Phylogeny and clitellar morphology of the giant Amazonian earthworm, Rhinodrilus priollii (oligochaeta: glossoscolecidae).
|Abstract:||The giant earthworm, Rhinodrilus priollii Righi 1967, is among the largest terrestrial invertebrates known worldwide, reaching lengths >2 m. To investigate the evolutionary history, of the species and aspects of their reproductive biology, we collected R. priollii specimens from several field sites in central Amazonia. Phylogenetic analyses of 16 individuals using a fragment of cytochrome c oxidase subunit 1 (CO1) identified seven haplotypes that diverged between 2-8%. Population structures indicate episodes of gene flow between populations and their divergence within the past 1-2 million years. Histological examination of clitella from sexually mature specimens identified cocoon secretory cells throughout the dorsal and dorsoventral epidermis. Unlike previously described secretory cells, those in R. priollii contained granules with a proteinaceous core covered by external glycosylation. Further, collagenous matrices formed the bulk of swollen clitella while albumin-secreting cells were noticeably absent, collectively suggesting a mechanism of cocoon production somewhat different from that described in other clitellate megadriles.|
Morphology (Animals) (Research)
Earthworms (Physiological aspects)
Earthworms (Genetic aspects)
Animal genetics (Research)
Lang, Shirley A.
Garcia, Marcos V.
James, Samuel W.
Sayers, Charlene W.
Shain, Daniel H.
|Publication:||Name: The American Midland Naturalist Publisher: University of Notre Dame, Department of Biological Sciences Audience: Academic Format: Magazine/Journal Subject: Biological sciences; Earth sciences Copyright: COPYRIGHT 2012 University of Notre Dame, Department of Biological Sciences ISSN: 0003-0031|
|Issue:||Date: April, 2012 Source Volume: 167 Source Issue: 2|
|Topic:||Event Code: 310 Science & research|
|Geographic:||Geographic Scope: United States Geographic Code: 1USA United States|
Among ~6000 species of formally recognized terrestrial megadriles (Blakemore, 2009), relatively few (~20) attain adult lengths exceeding 1 m. These atypically large earthworms remain a scientific curiosity in terms of their ecology, physiology, behavior, and evolution. Indeed, their large size poses challenges related to nutritional requirements, oxygen transport, predation, burrowing, reproduction, and cocoon construction. Nevertheless, giant earthworms have successfully and independently colonized a variety of habitats worldwide. Examples include the Giant Gippsland Earthworm, Megascolides australis McCoy 1878 of southern Australia (up to ~2 m; Van Praagh, 1992), Megascolex mekongianus Cognetti 1922 from Vietnam (up to 2.9 m; Blakemore et al., 2005), Microchaetus microchaetus Rapp 1849 from South Africa (up to 1.8 m; Plisko, 1999), Tonoscolex birmanicus Gates 1926 from Burma (up to ~3 m in some reports; Gates, 1972), Glossoscolex giganteus Leuckart 1835/6 from South America (up to ~2.7 m; Beddard, 1895), Celeriella gigantean Benham 1906 from New Zealand (up to 1.4 m; Lee, 1959), Driloleirus americanus Smith 1897 from Washington State, North America (up to 1 m; in Blakemore et al., 2005), and several Rhinodrilus species from South America, including the subject of this study, Rhinodrilus priollii Righi 1967.
More than 20 species of Rhinodrilus (family Glossoscolecidae) have been described, many of which are native to South America (James and Brown, 2006). One of the largest species in the genus, R. priollii, appears to be endemic to the Amazon Basin, but otherwise its geographic range and other aspects of its biology remain mostly unexplored. In this report, we present baseline data on the biogeography of R. priollii in central Amazonia, and examine cellular and morphological aspects of its atypically large clitellum.
MATERIALS AND METHODS
Rhinodrilus priollii Righi 1967 specimens were collected between Sep.-Dec. 2008, from field sites near Manaus, Brazil. Worms were maintained in 500-1000 L fiberglass storage vessels, containing 2-3 cm of ground soil and forest litter from the collection site. Containers were kept moist with occasional water sprinkling, covered, and placed in a shady area (e.g., under forest canopy). Under such conditions, specimens survived up to several months at low densities (e.g., 2-5 worms per container); higher densities significantly reduced survival time.
