Open Access

Molecular characterization of freshwater snails in the genus Bulinus: a role for barcodes?

  • Richard A Kane1Email author,
  • J Russell Stothard1,
  • Aidan M Emery1 and
  • David Rollinson1
Parasites & Vectors20081:15

DOI: 10.1186/1756-3305-1-15

Received: 10 April 2008

Accepted: 10 June 2008

Published: 10 June 2008

Abstract

Background

Reliable and consistent methods are required for the identification and classification of freshwater snails belonging to the genus Bulinus (Gastropoda, Planorbidae) which act as intermediate hosts for schistosomes of both medical and veterinary importance. The current project worked towards two main objectives, the development of a cost effective, simple screening method for the routine identification of Bulinus isolates and the use of resultant sequencing data to produce a model of relationships within the group.

Results

Phylogenetic analysis of the DNA sequence for a large section (1009 bp) of the mitochondrial gene cytochrome oxidase subunit 1 (cox1) for isolates of Bulinus demonstrated superior resolution over that employing the second internal transcribed spacer (its2) of the ribosomal gene complex. Removal of transitional substitutions within cox1 because of saturation effects still allowed identification of snails at species group level. Within groups, some species could be identified with ease but there were regions where the high degree of molecular diversity meant that clear identification of species was problematic, this was particularly so within the B. africanus group.

Conclusion

The sequence diversity within cox1 is such that a barcoding approach may offer the best method for characterization of populations and species within the genus from different geographical locations. The study has confirmed the definition of some accepted species within the species groups but additionally has revealed some unrecognized isolates which underlines the need to use molecular markers in addition to more traditional methods of identification. A barcoding approach based on part of the cox1 gene as defined by the Folmer primers is proposed.

Background

Freshwater snails belonging to the genus Bulinus act as intermediate hosts in the life cycle of the widespread and debilitating parasitic disease schistosomiasis in Africa, Madagascar and adjacent regions (see Fig. 1). Schistosome species within the S. haematobium group which depend on snails from Bulinus for transmission include three human pathogens (S. haematobium, S. intercalatum and S. guiniensis) and five others which may infect wild and domestic ruminants (S. bovis, S. curassoni, S. mattheei, S. leiperi and S. margrebowiei). The relationship and interaction between schistosomes and snails is very specific and compatibility may differ over quite small geographical ranges [1]. A reliable taxonomy of the genus Bulinus is a fundamental prerequisite for understanding the epidemiology of this disease.
https://static-content.springer.com/image/art%3A10.1186%2F1756-3305-1-15/MediaObjects/13071_2008_Article_15_Fig1_HTML.jpg
Figure 1

Bulinus wrighti. Bulinus wrighti an intermediate host of Schistosoma haematobium in South Yemen.

The thirty six species within the genus have been placed into four species 'groups' [2]; the B. africanus group, B. forskalii group, B. reticulatus group and the B. truncatus/tropicus complex. For the most part, species have been classified on the basis of their morphology although, in recent decades, the study of ploidy [3], allozymes [46] and DNA methods [713] have all played an increasing role in species discrimination. Morphological characters, whilst adequate to allocate a specimen to a species group are sometimes unreliable when used to classify at higher resolution [8, 10] especially within the B. africanus group. Consequently, there is a requirement for a robust system of identification and classification to supplement more traditional approaches. The data presented here represent initial steps towards achieving consistency and uniformity in the identification process. Nuclear (its2) and mitochondrial (cox1) sequences are compared with respect to their ability to resolve species and species group relationships within Bulinus and cox1 is used to screen 81 isolates and place them in a phylogenetic context.

Methods

Samples

The available samples selected for study represented as diverse a group as possible within the genus Bulinus and comprised of both collected and donated material that took the form of specimens from the field and maintained cultures which were stored in liquid nitrogen, ethanol or used fresh (Table 1). Those specimens preserved in ethanol were left in TE buffer pH 7.4 overnight in order to perfuse out any remaining alcohol from within the tissue that might interfere with subsequent extraction techniques.
Table 1

Isolates included in the study with key to alphanumeric identifiers used in the Figures.

