Skip to main content
Browse Subject Areas

Click through the PLOS taxonomy to find articles in your field.

For more information about PLOS Subject Areas, click here.

  • Loading metrics

A first molecular characterization of the scorpion telson microbiota of Hadrurus arizonensis and Smeringurus mesaensis

  • Christopher Shimwell ,

    Contributed equally to this work with: Christopher Shimwell, Lauren Atkinson

    Roles Investigation, Writing – original draft, Writing – review & editing

    Current address: Physician Assistant Program, Yale School of Medicine, New Haven, CT, United States of America

    Affiliation Department of Biology, Eastern Connecticut State University, Willimantic, CT, United States of America

  • Lauren Atkinson ,

    Contributed equally to this work with: Christopher Shimwell, Lauren Atkinson

    Roles Investigation, Writing – original draft, Writing – review & editing

    Current address: Department of Molecular Biosciences, University of Kansas, Lawrence, Kansas, United States of America

    Affiliation Department of Biology, Eastern Connecticut State University, Willimantic, CT, United States of America

  • Matthew R. Graham,

    Roles Formal analysis, Funding acquisition, Resources, Writing – review & editing

    Affiliation Department of Biology, Eastern Connecticut State University, Willimantic, CT, United States of America

  • Barbara Murdoch

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

    Affiliation Department of Biology, Eastern Connecticut State University, Willimantic, CT, United States of America


Scorpions represent an ancient lineage of arachnids that have radiated across the globe and are incredibly resilient—since some thrive in harsh environments and can exist on minimal and intermittent feedings. Given the emerging importance of microbiomes to an organism’s health, it is intriguing to suggest that the long-term success of the scorpion bauplan may be linked to the microbiome. Little is known about scorpion microbiomes, and what is known, concentrates on the gut. The microbiome is not limited to the gut, rather it can be found within tissues, fluids and on external surfaces. We tested whether the scorpion telson, the venom-producing organ, of two species, Smeringurus mesaensis and Hadrurus arizonensis, contain bacteria. We isolated telson DNA from each species, amplified bacterial 16S rRNA genes, and identified the collection of bacteria present within each scorpion species. Our results show for the first time that telsons of non-buthid scorpion species do indeed contain bacteria. Interestingly, each scorpion species has a phylogenetically unique telson microbiome including Mollicutes symbionts. This study may change how we view scorpion biology and their venoms.


Scorpions are an ancient lineage that originated over 400 million years ago, compared to a mere 0.2–1.5 million years for humans [1, 2]. Scorpions are divided into 2 major groups, Buthida and Iurida, that are further subdivided into 22 families. Given the emerging importance of microbiomes to an organism’s health [35], it is intriguing to suggest that the antiquity of scorpions and their success in colonizing terrestrial environments around the globe may be linked to their microbial symbionts [6, 7]. Although investigations of bacterial symbionts in scorpions are rare, a collection of important information is beginning to emerge. Early efforts isolated DNA from a variety of tissues or whole organisms as a PCR template, using primers for single or multiple genes that were specifically targeted to a single bacterial genus. Sanger sequencing identified the PCR targets. Using this approach, Wolbachia has been reported in scorpions representing families Buthidae [8], Hemiscorpiidae [9], and Scorpionidae [10]. However, a screening of common arachnid endosymbionts, specifically Wolbachia, Cardinium, Rickettsia and Spiroplasma, yielded no positive results in 61 samples of the scorpion family Vaejovidae, with a cautionary note regarding off-targets of some primers [11]. Although these studies contributed to our knowledge of the distribution of a single or limited number of bacterial genera in scorpion tissues, a broader survey of taxa was needed.

To acquire a wider-ranging survey of bacterial taxa, subsequent studies used PCR primers that targeted the 16S rRNA gene of numerous bacteria, followed by subcloning into plasmid vectors and Sanger sequencing. Intermediate steps designed to reduce the number of duplicate clones sequenced included either restriction enzyme digest [12] or denaturing gradient gel electrophoresis [13]. With these approaches, taxa detected in the gut microbiota of Centruroides limpidus and Vaejovis smithi included a predominance of Proteobacteria, in addition to Firmicutes, Actinobacteria and Spirochaetes [12]. In contrast, in Androctonus australis the gut and gonads included Firmicutes, Proteobacteria, Actinobacteria and Cyanobacteria, with Mollicutes being the most prevalent at 95% of all clones [13].

Novel lineages of Mollicutes have been described from gut tissue of C. limpidus and V. smithi [12]. One lineage termed Scorpion Group 1 (SG1) was found in V. smithi, but absent in C. limpidus, and had a 79% identity to Spiroplasma lampyridicola. Two other lineages, one in V. smithi, the other in C. limpidus, were Mycoplasma-related, being 88% identical to Mycoplasma hyorhinis. These 2 lineages together form a clade termed the Scorpion Mycoplasma Clade (SMC) [12]. Phylotypes corresponding to SMC have also been detected in A. australis [13].

A more detailed analysis using lineage-specific PCR primers and Sanger sequencing tested 23 scorpion morphospecies for the SG1 and SMC lineages [14]. The SMC lineage was detected in samples from both the Vaejovidae and Buthidae families, including V. smithi and C. limpidus, confirming their previous results [12]. SG1 was only detected in Vaejovidae, including additional Vaejovis and Mesomexovis species.

Beyond the SG1 lineage, additional Spiroplasma-like phylotypes have been detected in C. limpidus, A. australis and Diplocentrus duende scorpions. Centruroides limpidus contained a sequence 88% identical to Spiroplasma platyhelix that formed a clade with a sequence from a vinegaroon, Mastigoproctus sp. [14]. Spiroplasma sequences found in A. australis and D. duende were similar and grouped with a Citri-Chrysopicola-Mirum clade, thought to be derived from insect endosymbionts [14]. Whether Mycoplasma- and Spiroplasma-like phylotypes occur in other scorpion species is unknown.