Specimens were fixed in the field with 10% formalin for 1-3 d, then transferred to 70% EtOH for long-term storage. Following an ascending EtOH series to xylene, worm fragments were embedded in Paraplast X-tra (McCormick Scientific) and sectioned at 5-7 [micro]m on a Spencer "820" microtome. Sections were stained with Masson's trichrome according to Sheehan and Hrapchak (1980). Images were captured on a Canon Rebel XT coupled to a Zeiss Universal with a PI 232 mm 28 adaptor (Perspective Image LLC, Beaverton, OR).
DNA EXTRACTION AND AMPLIFICATION
Tissue samples (~30 mg of muscle scraped from inside the cuticle) from postmortem specimens (fixed in 70% EtOH only) were removed with a scalpel, and genomic DNA was extracted using an E.Z.N.A. Tissue Isolation Kit (Omega Bio-Tek). Mitochondrial cytochrome c oxidase subunit 1 (CO1) was amplified from genomic DNA using universal primers LCO and HCO as described (Folmer et al., 1994), amplifying a ~600 bp fragment.
DNA SEQUENCING AND EDITING
PCR products were excised from 1% agarose gels and prepared for sequencing using GeneClean (MP Biomedicals, LLC). DNA sequencing was conducted by GeneWiz Inc. (South Plainfield, New Jersey) with forward and reverse PCR primers. Sequences were viewed and manually adjusted in ChromasPro (Technelysium, Queensland, Australia), and aligned with CLUSTALW (Thompson et al., 1994) to determine overlapping regions suitable for phylogenetic analyses. GenBank accession numbers for new COI sequences are listed in corresponding Figure legends.
Maximum-likelihood (ML) analyses were performed for all DNA comparisons, using the pipeline sequence MUSCLE (Edgar, 2004) to align corresponding sequences from multiple individuals or homologous DNA across species, Gblocks (Castresana, 2000) for alignment curation, PhyML (Guindon and Gascuel, 2003) for tree building and TreeDyn (Chevenet et al., 2006) for tree drawing, as configured in the Phylogeny.fr platform (Dereeper et al., 2008). The aLRT statistical test (approximation of the standard Likelihood Ratio Test; Anisimova and Grascuel, 2006) embedded in PhyML determined branch support values. Default settings were used for all parameters.
[FIGURE 1 OMITTED]
Specimens of Rhinodrilus (Fig. 1) were collected from four geographic locations proximal to Manaus, Brazil: Universidade Federal do Amazonas (UFAM) experimental farm (02[degrees]38'44.35"S, 60[degrees]02'44.20"W), Instituto Nacional de Pesquisas Amazonia (INPA) field station (02[degrees]37'32.94"S, 60[degrees]02'38.72"W), RPPN field site near Encontro das Aguas (03'06.882S, 59'W 54.291'W), and a private farm (02[degrees]54'33"S, 59[degrees]56'34"W)--all below elevation 100 m (Fig. 2). In total, ~50 specimens were collected, most of which (~30) were from the UFAM experimental farm. Worms were generally not observed during daylight hours except during persistent heavy rains, upon which they surfaced at densities up to ~100 per [km.sup.2]. Under such conditions, they moved actively atop the forest litter for the duration of rainfall and several hours thereafter, leaving characteristic linear trails in soft sediment (e.g., dirt roads). Occasionally, worms were observed being carried passively in transient runoff streams during particularly heavy rainfall. Worms also surfaced during the evening based on remnant tracks, even in the absence of rainfall (though track numbers were much fewer under dry conditions). Specimens ranging in length between 1-2 m in an extended position were common in undisturbed areas (e.g., primary growth forest); developed areas, including nature reserves within urban areas, appeared to lack any significant numbers of R. priollii individuals. The largest specimens were collected at the UFAM field size, reaching lengths over 2 m (up to ~220 cm when extended).
Gene fragments from CO1 were successfully amplified from 16 Rhinodnlus priollii individuals representing seven haplotypes (Table 1); seven specimens collected from the PM field site identified two haplotypes that were likely Rhinodrilus contortus Cernosvitov 1938, based on geographic and morphological criteria.
