Microbial hotspots and hot moments in soil: Concept & review. Soil Biol Biochem. 2015;83: 184–199.
  26. 26. Hedges JI, Oades JM. Comparative organic geochemistries of soils and marine sediments. Org Geochem. 1997;27: 319–361.
  27. 27. Aleklett K, Kiers ET, Ohlsson P, Shimizu TS, Caldas VE, Hammer EC. Build your own soil: exploring microfluidics to create microbial habitat structures. ISME J. 2018;12: 312–319. pmid:29135971
  28. 28. Hill TCJ, Walsh KA, Harris JA, Moffett BF. Using ecological diversity measures with bacterial communities. FEMS Microbiol Ecol. 2003;43: 1–11. pmid:19719691
  29. 29. Bolhuis H, Cretoiu MS, Stal LJ. Molecular ecology of microbial mats. FEMS Microbiol Ecol. 2014;90: 335–350. pmid:25109247
  30. 30. Lu X-M, Chen C, Zheng T-L. Metagenomic Insights into Effects of Chemical Pollutants on Microbial Community Composition and Function in Estuarine Sediments Receiving Polluted River Water. Microb Ecol. 2017;73: 791–800. pmid:27744476
  31. 31. Spalding MD, Fox HE, Allen GR, Davidson N, Ferdaña ZA, Finlayson M, et al. Marine Ecoregions of the World: A Bioregionalization of Coastal and Shelf Areas. BioScience. 2007;57: 573–583.
  32. 32. Martiny JBH, Bohannan BJM, Brown JH, Colwell RK, Fuhrman JA, Green JL, et al. Microbial biogeography: putting microorganisms on the map. Nat Rev Microbiol. 2006;4: nrmicro1341. pmid:16415926
  33. 33. Bakun A. Global Climate Change and Intensification of Coastal Ocean Upwelling. Science. 1990;247: 198–201. pmid:17813287
  34. 34. Bakun A, Black BA, Bograd SJ, García-Reyes M, Miller AJ, Rykaczewski RR, et al. Anticipated Effects of Climate Change on Coastal Upwelling Ecosystems. Curr Clim Change Rep. 2015;1: 85–93.
  35. 35. Capone DG, Hutchins DA. Microbial biogeochemistry of coastal upwelling regimes in a changing ocean. Nat Geosci. 2013;6: 711–717.
  36. 36. Huerta-Diaz MA, Delgadillo-Hinojosa F, Otero XL, Segovia-Zavala JA, Hernandez-Ayon JM, Galindo-Bect MS, et al. Iron and Trace Metals in Microbial Mats and Underlying Sediments: Results From Guerrero Negro Saltern, Baja California Sur, Mexico. Aquat Geochem. 2011;17: 603.
  37. 37. Huerta-Diaz MA, Delgadillo-Hinojosa F, Siqueiros-Valencia A, Valdivieso-Ojeda J, Reimer JJ, Segovia-Zavala JA. Millimeter-scale resolution of trace metal distributions in microbial mats from a hypersaline environment in Baja California, Mexico. Geobiology. 2012;10: 531–547. pmid:22989089
  38. 38. López-Cortés A, García-Pichel F, Nübel U, Vázquez-Juárez R. Cyanobacterial diversity in extreme environments in Baja California, Mexico: a polyphasic study. Int Microbiol. 2001;4: 227–236. pmid:12051567
  39. 39. Martini AM, Walter LM, Lyons TW, Hover VC, Hansen J. Significance of early-diagenetic water-rock interactions in a modern marine siliciclastic/evaporite environment: Salina Ometepec, Baja California. GSA Bull. 2002;114: 1055–1069.
  40. 40. Omoregie EO, Crumbliss LL, Bebout BM, Zehr JP. Determination of Nitrogen-Fixing Phylotypes in Lyngbya sp. and Microcoleus chthonoplastes Cyanobacterial Mats from Guerrero Negro, Baja California, Mexico. Appl Environ Microbiol. 2004;70: 2119–2128. pmid:15066804
  41. 41. Omoregie EO, Crumbliss LL, Bebout BM, Zehr JP. Comparison of diazotroph community structure in Lyngbya sp. and Microcoleus chthonoplastes dominated microbial mats from Guerrero Negro, Baja, Mexico. FEMS Microbiol Ecol. 2004;47: 305–308. pmid:19712319
  42. 42. Orphan VJ, Jahnke LL, Embaye T, Turk KA, Pernthaler A, Summons RE, et al. Characterization and spatial distribution of methanogens and methanogenic biosignatures in hypersaline microbial mats of Baja California. Geobiology. 2008;6: 376–393. pmid:18564187
  43. 43. Reimer JJ, Huerta-Diaz MA. Phosphorus Speciation and Sedimentary Fluxes in Hypersaline Sediments of the Guerrero Negro Salt Evaporation Area, Baja California Sur, Mexico. Estuaries Coasts. 2011;34: 514–528.