The venom of venomous organisms has long intrigued researchers regarding its potential for clinically relevant natural products [15]. Venom-microbiomics is a newly emerging field that seeks to study venom-associated microbes found in a variety of different organisms, including snakes, spiders, insects, fish, etc [16]. Given that in some organisms venom toxicity can be enhanced by endogenous bacteria, that scorpion stings can result in bacterial infections [17], and scorpion venom contains antimicrobial compounds that can be produced by bacteria [1821], it seems plausible that the venom-producing appendage, the telson, would harbor bacteria. To date there are few reports of bacteria in the telson. Attempts to grow bacteria from the venom of H. arizonensis and Heterometrus spinifer were inconsistent due in part to the variable and small volumes of venom isolated, despite having success culturing bacteria from the venom of numerous snake species [22, 23]. Wolbachia was detected in 10/20 (50%) of venom gland samples of the highly cytotoxic Hemiscorpius lepturus [9], however the study did not assess taxa beyond this single genus. In a separate report, the telson from the Old World buthid A. australis, a dangerously neurotoxic species, documented representatives belonging to Firmicutes, Actinobacteria, Proteobacteria and Flavobacteria taxa [13], although the sample size was limited to 3 animals and 7 bacterial isolates in total [13]. None of the telson samples represented bacterial class Mollicutes.

In this study we characterized the microbial diversity in telsons from 2 New World scorpion species representing different families, Smeringurus mesaensis of Vaejovidae and Hadrurus arizonensis of Hadruridae [24]. We used polymerase chain reaction (PCR) to create libraries of 16S rRNA gene sequences, commonly used in microbial barcoding, followed by sequencing to allocate taxonomic assignments. Phylogenetic analysis shows a rich diversity of bacteria in scorpion telsons, that are mostly species-specific, and have representatives from previously identified and novel Mollicutes phylotypes.

Materials and methods

Scorpion collection and dissection

We collected H. arizonenesis (Fig 1A and 1B; n = 7) from just east of Cattail Cove State Park, AZ (34.356159°, -114.147638°) and S. mesaensis (Fig 1C; n = 4) from Borrego Springs, CA (33.280283°, -116.292855°). For arachnid-related studies such as this, no ethics approval is required. The scorpions were held in captivity for 3–5 weeks without food or water, prior to freezing at -80°C until needed. During their captivity, each scorpion was housed individually within their own plastic container, to minimize contamination between scorpions. The scorpion exoskeleton was washed with 70% ethanol followed by water two times [12], prior to isolating telsons for DNA extraction. Under a dissecting microscope using sterile dissection tools, the telson was cut away from the rest of the metasoma and the aculeus was removed. The telson was subsequently bisected longitudinally to split it open, thus exposing the tissue inside. The dissection tools were sprayed with 70% ethanol and air-dried, prior to removal of the telson tissue. Sample tissue isolated for DNA extraction was referred to as venom gland or telson tissue, but could include the venom and venom gland tissue, plus the surrounding tissue, and the hemolymph. For each telson, the tissues were transferred to sterile 1.5 ml Eppendorf tubes in preparation for DNA extraction.

Fig 1. Images of H. arizonensis and S. mesaensis.

Images of A, B) H. arizonensis with an enlarged view of its telson and stinger, and C) S. mesaensis.

DNA extraction from scorpion telsons

A modified Epicentre Master Pure DNA Purification (Lucigen) protocol was used to extract DNA from the scorpion telsons. Tissues were cut into small pieces, placed on ice and each sample was mixed with 300 μl Tissue and Cell Lysis Buffer and 50 μg Proteinase K. Samples were homogenized using a sterile cell homogenizer until a liquid suspension was made. Samples were incubated overnight in a 56°C shaking water bath. Each sample was iced and mixed vigorously with 175 μl of MPC Protein Precipitation Reagent and then centrifuged at 10,000 x g for 10 minutes at 4°C. Supernatants were mixed with 500 μl of cold -20°C isopropanol and stored at -20°C for 30 minutes to overnight. Samples were warmed to 4°C and centrifuged at 10,000 x g for 10 minutes at 4°C to pellet the DNA. Supernatants were decanted, and the pellets were washed twice with 70% ethanol. The pellets were air dried for 30 minutes and resuspended in 50 μL of TE buffer (10 mM Tris, 1 mM EDTA, pH 8).

Amplification of 16S rRNA gene from scorpion telsons

Isolated DNA samples were subjected to PCR to test for the presence of bacteria in scorpion telsons using the 63F/1387R primers that specifically amplify the bacterial 16S rRNA gene from complex mixtures [25]. PCR mixtures of 25 μl contained the following: 50 to 200 ng of DNA template, 0.5 μM of each primer, 200 μM dNTPs, 2.5 units of Taq DNA Polymerase, 20 mM Tris and 50 mM KCl buffer, and 1.5 mM MgCl. The reaction conditions were 96°C for five minutes, 30 cycles at 94°C for 60 seconds, 58°C for 60 seconds, 72°C for one minute and 50 seconds, and a subsequent final extension at 72°C for 10 minutes. Electrophoresis of the PCR products (~1.4 kb 16S rRNA gene) was performed on a 1% (w/v) agarose gel in TAE with SYBR-Safe (1:10,000 Invitrogen). Gels were visualized with GelDoc (BioRad) software. Fresh PCR amplicons were used for TOPO cloning.