Comparisons of representative CO1 sequences indicated that haplotypes occurred within and between populations (Fig. 3). The two major Rhinodrilus priollii haplotype lineages were 7-8% divergent in the CO1 locus, and contained representatives from multiple populations suggesting recent episodes of gene flow. Two R. contortus haplotypes formed a third clade ~18% divergent from R. priollii CO1 sequences.
The clitellum of Rhinodrilus priollii specimens was pronounced in mature individuals (up to ~3 cm in diameter), forming a saddle-like structure around the dorso-lateral aspect of the worm. Histological sections through clitella in mature individuals revealed thick, collagenous layers (2-3 mm) separating outer, circular muscle fibers and the epidermis (Fig. 4). Collagen appeared to be supported by a proteinaceous scaffolding (Fig. 5A), and was absent in comparable body wall sections or clitella from immature individuals (Fig. 5B). Thicker regions of the clitellum (i.e., more dorsal) contained two collagenous layers demarcated by a relatively thin, proteinaceous boundary (Fig. 6).
Granulated secretory cells were observed throughout the dorsal and dorso-lateral epidermis, along the length of the clitellum. Cell bodies were typically anchored in the outer collagenous layer, extending elaborate tubules to the epidermal surface (Fig. 7A). Granules were packed within the cell body and tubules, often displaying an azocarmine-staining core (red) surrounded by an alcian blue-staining surface (blue; Fig. 7B).
Our behavioral observations of Rhinodrilus priollii Righi 1967 are consistent with other megadrile species, in that worms were more active during evening hours, and surface during heavy rainfall. The cause of surfacing during rainfall has been debated, and may be related to increased carbon dioxide levels, burrow flooding and/or mating behavior (Edwards, 2004). That no R. priollii specimens were observed at peak daylight hours suggests they are efficient burrowers, even in the relatively hard, root-dense soil typical of central Amazonia.
[FIGURE 2 OMITTED]
Once might reasonably assume that the climatic regime and nutrient-poor soil characteristic of equatorial Amazonia would not be suitable for a large, burrowing annelid. However, the large size of individuals (300-400 g) likely acts as a thermal mass that prolongs survival in exposed areas; for example, relatively small specimens of Rhinodrilus priollii and other worm species were often found desiccated on dirt roads, while large specimens were not. More importantly perhaps is that lack of soil nutrients may necessitate ingestion and processing of large soil quantities to meet nutritional requirements. Indeed, dissected specimens were filled with soil debris, though gut: body ratios appear comparable to common earthworms, (e.g., Lumbricus terrestris. Eisenia fetida). Gigantism in worms may, in principle, represent an evolutionary, advantage in nutrient-deficient soils by permitting enhanced nutrient absorption due to a longer gut, but experimental support for this notion is lacking (see below).
In addition to their unusual length, a striking morphological feature of mature Rhinodrilus priollii specimens is their saddle-like clitellum which can measure up to ~3 cm in diameter, almost twice the diameter of a typical midbody segment. Histological sections revealed the underlying source of this biomass, namely collagenous layers that separated outer muscle layers from the epidermis. These collagenous matrices are likely transient structures associated with reproduction, based on their absence in clitella of immature specimens or midbody segments. Note that comparable collagenous material has not been described in other earthworm clitella; rather, elongated albumen-secreting cells appear in a similar position and are major contributors to clitellum swelling (Grove, 1925; Lufty, 1965). Possibly, R. priollii specimens examined in this study had recently secreted cocoons thus explaining the absence of albumen-secreting cells, though the abundance of granulated Type II/III-like cells throughout the clitellar epidermis does not support this hypothesis (Grove and Cowley, 1927; Sayers et al., 2009). Alternatively, albumenotrophic glands may be positioned elsewhere in the reproductive system (e.g., prostates; Omodeo, 2000). A detailed examination of secreted R. priollii cocoons and reproductive structures may reveal the basis of this apparent morphological difference.