  44. 44. Valdivieso-Ojeda JA, Huerta-Diaz MA, Delgadillo-Hinojosa F. High enrichment of molybdenum in hypersaline microbial mats of Guerrero Negro, Baja California Sur, Mexico. Chem Geol. 2014;363: 341–354.
  45. 45. Walsh EA, Kirkpatrick JB, Rutherford SD, Smith DC, Sogin M, D’Hondt S. Bacterial diversity and community composition from seasurface to subseafloor. ISME J. 2015;10: ismej2015175. pmid:26430855
  46. 46. 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–D596. pmid:23193283
  47. 47. Parada AE, Needham DM, Fuhrman JA. Every base matters: assessing small subunit rRNA primers for marine microbiomes with mock communities, time series and global field samples. Environ Microbiol. 2016;18: 1403–1414. pmid:26271760
  48. 48. Stoeck T, Bass D, Nebel M, Christen R, Jones MDM, Breiner H-W, et al. Multiple marker parallel tag environmental DNA sequencing reveals a highly complex eukaryotic community in marine anoxic water. Mol Ecol. 2010;19 Suppl 1: 21–31. pmid:20331767
  49. 49. Tremblay J, Singh K, Fern A, Kirton ES, He S, Woyke T, et al. Primer and platform effects on 16S rRNA tag sequencing. Front Microbiol. 2015;6. pmid:26300854
  50. 50. Bates ST, Berg-Lyons D, Caporaso JG, Walters WA, Knight R, Fierer N. Examining the global distribution of dominant archaeal populations in soil. ISME J. 2011;5: 908–917. pmid:21085198
  51. 51. Quince C, Lanzen A, Davenport RJ, Turnbaugh PJ. Removing Noise From Pyrosequenced Amplicons. BMC Bioinformatics. 2011;12: 38. pmid:21276213
  52. 52. Caporaso JG, Lauber CL, Walters WA, Berg-Lyons D, Huntley J, Fierer N, et al. Ultra-high-throughput microbial community analysis on the Illumina HiSeq and MiSeq platforms. ISME J. 2012;6: 1621–1624. pmid:22402401
  53. 53. Thompson L. EMP 16S Illumina Amplicon Protocol [Internet]. [cited 25 Jan 2019].
  54. 54. Thompson L. EMP 18S Illumina Amplicon Protocol [Internet]. [cited 25 Jan 2019].
  55. 55. Bokulich NA, Kaehler BD, Rideout JR, Dillon M, Bolyen E, Knight R, et al. Optimizing taxonomic classification of marker gene sequences [Internet]. PeerJ Preprints; 2017 Aug. Report No.: e3208v1.
  56. 56. Core R Team D. R: A Language and Environment for Statistical Computing. 2011.
  57. 57. Anderson MJ. Permutation tests for univariate or multivariate analysis of variance and regression. Can J Fish Aquat Sci. 2001;58: 626–639.
  58. 58. Bray JR, Curtis JT. An Ordination of the Upland Forest Communities of Southern Wisconsin. Ecol Monogr. 1957;27: 325–349.
  59. 59. Jaccard P. The Distribution of the Flora in the Alpine Zone.1. New Phytol. 1912;11: 37–50.
  60. 60. Langenheder S, Ragnarsson H. The Role of Environmental and Spatial Factors for the Composition of Aquatic Bacterial Communities. Ecology. 2007;88: 2154–2161. pmid:17918394
  61. 61. Hao Y-Q, Zhao X-F, Zhang D-Y. Field experimental evidence that stochastic processes predominate in the initial assembly of bacterial communities. Environ Microbiol. 2016;18: 1730–1739. pmid:25809418
  62. 62. Cleary DFR, Polónia ARM, Becking LE, Voogd NJ de, Purwanto, Gomes H, et al. Compositional analysis of bacterial communities in seawater, sediment, and sponges in the Misool coral reef system, Indonesia. Mar Biodivers. 2017; 1–13.
  63. 63. Daly NL, Seymour J, Wilson D. Exploring the therapeutic potential of jellyfish venom. Future Med Chem. 2014;6: 1715–1724. pmid:25406009
  64. 64. Nielsen LP, Risgaard-Petersen N. Rethinking Sediment Biogeochemistry After the Discovery of Electric Currents. Annu Rev Mar Sci. 2015;7: 425–442. pmid:25251266
  65. 65. Won N-I, Kim K-H, Kang JH, Park SR, Lee HJ. Exploring the Impacts of Anthropogenic Disturbance on Seawater and Sediment Microbial Communities in Korean Coastal Waters Using Metagenomics Analysis. Int J Environ Res Public Health. 2017;14: 130. pmid:28134828
  66. 66. Stoyan H, De-Polli H, Böhm S, Robertson GP, Paul EA. Spatial heterogeneity of soil respiration and related properties at the plant scale. Plant Soil. 2000;222: 203–214.
  67. 67. Downing JA, Rath LC. Spatial patchiness in the lacustrine sedimentary environment1. Limnol Oceanogr. 1988;33: 447–458.