TOPO TA cloning and transformation

TOPO TA cloning acts to separate the collection of 16S rRNA sequences found within the PCR amplicons into individual sequences by subcloning the sequences into plasmid vectors and growing the plasmids in bacteria [12]. DNA extracted from individual bacterial colonies serves as the template for a second vector-based PCR prior to Sanger sequencing, as described below. TOPO TA cloning (Invitrogen) was performed according to the manufacturer’s suggestions. Briefly, the reagents below were added to a tube in the order shown: 1 μL of fresh PCR product, 1 μL salt solution, 3 μL of water, and 1 μL of Invitrogen pCR® 4-TOPO® cloning plasmid. The reaction was mixed and incubated at room temperature for 30 minutes. The reactions were iced or stored at -20°C prior to transformations. The transformations occurred on ice, where 2 μL of the TOPO subcloning reaction was added to 50 μL of Transform One Shot competent cells (Invitrogen; hereafter termed competent cells). After 30 minutes, the competent cells were heat shocked for 30 seconds at 42°C, and returned to ice for 5 minutes. The competent cells were mixed with 250 μL of SOC medium (2% [w/v] Tryptone, 0.5% [w/v] Yeast Extract, 10 mM NaCl, 2.5 mM KCl, 10 mM MgCl2, 10 mM MgSO4, and 20 mM glucose) and incubated for 1 hour at 37°C in a shaking water bath (200 rpm). Fifty μL of cultured transformants were plated on LB agar with ampicillin (1% [w/v] bacto-tryptone, 0.5% [w/v] bacto-yeast extract, 1% [w/v] NaCl, 1.5% [w/v] agar, and 50 μg/mL ampicillin) and grown overnight at 37°C. Ampicillin was used to select for transformants containing plasmids with inserts. Negative controls included either competent cells alone without plasmids, or with plasmids lacking the addition of inserts. Colony growth was not detected on any of the negative controls.

DNA isolation and PCR of transformant DNA

Individual transformants were subcultured in liquid broth with 50 μg/ mL ampicillin for 24 hours in a shaking water bath at 37°C. The cells were pelleted for 2 minutes at 8,000 x g and DNA isolated using a DNeasy (Qiagen) protocol, according to the manufacturer’s suggestions. DNA was eluted from the column using 100 μl of Buffer AE. The isolated DNA samples were subjected to PCR using M13 forward and reverse primers, whose binding sites are specific to the TOPO cloning vector, rather than to bacterial gene sequences. PCR mixtures of 25 μl contained the following: 1 μl DNA template, 0.5 μM of each primer, 200 μM dNTPs, 2.5 units of Taq DNA Polymerase, 20 mM Tris and 50 mM KCl buffer, and 1.5 mM MgCl. The reaction conditions were 96°C for 5 minutes, 30 cycles at 94°C for 30 seconds, 55°C for 30 seconds, 72°C for 1 minute, with a final extension at 72°C for 10 minutes. Electrophoresis of PCR products (~1.4 kb 16S rRNA gene) was performed on a 1% (w/v) agarose gel in TAE with SYBR-Safe (1:10,000 Invitrogen). Gels were visualized with GelDoc (BioRad) software. Positive controls included transformants with a known ~1.4 kb insert, whereas negative controls lacked template DNA.

Analysis of sequencing results

PCR samples positive for the correctly sized insert of ~ 1.4 kb were cleaned with ExoSAP-IT (GE Healthcare, Piscataway, NJ, USA) prior to sequencing. PCR reactions (6 μl) were mixed with 2 μl ExoSAP-IT, incubated at 37°C and subsequently 80°C, each for 15 minutes. For sequencing, 3 μl of the ExoSAP-IT reaction was combined with 9 μl of PCR water per sample well. This yielded at least 70 ng/ μl of template per well. Primers were arrayed at ~3 pmol/ μl. Samples were shipped overnight at ambient temperature to the DNA Resource Core of Dana-Farber/Harvard Cancer Center; this core was funded in part by an NCI Cancer Center support grant 2P30CA006516-48. Sequencing reactions were performed on an ABI3730xl DNA analyzer. Each sample was sequenced in the forward direction. Ambiguous nucleotides were trimmed by hand in Geneious v.7.1.9 (Biomatters Ltd, Auckland, New Zealand). Chimeras were removed and the sequences were further trimmed upon submission to the National Center for Biotechnology Information (NCBI) Genbank under accession numbers OP050008—OP050060; OP050280—OP050295; OP050295—OP050317; OP047949—OP047976; OP050061—OP050062; OP050318—OP050319. The resulting sequences were used to identify bacteria using the NCBI Basic Local Alignment Search Tool (BLAST) [26]. Sequences were clustered into operational taxonomic units (OTUs) in mothur v.1.40.5 at a 3% cutoff with OptiClust [27], using SILVA (Silva seed v132) as a reference database.

Phylogenetic analysis

To explore relationships among bacterial taxa, we generated two phylogenetic trees: 1) using all 16S sequences generated in this study, and 2) with samples from this study identified as belonging to class Mollicutes combined with representative Mollicutes sequences from the literature [14], the Ribosomal Database Project (RDP) [28], the Silva Database [29], and GenBank. For both analyses, sequences were aligned according to secondary structure using SSU-ALIGN v0.1.1 [30]. Using the program, we masked columns in which nucleotides were assigned with low confidence (S1 Fig). The alignments were used to generate Maximum Likelihood (ML) phylogenies with iQtree version 1.6.6 [31], implementing ModelFinder [32] to determine best-fit substitution models, and ultrafast bootstrap resampling to gauge nodal support [33]. The consensus phylogenies were visualized in FigTree v. 1.4.4 ( and annotated in Adobe Illustrator.

Diversity and statistical analysis

Based on the OTUs, alpha diversity was estimated as richness, evenness, and the Shannon index. A two-sampled t-test assuming unequal variance was used to compare mean values ± standard error, between the scorpion species. Beta diversity was measured using Bray-Curtis similarity and analyzed with permutational multivariate analysis of variance (PERMANOVA) and permutational multivariate analysis of dispersion (PERMDISP) with 2,000 permutations in Primer-E version 6 [34].