[FIGURE 3 OMITTED]
[FIGURE 4 OMITTED]
[FIGURE 5 OMITTED]
In principle, collagenous layers observed in the Rhinodrilus priollii clitellum may have dual functions. First, the volumetric expansion of the clitellum leads to a linear increase in epidermal surface area, thus providing additional physical space for cocoon secretory glands. Secondly, the diameter of the secreted cocoon sheath will consequently be larger than the body, thus facilitating cocoon deposition via its characteristic sliding over smaller, anterior segments to remove the cocoon sheath (see Stephenson, 1930; Coleman and Shain, 2009).
Secretory glands observed in peripheral regions of the collagenous layer and epidermis were morphologically similar to Type II/III cells reported previously in the leech, Theromyzon tessulatum (Sayers et al., 2009). In contrast to those cells, however, Rhinodrilus priollii glands displayed granules that stained with both alcian-blue (outer granule) and azocarmine (inner granule) in Masson's stain, suggesting a proteinaceous core surrounded by a glycosylated external layer. In T. tessulatum, Type II cells (glycosylated) and Type III cells (proteinaceous) give rise to opercula and cocoon membrane structures, respectively (Sayers et al., 2009). Thus, the apparent fusion of Type II and Type III granules observed in R. priollii suggests a different mechanism of cocoon construction that will require further investigation. Note that histological staining of comparable cells in other species using hematoxylin and eosin (H&E) and other stains did not resolve the morphologically indistinguishable Type II and Type III cells (blue and red in Masson's stain, respectively; Sayers et al., 2009), and thus meaningful comparisons are difficult to make between R. priollii and cocoon secretory cells reported in older literature (e.g., Grove and Cowley, 1927; Defretin and Demailly, 1953; Lufty, 1965; Fleming and Baron, 1982).
[FIGURE 6 OMITTED]
Using CO1 molecular clock variance values (e.g., Knowlton et al., 1993; Chang et al., 2008), the relative depth of Rhinodrilus priollii populations based on CO1 haplotype divergence (~8%) suggests they have occupied the Amazon Basin over the past 1-2 million years. Rhinodrilus priollii individuals are capable of moving considerable distances based on deep structures detected within populations (see Fig. 3). Active dispersal by crawling is the most obvious mechanism by which R. priollii populations have expanded, but passive dispersal by transient run-off streams (as observed in this study), and possibly in seasonal or permanent waterways, cannot be excluded as an important dispersal mechanism. Taken together, the current geographic range of R. priollii is likely to extend well beyond the area surveyed here, and additional sampling may reveal an ancestry considerably older than what has been determined here.
[FIGURE 7 OMITTED]
Giant earthworms have arisen independently and on multiple occasions, based on their higher-ranked taxonomic positions (e.g., Moniligasteridae, Microchaetidae, Glossoscolecidae, Megascolecidae; Blakemore et al., 2005). Further, they inhabit various environments, climatic regimes and geographic regions (e.g., Australia; Vietnam; South Africa, North America, South America, etc.), leaving open the question as to what underlying mechanism(s) or environmental factor(s), if any, lead to gigantism. In other animals (e.g., insects, mammals), gigantism has been explained as a consequence of elevated growth hormone levels (Nijhout, 1998; Maheshwari et al., 2000), a phenotype that is relatively rare within Animalia. By analogy, stochastic variation in growth hormone levels across the Clitellata as a consequence of random genetic variance may explain the occasional and punctuated (Eldredge and Gould, 1972) appearance of giant earthworm species in a variety of habitats worldwide.
Acknowledgments.--Supported by a Fullbright scholarship and NSF grant IBN-0417081000 to DHS.
ANISIMOVA, M. AND O. GASCUEL. 2006. Approximate likelihood ratio test for branches: a fast, accurate and powerful alternative. Syst. Biol., 55:539-552.
BEDDARD, F. E. 1895. A monograph of the order Oligochaeta. Clarendon Press, Oxford. 770 p.
BLAKEMORE, R.J., C. S. CSUZD1, M. T. ITO, N. KANEKO, M. G. PAOLETTI, S. E. SPIRIDONOV, T. UCHIDA AND B. D. VAN PRAAGH. 2005. Megascolex (Promegascolex mekongianus Cognetti, 1922--its extent, ecology and allocation to Amynthas (Clitellata/Oligochaeta: Megascolecidae). Opusc. Zool. Budapest, 36:19-30.