  68. 68. Machado RJA, Estrela AB, Nascimento AKL, Melo MMA, Torres-Rêgo M, Lima EO, et al. Characterization of TistH, a multifunctional peptide from the scorpion Tityus stigmurus: Structure, cytotoxicity and antimicrobial activity. Toxicon. 2016;119: 362–370. pmid:27267248
  69. 69. The effect of fertilizer on the growth rate of the diatom Licmophora abbreviata | The Expedition. Available:
  70. 70. Li H, Li T, Beasley DE, Heděnec P, Xiao Z, Zhang S, et al. Diet Diversity Is Associated with Beta but not Alpha Diversity of Pika Gut Microbiota. Front Microbiol. 2016;7. pmid:27512391
  71. 71. Prober SM, Leff JW, Bates ST, Borer ET, Firn J, Harpole WS, et al. Plant diversity predicts beta but not alpha diversity of soil microbes across grasslands worldwide. Ecol Lett. 2015;18: 85–95. pmid:25430889
  72. 72. Barberán A, Casamayor EO. Global phylogenetic community structure and β-diversity patterns in surface bacterioplankton metacommunities. Aquat Microb Ecol. 2010;59: 1–10.
  73. 73. Campbell AM, Fleisher J, Sinigalliano C, White JR, Lopez JV. Dynamics of marine bacterial community diversity of the coastal waters of the reefs, inlets, and wastewater outfalls of southeast Florida. MicrobiologyOpen. 2015;4: 390–408. pmid:25740409
  74. 74. Richa K, Balestra C, Piredda R, Benes V, Borra M, Passarelli A, et al. Distribution, community composition and potential metabolic activity of bacterioplankton in an urbanized Mediterranean Sea coastal zone. Appl Env Microbiol. 2017; AEM.00494-17. pmid:28667110
  75. 75. Green J, Bohannan BJM. Spatial scaling of microbial biodiversity. Trends Ecol Evol. 2006;21: 501–507. pmid:16815589
  76. 76. Lozupone CA, Knight R. Global patterns in bacterial diversity. Proc Natl Acad Sci. 2007;104: 11436–11440. pmid:17592124
  77. 77. Chen W, Pan Y, Yu L, Yang J, Zhang W. Patterns and Processes in Marine Microeukaryotic Community Biogeography from Xiamen Coastal Waters and Intertidal Sediments, Southeast China. Front Microbiol. 2017;8. pmid:29075237
  78. 78. Martiny JBH, Eisen JA, Penn K, Allison SD, Horner-Devine MC. Drivers of bacterial β-diversity depend on spatial scale. Proc Natl Acad Sci. 2011;108: 7850–7854. pmid:21518859
  79. 79. O’Brien SL, Gibbons SM, Owens SM, Hampton‐Marcell J, Johnston ER, Jastrow JD, et al. Spatial scale drives patterns in soil bacterial diversity. Environ Microbiol. 2016;18: 2039–2051. pmid:26914164
  80. 80. Zhang H, Huang X, Huang L, Bao F, Xiong S, Wang K, et al. Microeukaryotic biogeography in the typical subtropical coastal waters with multiple environmental gradients. Sci Total Environ. 2018;635: 618–628. pmid:29679834
  81. 81. Camanocha A, Dewhirst FE. Host-associated bacterial taxa from Chlorobi, Chloroflexi, GN02, Synergistetes, SR1, TM7, and WPS-2 Phyla/candidate divisions. J Oral Microbiol. 2014;6: 25468. pmid:25317252
  82. 82. Wasmund K, Cooper M, Schreiber L, Lloyd KG, Baker BJ, Petersen DG, et al. Single-Cell Genome and Group-Specific dsrAB Sequencing Implicate Marine Members of the Class Dehalococcoidia (Phylum Chloroflexi) in Sulfur Cycling. mBio. 2016;7: e00266–16. pmid:27143384
  83. 83. Yonghui Gao, Cornwell Jeffrey C., Stoecker DK, Owens Michael S. Influence of cyanobacteria blooms on sediment biogeochemistry and nutrient fluxes. Limnol Oceanogr. 2014;59: 959–971.
  84. 84. Makhalanyane TP, Valverde A, Velázquez D, Gunnigle E, Goethem MWV, Quesada A, et al. Ecology and biogeochemistry of cyanobacteria in soils, permafrost, aquatic and cryptic polar habitats. Biodivers Conserv. 2015;24: 819–840.
  85. 85. Paerl H. The cyanobacterial nitrogen fixation paradox in natural waters. F1000Research. 2017;6. pmid:28357051
  86. 86. Franco DC, Signori CN, Duarte RTD, Nakayama CR, Campos LS, Pellizari VH. High Prevalence of Gammaproteobacteria in the Sediments of Admiralty Bay and North Bransfield Basin, Northwestern Antarctic Peninsula. Front Microbiol. 2017;8. pmid:28210255
  87. 87. Sun MY, Dafforn KA, Johnston EL, Brown MV. Core sediment bacteria drive community response to anthropogenic contamination over multiple environmental gradients. Environ Microbiol. 2013;15: 2517–2531. pmid:23647974