The telson contains diverse bacterial taxa

To investigate the microbial diversity of the scorpion venom-producing appendage, the telson, we created 11, 16S rRNA libraries, 1 per telson (S. mesaensis n = 4; H. arizonensis n = 7). From a total of 267 clones, 40% (107 clones) yielded full-length products and were sent for sequencing. Some sequences contained chimeras that were split apart manually, thus yielding 114 sequences that were classified using NCBI Genbank.

BLAST searches of sequenced clones revealed distinct differences between bacterial taxa found in S. mesaensis and H. arizonensis, indicating that each scorpion species has its own unique group of bacteria. Seven and 8 different phyla were detected in S. mesaensis and H. arizonensis, respectively. The most abundant phyla for S. mesaensis were Proteobacteria (44%), Tenericutes (25%) and Firmicutes (16%), whereas the most abundant phyla for H. arizonensis were Firmicutes (40%), Actinobacteria (20%), Bacteroidetes (18%), and Proteobacteria (12%; Fig 2A). Operational taxonomic unit (OTU) analysis showed that most OTUs clustered by host species, with 35 and 11 unique to H. arizonensis and S. mesaensis, respectively. Only 4 of the 50 (8%) OTUs were shared by both species (Fig 2B). The percentage distribution of OTUs showed that a single OTU could be found in 2 to 4 scorpions, representing 2% to 16% of all OTUs, but most OTUs were found in only 1 scorpion (72%) (Fig 2C and 2D). Based on the OTUs, measures of alpha diversity between the scorpion species using the mean Shannon indices were not statistically different (H. arizonensis 1.77 +/- 0.08, S. mesaensis 0.91 +/- 0.20, p = 0.11). Similarly, mean measures of richness (7.71 +/- 0.57, 4.25 +/- 0.83, p = 0.14) and evenness (0.92 +/- 0.02, 0.60 +/- 0.10, p = 0.22) for H. arizonensis and S. mesaensis respectively, showed no significant differences. The ordination plot of beta diversity based on Bray-Curtis similarity (Fig 2E) showed the centroids differed between the scorpion species (pseudo-F = 1.538, df = 10, p = 0.028), but their dispersion did not (F = 0.381, p = 0.651). These data indicate a significant difference in diversity between the microbiota of H. arizonensis and S. mesaensis, but not within the respective species.

Fig 2. Composition of the S. mesaensis and H. arizonensis telson microbiota.

A) Taxonomic assignments at the phylum level for individual samples and the aggregated data (right side) for each species. The Shannon index value for each sample is shown below the graph. B) The OTU distribution by species shows that most OTUs (46 out of 50) were unique to the host species; only 4 OTUs were common to both. C) The percentage distribution of OTUs shows the vast majority of OTUs were found in only one scorpion, and a single OTU was never found in more than four scorpions. D) Heatmap of the relative abundance (%) of each OTU and their assigned genera from BLAST results. The columns represent individual scorpions. The relative abundance is calculated as the percentage of OTU sequences per scorpion. White = 0%; light gray = 10–33%; dark gray = 50–67%; black = 100%. E) Bray-Curtis similarity and PERMANOVA indicate the centroids differ statistically between the microbiota in each scorpion species (pseudo-F = 1.538, p = 0.028, df = 10). Triangles represent individual scorpions; green–H. arizonensis, blue–S. mesaensis. For (A), (D), (E), 1 to 7 are H. arizonensis, A to D are S. mesaensis.

The 16S rRNA sequences from the cloned telson libraries are species-specific

BLAST searches returned identity scores ranging from 86.3% to 100% (S1 Table). Scorpions of the same species shared many common bacterial genera. For example, 50% of S. mesaensis had Escherichia, Sphingomonas or Bacillus, whereas 71% of H. arizonensis had Bacillus and 43% had Staphlococcus (S1 Table). Interestingly, Mollicutes phylotypes were detected in both scorpion species. Mycoplasma was detected in 8 clones from 1 S. mesaensis scorpion whose identities were most like uncultured bacterial clones from the gut tissues of V. smithi and Mesomexovis aff. punctatus [12] and clustered into clade 2 (Fig 3). One H. arizonensis specimen contained 4 clones of Spiroplasma with identities from 88.8 to 95.8% akin to Spiroplasma platyhelix (S1 Table). These Spiroplasma-like sequences grouped into clade 1 (Fig 3).

Fig 3. Phylogenetic tree showing species-specific clades for telson bacteria isolated from S. mesaensis and H. arizonensis.

A Maximum Likelihood phylogeny was constructed based on the DNA sequences of 114 16S rRNA samples isolated from S. mesaensis (n = 32) and H. arizonensis (n = 82) telsons. Scorpion-specific clades are identified by vertical bars numbered 1–12 with samples from H. arizonensis indicated in black; S. mesaensis indicated in red. We considered clades to be scorpion-specific if they contained 3 or more taxa from a single scorpion species and were supported by bootstrap values greater than 70.

The highly structured topology seen in Fig 3 suggests considerable genetic diversity among microbes from scorpion telsons. The tree shows 4 clades of exclusively S. mesaensis and 8 clades exclusively of H. arizonensis samples. Only 5 samples from S. mesaensis nested within H. arizonensis samples. No H. arizonensis samples nested within the S. mesaensis groups. These data indicate that most sequences cluster into clades that are species-specific. Samples with low values for percent identity tend to form long branches, suggesting the presence of unique microbes in these scorpion species (Fig 3).