--. 2009. Cosmopolitan earthworms--a gobal and historical perspective, p. 257-283. In: D. H. Shain (ed.). Annelids in Modern Biology. John Wiley & Sons, Inc., Hoboken, New Jersey, USA.
CASTRESANA, J. 2000. Selection of conserved blocks for multiple alignments for their use in phylogenetic alignments. Mol. Biol. Evol., 17:540-552.
CHANG, C., S. LIN AND J. CHEN. 2008. Molecular systematic and phylogeography of the gigantic earthworms of the Metaphire formosae species group (Clitellata, Megascolecidae). Mol. Phylogenet. Evol., 49:958-968.
CHEVENET, F., C. BRUN, A. L. BANULS, B. JACQ AND R. CHRISTEN. 2006. TreeDyn: towards dynamic graphics and annotations for analyses of trees. BMC Bioinform., 7:439.
COLEMAN, J. AND D. H. SHAIN. 2009. Clitellate cocoons and their secretion, p. 328-346. In: D. H. Shain (ed.). Annelids in Modern Biology. John Wiley & Sons, Inc., Hoboken, New Jersey, USA.
DEFRETIN, R. AND E. DEMAILLY. 1953. Sur quelques caracteres histochimique des divers types de cellules glandulaires du clitellum du Lombric. C. r. Seanc. Soc. Biol., 147:1251-1253.
DEREEPER, A., V. GUIGNON, G. BLANC, S. AUDIC, S. BUFFET, F. CHEVENET, J.-F. DUFAVARD, S. GUINDON, V. LEFORT, M. LESCOT, J.-M. CLAVERIE AND O. GASCUEL. 2008. Phylogeny.fr: robust phyogenetic analysis for the non-specialist. Nucl. Acids Res., 36:W465-W469.
EDGAR, R. C. 2004. MUSCLE: a multiple sequence alignment method with reduced time and space complexity. BMC Bioinform., 32:1792-1797.
EDWARDS, C. A. 2004. Earthworm Ecology. CRC Press, Boca Raton, Florida.
ELDREDGE, N. AND S. J. GOULD. 1972. Punctuated equilibria: an alternative to phyletic gradualism, p. 82-115. In: T. M. Schopf (ed.). Models in Paleobiology. Freeman Cooper, San Francisco, California.
FLEMING, T. P. AND P. J. BARON. 1982. The histochemistry of the clitellum of Tubifex tubifex (Annelida: Oligochaeta). Folia Hiostochem. Cytochem., 20:109-128.
FOLMER, O., M. BLACK, W. HOEH, R. LUTZ AND R. VRIJENHOEK. 1994. DNA primers for amplification of mitochondrial cytochrome c oxidase subunit 1 from diverse metazoan invertebrates. Mol. Mar. Biol. Biotechnol., 3:294-299.
GATES, G. E. 1972. Burmese earthworms, an introduction to the systematics and biology of Megadrile oligochaetes with special reference to South-East Asia. Trans. Am. Phil. Soc., 62:1-326.
GUINDON, S. AND O. GASCUEL. 2003. A simple, fast and accurate algorithm to estimate large phylogenies by maximum likelihood. Syst. Biol., 52:696-704.
GROVE, M. A. 1925. On the reproductive processes of the earthworm, Lumbricus terrestris. Quart. J. Microscop. Sci., 69:245-290.
--AND L. F. COWLEY. 1927. The relation of the glandular elements of the clitellum of the Brandling worm (Eisenia foetida, Sav.) to the secretion of the cocoon. Quart. J. Microscop. Sci., 71:31-45.
JAMES, S. W. AND G. G. BROWN. 2006. Earthworm ecology and diversity in Brazil, p. 56-116. In: F. M. S. Moreira, J. O. Siqueira and L. Brussaard (eds.). Soil biodiversity in Amazonian and other Brazilian ecosystems. CAB International, Wallingford.
KNOWLTON, N., L. A. WEIGT, L. A. SOLORANZO, D. K. MILLS AND E. BERMINGHAM. 1993. Divergence in proteins, mitochondrial DNA, and reproductive compatibility across the isthmus of Panama. Science, 260:1629-1632.