16S rRNA phylogeny shows sequence contributions to the scorpion Mycoplasma clade and a novel Spiroplasma-like lineage

To determine the relationship between our 16S rRNA Mycoplasma-like and Spiroplasma-like sequences to Mollicutes, we sourced sequences from public databases and the literature (312 in total) to create a phylogenetic tree (Fig 4 and S2 Fig). The Mycoplasma-like sequences from S. mesaensis were grouped as part of the previously designated Scorpion Mycoplasma Clade [12, 14], that includes scorpions from both the Buthidae and Vaejovidae families. Within this clade, the S. mesaensis sequences formed a tightly grouped sister clade with other Vaejovidae family members, being more closely related to sequences from Mesomexovis spp. compared to V. smithi (Fig 4). The node values (100) indicate that these relationships are highly supported. The Spiroplasma-like sequences from H. arizonensis grouped with other Spiroplasma sequences, forming a sister clade with sequences from Spiroplasma platyhelix with high node values (100; Fig 4). These H. arizonensis sequences appear to form a novel lineage that is unrelated to previously reported scorpion sequences.

Fig 4. Phylogenetic tree of Mollicutes 16S rRNA.

The phylogenetic tree was constructed using Maximum Likelihood, including a total of 312 sequences representing Mollicutes taxa. Scorpion sequences are in bold. Red collapsed regions indicate 12 sequences reported in this study from H. arizonensis and S. mesaensis. For an expanded version of this figure see S2 Fig.


Given the importance of the microbiome to the success of several organisms [35], and indirect evidence suggesting the presence of bacteria associated with the scorpion venom and venom organ [1821], we tested whether the venom organ of H. arizonensis and S. mesaensis harbored bacteria. To the best of our knowledge, we have provided the first evidence of the broad bacterial diversity in the telsons of H. arizonensis and S. mesaensis. Interestingly, each scorpion species has its own set of telson bacteria (Fig 2) that group by host species in phylogenetic analyses (Figs 3 and 4). Sequences from S. mesaensis added another Vaejovidae family member to the previously reported Scorpion Mycoplasma Clade and a novel lineage of Spiroplasma-like sequences was found in H. arizonensis (Fig 4). Our study contributes to the emerging field of venom-microbiomics that seeks to integrate the areas of venomics with microbiology [16].

In this study we housed the scorpions in individual containers prior to tissue isolation to reduce the chance of cross contamination between animals and isolated the telson/venom gland samples under sterile conditions with a dissecting microscope. Despite our best efforts to mitigate potential sources of contamination, we cannot rule out that regions beyond the venom gland itself, like the hemolymph or exoskeleton, may have contributed microbiota.

Previous research has shown that the scorpion gut microbiome is largely species-specific [12, 14]. Similarly, our data indicate distinct telson microbiomes in S. mesaensis compared to H. arizonensis (Figs 24). At the phylum level, we found each scorpion species to have its own set of bacteria (Fig 2). Given that Proteobacteria make up the largest bacterial phylum, it is not surprising that these Gram-negative bacteria were predominant in S. mesaensis (Fig 2). A predominance of Proteobacteria is consistent with previous studies in V. smithi and C. limpidus [12], but contrary to the findings in A. australis, where 95% of the clones from gut and gonad tissues were Mollicutes [13]. Unlike S. mesaensis, Proteobacteria were limited in abundance in H. arizonensis, where Firmicutes dominated (Fig 2). Only 8% of OTUs were shared between the species and the Bray-Curtis similarity showed that the centroids but not the dispersion were significantly different (Fig 2), providing additional and statistical evidence for specificity of the microbiomes by species.

Our phylogenetic tree from the cloned libraries showed that the sequences separate into 12 scorpion-specific clades, with 4 clades from S. mesaensis and 8 clades from H. arizonensis (Fig 3). Of the 114 sequences analyzed, 5 S. mesaensis sequences were nested within H. arizonensis samples; none of H. arizonensis samples nested within groups of S. mesaensis sequences. Albeit the prevailing trend showed clustering of the bacterial 16S rRNA sequences, according to their host species.

As aforementioned, the 114 bacterial clones isolated from scorpion telsons represented a broad range of taxa including some which are related to Mycoplasma and Spiroplasma. Mycoplasma and Spiroplasma are from the Mollicutes class of bacteria, and their effects on hosts range from pathogenic, to commensal, to beneficial [35]. Mollicutes hallmarks are a lack of a cell wall and extremely small size, often having widths of less than 0.2 μm. They can reside on the outer surface of cells, inside of cells or extracellularly. Spiroplasma are typically found in plants and arthropods, as are Mycoplasma, that are additionally found in vertebrate animals. Mycoplasma and Spiroplasma were of particular interest since in other scorpion species, these genera formed novel lineages that were related to gut microbiota [12, 14], and Mollicutes phylotypes were predominant in the tissues of A. australis [13]. For S. mesaensis, from a single scorpion we retrieved 8 Mycoplasma-like clones that formed clade 2 (Fig 3). Sequences from this clade showed close identity with sequences from various scorpion species including for example, V. smithi (94%; KM978265.2), M. aff. punctatus (97%; MF134711 and MF134712), C. limpidus (91%; KM978292.1) [14], and A. australis (91%; KT880638.1) [13]. Mycoplasma had previously been detected in 2 scorpion families, Vaejovidae and Buthidae [1214], forming a novel clade termed the Scorpion Mycoplasma Clade, with separate branches for each family [12, 14]. Our results provide an additional Vaejovidae family member to this small albeit ever-expanding Scorpion Mycoplasma Clade, S. mesaensis, that is most closely related to Mycoplasma found in Mesomexovis species (Fig 4). This result provides additional evidence of cospeciation between scorpions and Scorpion Mycoplasma Clade symbionts, as previously proposed [14]. Mycoplasma has not yet been detected in scorpions beyond these 2 families.

From a single H. arizonensis scorpion we detected 4 sequences most closely related to Spiroplasma platyhelix (Fig 3 and S1 Table) [36]. The ML analysis grouped all 4 sequences into a single clade that included Spiroplasma platyhelix, and formed a sister clade with Spiroplasma sequences from other arthropods, including beetles and ticks (Fig 4 and S2 Fig) [37, 38]. Node values (100) highly support this topology.