LEE, K. E. 1959. The earthworm fauna of New Zealand. New Zealand Department of Scientific and Industrial Research, Wellington. Bulletin 130, 486 p.
LUFTY, R. G. 1965. Studies on the skin of oligochaetes. 1. On the histology, cytology, and histochemistry of the clitellum of Allolobophora caliginosa. Proc. Egypt. Acad. Sci., 19:65-76.
MAHESHWARI, H. G., T. R. PREZANT, V. HERMAN-BONERT, H. SHAHINIAN, K. KOVACS AND S. MELMED. 2000. Long-Acting Peptidomimergic Control of Gigantism Caused by Pituitary Acidophilic Stem Cell Adenoma. J. Clin. Endocrin. Metab., 85:3409-3416.
NIJHOUT, F. H. 1998. Insect Hormones. Princeton University Press, Princeton, New Jersey. 280 p.
OMODEO, P. 2000. Evolution and biogeography of megadriles (Annelida, Clitellata). Ital. J. Zool., 67:179-201.
PLISKO, J. D. 1999. Designation of lectotypes for Microchaetus microchaetus (Rapp, 1849) and Microchaetus rappi Beddard, 1886, and historical perspectives on these species (Oligochaeta: Microchaetidae). Ann. Natal Mus., 40:269-276.
SAYERS, C. W., J. COLEMAN AND D. H. SHAIN. 2009. Cell dynamics during cocoon secretion in the aquatic leech, Theromyzon tessulatum (Annelida: Clitellata: Glossiphoniidae). Tiss. Cell, 41:35-42.
SHEEHAN, D. ANB B. HRAPCHAK. 1980. Theory and Practice of Histology. CV Mosby Co., St. Louis.
STEPHENSON, J. 1930. The Oligochaeta. Clarendon Press, Oxford. 978 p.
THOMPSON, J. D., D. G. HIGGINS AND T. J. GIBSON. 1994. CLUSTAL W: improving the sensitivity of progressive multiple sequence alignment through sequence weighting, position-specific gap penalties and weight matrix choice. Nucl. Acids Res., 22:4673-4680.
VAN PRAAGH, B. 1992. The biology and conservation of the giant Gippsland earthworm Megascolides australis McCoy, 1878. Soil Biol. Biochem., 24:1363-1367.
SUBMITTED 9 MAY 2011
ACCEPTED 4 NOVEMBER 2011
SHIRLEY A. LANG
Biology Department, 315 Penn Street, Rutgers The State University of New Jersey, Camden 08102
MARCOS V. GARCIA
Embrapa Amazonia Ocidental, C.P. 319, 69.001-970 Manaus/AM, Brazil
SAMUEL W. JAMES
Biodiversity Institute, Kansas University, Lawrence 66045
CHARLENE W. SAYERS
Biology Department, 315 Penn Street, Rutgers The State University of New Jersey., Camden 08102
DANIEL H. SHAIN (1)
Biology Department, 315 Penn Street, Rutgers The State University of New Jersey, Camden 08102
(1) Corresponding author: e-mail: email@example.com; Telephone: (856) 225-6144; FAX: (856) 225-6312
TABLE 1.--Description of field sites and number of Rhinodrilus specimens examined Geographic Number Field site coordinates examined Instituto Nacional 02[degrees] 37[degrees] 33"S 5 de Pesquisas 60[degrees] 02[degrees] 39"W Amazonia (INPA) RPPN (near Encontro 03[degrees] 06[degrees] 53"S 2 das Aguas) 59[degrees] 54[degrees] 17"W Universidade Federal 02[degrees] 38[degrees] 44"S 9 do Amazonas (UFAM) 60[degrees] 02[degrees] 44"W experimental farm Private farm (PF) 02[degrees] 54[degrees] 33"S 7 59[degrees] 56[degrees] 34"W Col Field site haplotypes Instituto Nacional 3 de Pesquisas Amazonia (INPA) RPPN (near Encontro 1 das Aguas) Universidade Federal 3 do Amazonas (UFAM) experimental farm Private farm (PF) 2
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