The detection of Spiroplasma in discrete scorpion families and species is increasing. Including this study, endogenous Spiroplasma sequences have been detected in 3 scorpion families and 8 species as follows: 1. Hadruridae—H. arizonensis (this study); 2. Vaejovidae–V. smithi, Vaejovis granulatus, M. aff. punctatus, Mesomexovis aff. oaxaca, Mesomexovis aff. variegatus; 3. Buthidae–C. limpidus, A. australis. [1214]. Not included in this tally are Spiroplasma sequences from D. duende and A. australis, that were likely derived from endosymbionts of insect prey, rather than forming part of the endogenous microbiome of the scorpions themselves [13, 14].

Spiroplasma-like sequences of the Vaejovidae family includes the novel lineage termed Scorpion Group 1 (SG1) which are thus far restricted to this family alone [12, 14]. Our phylogenetic analysis indicates that SG1 represents a distinct lineage with low haplotype diversity that is most closely related to sequences from the mollusk Leptochiton boucheti (Fig 4). This latter prediction has strong node support (bootstrap (bs) = 97) and differs from previous reports [12, 14], likely due to differing analytical methods. Spiroplasma taxa from the Buthidae family are divergent, with the A. australis sequences grouped into a clade combined with several other Spiroplasma species, whereas OTU4 from C. limpidus formed a sister clade with samples from a vinegaroon, Mastigoproctus sp., as it did previously [14]. The predicted phylogenetic relationship between C. limpidus and Mastigoproctus is strongly supported (bs = 99). The Spiroplasma detected in H. arizonensis are divergent from the sequences of OTU4 (85% identity), SG1 (76–77% identity or unrelated) and A. australis (84–86% identity), and thus form a novel scorpion lineage (Fig 4).

Although our sequence data from S. mesaensis and H. arizonensis provide great insights into telson microbiomes, the actual bacterial diversity is likely to be much greater. TOPO cloning allowed us to accurately identify several bacterial phylotypes, but high throughput sequencing methods would provide a more detailed data set. Additionally, our analyses are constrained by the quality and number of sequences in the reference database and we acknowledge that the 16S rRNA gene sequence alone is not sufficient to assign all taxa to species. Notwithstanding the limitations, our survey is the first to report bacteria in the telsons of H. arizonenesis (the first hadrurid) and S. mesaensis, complementing the detection of telson bacteria in A. australis [13] and H. lepturus [9]. Further, our results indicate that different scorpion species contain unique suites of microbes (Figs 2 and 3).

While the gut microbiome can be influenced by several factors including genetics, environment, and diet [12, 14, 39], which of these factors can alter the telson microbiome is unknown. Horizontal acquisition of bacterial symbionts is not likely since, for example, the sequences we isolated are not closely related to insect endosymbionts (S1 Table). However, there is evidence supporting the vertical transmission of bacterial symbionts in scorpions. Previous studies showed that in 2 species, M. aff. punctatus and Centruroides noxius, scorpion embryos and their mothers’ gut had identical Mollicutes bacterial symbionts [14], and bacteria have been detected in the gonads of A. australis [13]. Further, evidence suggests a coevolution between scorpion species and their Mycoplasma and Spiroplasma symbionts, SMC and SG1 taxa, dating back to a common ancestor from more than 120 million years ago [14]. More research is needed within and between scorpion species and scorpion families to determine the association of their bacterial symbionts.

What function might the telson microbiome provide? Bacteria in some organisms, like antlion larvae or pufferfish, function to produce or increase the toxicity of the venom, making the venom more effective [40, 41]. This would increase the chances of successful defense and prey capture. It may be that the telson microbiome also plays a role in the biochemistry and toxicity of the scorpion venom. An additional explanation is that the telson bacteria protect the scorpion from other microorganisms. For example, the genome of “Candidatus” Spiroplasma holothuricola, isolated from sea cucumbers in a deep-sea ecosystem, contained genes from the clustered regularly interspaced short palindromic repeats (CRISPR) /Cas system and toxins for defending against microbes [42]. Further, antimicrobial peptides may provide innate immunity. Several studies have detected antimicrobial peptides in scorpion venom, where they are assumed to be produced by the scorpion [43]. However, based on our results we propose that some of the antimicrobial peptides may be produced by the telson bacteria. One would expect that since the scorpion telson contains bacteria, the venom should also contain bacteria. Indeed, bacteria have been successfully isolated from the venom of snakes and spiders [23], even though venom extraction and analysis can be challenging. For example, Esmaeilishirazifard et al., 2018 [22], attempted to culture bacteria from scorpion venoms, including H. arizonensis studied here, but no bacterial growth was reported, due to sampling limitations that included scorpion availability and low volumes (<1 to 30 ul) of venom. Despite these challenges it would be interesting to re-explore scorpion venom for bacteria in the future.


Here we provide the first molecular evidence of bacteria in the telsons of the scorpion species S. mesaensis and H. arizonensis and reveal unique microbiomes, including novel bacterial lineages, from the 2 species tested. Given the emerging importance of the microbiome for health and well-being in numerous organisms, it is not surprising that an ancient appendage involved in food acquisition and defense, has its own microbiome. Although the precise function of the telson microbiome is unknown, our findings may change how we view the biology of scorpions, their venoms, and the microscopic life that lives within them.

Supporting information

S1 Fig. Secondary structure of 16S rRNA showing sites that were included and excluded (masked) in phylogenetic analysis of Mollicutes phylotypes.

The figure was created with the SSU-ALIGN package ( which derived the structure diagram from the CRW database (


S2 Fig. Expanded phylogenetic tree of Mollicutes 16S rRNA.


S1 Table. Identification using DNA sequencing of the bacteria isolated from scorpions, their percent identity as indicated by BLAST, clade organization, and OTU assignment.



We thank G. Graham and P. Cushing for assistance in the field, and W.B. Mattingly for help with diversity measures and statistical analysis. Specimens from California were collected by MRG under a scientific collecting permit from the California Department of Fish and Wildlife to the U.S. Geological Survey (SCP838). We thank the Biology Department, Eastern Connecticut State University, for their continued support of undergraduate research.


  1. 1. Polis GA. The biology of scorpions. Stanford, CA: Stanford University Press 1990.
  2. 2. Adcock GJ, Dennis ES, Easteal S, Huttley GA, Jermiin LS, Peacock WJ, et al. Mitochondrial DNA sequences in ancient Australians: Implications for modern human origins. Proc Natl Acad Sci U S A. 2001;98(2):537–42. pmid:11209053.
  3. 3. Cho I, Blaser MJ. The human microbiome: At the interface of health and disease. Nat Rev Genet. 2012;13(4):260–70. pmid:22411464.
  4. 4. Singh RK, Chang HW, Yan D, Lee KM, Ucmak D, Wong K, et al. Influence of diet on the gut microbiome and implications for human health. Journal of Translational Medicine. 2017;15. pmid:28388917.
  5. 5. Turnbaugh PJ, Ridaura VK, Faith JJ, Rey FE, Knight R, Gordon JI. The effect of diet on the human gut microbiome: A metagenomic analysis in humanized gnotobiotic mice. Science translational medicine. 2009;1(6):6ra14. pmid:20368178.
  6. 6. Bouchon D, Zimmer M, Dittmer J. The terrestrial isopod microbiome: An all-in-one toolbox for animal-microbe interactions of ecological relevance. Front Microbiol. 2016;7:1472. Epub 20160923. pmid:27721806.
  7. 7. Cannicci S, Fratini S, Meriggi N, Bacci G, Iannucci A, Mengoni A, et al. To the land and beyond: Crab microbiomes as a paradigm for the evolution of terrestrialization. Front Microbiol. 2020;11:575372. Epub 20201007. pmid:33117320.
  8. 8. Suesdek-Rocha L, Bertani R, da Silva P, Selivon D. The first record for Wolbachia in a scorpion: The parthenogenetic yellow scorpion Tityus serrulatus (Scorpiones, Buthidae). Revista Iberica de Arachnologia. 2006;14:183–4.
  9. 9. Baradaran M, Jalali A, Jolodar A. Molecular diagnosis of Wolbachia endosymbiont from Iranian scorpion Hemiscorpius lepturus using polymerase chain reaction (PCR) amplification of 16 S rDNA gene. Afr J Biotechnol. 2011;10(85):19802–806.
  10. 10. Baldo L, Prendini L, Corthals A, Werren JH. Wolbachia are present in Southern African scorpions and cluster with supergroup F. Curr Microbiol. 2007;55(5):367–73. Epub 20070805. pmid:17676427.
  11. 11. Bryson RW Jr. Bacterial endosymbiont infections in ’living fossils’: A case study of North American vaejovid scorpions. Mol Ecol Resour. 2014;14(4):789–93. pmid:24373187.
  12. 12. Bolanos LM, Rosenblueth M, Castillo-Ramirez S, Figuier-Huttin G, Martinez-Romero E. Species-specific diversity of novel bacterial lineages and differential abundance of predicted pathways for toxic compound degradation in scorpion gut microbiota. Environmental microbiology. 2016;18(5):1364–78. Epub 2015/06/11. pmid:26058415.
  13. 13. Elmnasri K, Hamdi C, Ettoumi B, Crotti E, Guesmi A, Najjari A, et al. Highly divergent Mollicutes symbionts coexist in the scorpion Androctonus australis. J Basic Microbiol. 2018;58(10):827–35. Epub 20180718. pmid:30019339.
  14. 14. Bolanos LM, Rosenblueth M, Manrique de Lara A, Migueles-Lozano A, Gil-Aguillon C, Mateo-Estrada V, et al. Cophylogenetic analysis suggests cospeciation between the Scorpion Mycoplasma Clade symbionts and their hosts. PLoS One. 2019;14(1):e0209588. Epub 20190109. pmid:30625167.
  15. 15. Oliveira AL, Viegas MF, da Silva SL, Soares AM, Ramos MJ, Fernandes PA. The chemistry of snake venom and its medicinal potential. Nature Reviews Chemistry. 2022;6(7):451–69. pmid:35702592
  16. 16. Ul-Hasan S, Rodriguez-Roman E, Reitzel AM, Adams RMM, Herzig V, Nobile CJ, et al. The emerging field of venom-microbiomics for exploring venom as a microenvironment, and the corresponding Initiative for Venom Associated Microbes and Parasites (iVAMP). Toxicon X. 2019;4:100016. Epub 20190920. pmid:32550573.
  17. 17. Alavi SM, Azarkish A. Secondary bacterial infection among the patients with scorpion sting in Razi hospital, Ahvaz, Iran. Jundishapur J Microbiol. 2011;4(1):37–42.
  18. 18. Cao L, Dai C, Li Z, Fan Z, Song Y, Wu Y, et al. Antibacterial activity and mechanism of a scorpion venom peptide derivative in vitro and in vivo. PLoS One. 2012;7(7):e40135. Epub 2012/07/14. pmid:22792229.
  19. 19. Liu G, Yang F, Li F, Li Z, Lang Y, Shen B, et al. Therapeutic potential of a scorpion venom-derived antimicrobial peptide and its homologs against antibiotic-resistant Gram-positive bacteria. Front Microbiol. 2018;9:1159. Epub 2018/06/14. pmid:29896190.
  20. 20. Perumal Samy R, Stiles BG, Franco OL, Sethi G, Lim LHK. Animal venoms as antimicrobial agents. Biochem Pharmacol. 2017;134:127–38. Epub 2017/03/16. pmid:28288817.
  21. 21. Wang X, Wang G. Insights into antimicrobial peptides from spiders and scorpions. Protein Pept Lett. 2016;23(8):707–21. Epub 2016/05/12. pmid:27165405.
  22. 22. Esmaeilishirazifard E, Usher L, Trim C, Denise H, Sangal V, Tyson GH, et al. Microbial adaptation to venom is common in snakes and spiders. bioRxiv. 2018:348433.
  23. 23. Esmaeilishirazifard E, Usher L, Trim C, Denise H, Sangal V, Tyson GH, et al. Bacterial adaptation to venom in snakes and arachnida. Microbiol Spectr. 2022;10(3):e0240821. Epub 20220523. pmid:35604233.
  24. 24. Santibáñez-López CE, Ojanguren-Affilastro AA, Sharma PP. Another one bites the dust: Taxonomic sampling of a key genus in phylogenomic datasets reveals more non-monophyletic groups in traditional scorpion classification. Invertebrate Systematics. 2020;34(2):133–43.
  25. 25. Marchesi JR, Sato T, Weightman AJ, Martin TA, Fry JC, Hiom SJ, et al. Design and evaluation of useful bacterium-specific PCR primers that amplify genes coding for bacterial 16S rRNA. Appl Environ Microbiol. 1998;64(2):795–9. pmid:9464425.
  26. 26. Altschul SF, Gish W, Miller W, Myers EW, Lipman DJ. Basic local alignment search tool. J Mol Biol. 1990;215(3):403–10. pmid:2231712.
  27. 27. Westcott SL, Schloss PD. OptiClust, an improved method for assigning amplicon-based sequence data to operational taxonomic units. mSphere. 2017;2(2). Epub 20170308. pmid:28289728.
  28. 28. Cole JR, Chai B, Marsh TL, Farris RJ, Wang Q, Kulam SA, et al. The Ribosomal Database Project (RDP-II): Previewing a new autoaligner that allows regular updates and the new prokaryotic taxonomy. Nucleic Acids Res. 2003;31(1):442–3. pmid:12520046.
  29. 29. 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(Database issue):D590–6. Epub 20121128. pmid:23193283.
  30. 30. Nawrocki E. Structural RNA homology search and alignment using covariance models. Washington University in St. Louis; 2009.
  31. 31. Nguyen LT, Schmidt HA, von Haeseler A, Minh BQ. IQ-TREE: A fast and effective stochastic algorithm for estimating maximum-likelihood phylogenies. Mol Biol Evol. 2015;32(1):268–74. Epub 20141103. pmid:25371430.
  32. 32. Kalyaanamoorthy S, Minh BQ, Wong TKF, von Haeseler A, Jermiin LS. ModelFinder: Fast model selection for accurate phylogenetic estimates. Nat Methods. 2017;14(6):587–9. Epub 20170508. pmid:28481363.
  33. 33. Minh BQ, Nguyen MA, von Haeseler A. Ultrafast approximation for phylogenetic bootstrap. Mol Biol Evol. 2013;30(5):1188–95. Epub 20130215. pmid:23418397.
  34. 34. Anderson M, Gorley R, Clarke KP. PRIMER: Guide to Software and Statistical Methods. PRIMER-E, Plymouth, UK. 2008.
  35. 35. Regassa LB, Gasparich GE. Spiroplasmas: Evolutionary relationships and biodiversity. Front Biosci. 2006;11:2983–3002. Epub 20060901. pmid:16720370.
  36. 36. Williamson DL, Adams JR, Whitcomb RF, Tully JG, Carle P, Konai M, et al. Spiroplasma platyhelix sp. nov., a new mollicute with unusual morphology and genome size from the dragonfly Pachydiplax longipennis. Int J Syst Bacteriol. 1997;47(3):763–6. pmid:9226909.
  37. 37. Tinsley MC, Majerus ME. A new male-killing parasitism: Spiroplasma bacteria infect the ladybird beetle Anisosticta novemdecimpunctata (Coleoptera: Coccinellidae). Parasitology. 2006;132(Pt 6):757–65. Epub 20060203. pmid:16454865.
  38. 38. Tully JG, Rose DL, Yunker CE, Carle P, Bove JM, Williamson DL, et al. Spiroplasma ixodetis sp. nov., a new species from Ixodes pacificus ticks collected in Oregon. Int J Syst Bacteriol. 1995;45(1):23–8. pmid:7857803.
  39. 39. Bletz MC, Goedbloed DJ, Sanchez E, Reinhardt T, Tebbe CC, Bhuju S, et al. Amphibian gut microbiota shifts differentially in community structure but converges on habitat-specific predicted functions. Nat Commun. 2016;7:13699. Epub 20161215. pmid:27976718.
  40. 40. Campbell S, Harada RM, DeFelice SV, Bienfang PK, Li QX. Bacterial production of tetrodotoxin in the pufferfish Arothron hispidus. Nat Prod Res. 2009;23(17):1630–40. pmid:19851930.
  41. 41. Yoshida N, Oeda K, Watanabe E, Mikami T, Fukita Y, Nishimura K, et al. Protein function. Chaperonin turned insect toxin. Nature. 2001;411(6833):44. pmid:11333970.
  42. 42. He LS, Zhang PW, Huang JM, Zhu FC, Danchin A, Wang Y. The enigmatic genome of an obligate ancient Spiroplasma symbiont in a hadal holothurian. Appl Environ Microbiol. 2018;84(1). Epub 20171215. pmid:29054873.
  43. 43. Harrison PL, Abdel-Rahman MA, Miller K, Strong PN. Antimicrobial peptides from scorpion venoms. Toxicon. 2014;88:115–37. Epub 20140619. pmid:24951876.