Label on tree

Field collected (F) or Lab culture (L)

Putative identification

Sample origin

GPS Co-ordinate where available

Accession numbers

A1

F

B. globosus

Pemba Island, Tanzania

S05 24 626/E39 43 756

AM921823

A2

F

B. globosus

Ngwachani school, Pemba Island, Tanzania

S05 19 364/E39 44 517

AM921826

A3

F

B. globosus

Chan-jamjawiri, Pemba Island, Tanzania

S05 18 094/E39 45 192

AM921828

A4

F

B. globosus

Machengwe, Pemba Island, Tanzania

S05 04 957/E39 45 814

AM921829

A5

F

B. globosus

Kimbuni, Pemba Island, Tanzania

S05 21 231/E39 42 841

AM921830

A6

F

B. globosus

Road to Mtangani, Pemba Island, Tanzania

S05 21 525/E39 46 122

AM921820

A7

F

B. globosus

Road to Mtangani, Pemba Island, Tanzania

S05 21 600/E39 46 125

AM921825

A8

F

B. globosus

Ngwachani school, Pemba Island, Tanzania

S05 19 364/E39 44 517

AM921827

A9

F

B. globosus

Pietermaritzburg, South Africa (Prof. K. N. De Kock)

 

AM286289

A10

F

B. globosus

Pietermaritzburg, South Africa (Prof. K. N. De Kock)

 

AM286290

A11

F

B. globosus

Tiengre stream, Kisumu, West Kenya (via DBL)

 

AM286285

A12

F

B. globosus

Tiengre stream, Kisumu, West Kenya (via DBL)

 

AM286284

A13

F

B. globosus

Kandaria dam, Kisumu, West Kenya (via DBL)

 

AM286286

A14

F

B. globosus

Ipogoro, Iringa, Tanzania

 

AM286288

A15

F

B. globosus

Lugufu, Tanzania (Dr E. Michel)

S05 05 371/E30 11 689

AM286287

A16

F

B. globosus

IRDC farm, Iringa, Tanzania (Dr S. Walker)

S07 46 290/E35 45 590

AM921821

A17

F

B. globosus

IRDC farm, Iringa, Tanzania (Dr S. Walker)

S07 46 285/E35 45 355

AM921824

A18

F

B. globosus

Moyo, Uganda

N03 28 219/E31 55 360

AM286291

A19

F

B. globosus

Moyo, Uganda

N03 28 219/E31 55 360

AM921843

A20

F

B. globosus

Moyo, Uganda

N03 28 219/E31 55 360

AM921851

A21

F

B. globosus

Kachetu, East Kenya

S03 54 350/E39 32 250

AM921847

A22

F

B. globosus

Mwamduli, East Kenya

S03 54 350/E39 31 470

AM921850

A23

F

B. globosus

Kinyasini, Unguja Island, Tanzania

S05 58 180/E39 18 573

AM286292

A24

F

B. globosus

Kinango, East Kenya

S04 05 263/E39 18 721

AM921845

A25

F

B. globosus

Kinango, East Kenya

S04 05 263/E39 18 721

AM921844

A26

F

B. globosus

Kinyasini, Unguja, Island, Tanzania

S05 58 180/E39 18 573

AM921839

A27

F

B. globosus

Kinyasini, Unguja, Island, Tanzania

S05 58 180/E39 18 573

AM921840

A28

F

B. africanus

Isipingo, Durban, South Africa, (Prof. C. Appleton)

S29 58 584/E30 55 503

AM286295

A29

F

B. africanus

Isipingo, Durban, South Africa, (Prof. C. Appleton)

S29 58 584/E30 55 503

AM286296

A30

F

B. globosus

Mogtedo barrage, Burkina Faso

N12 18 388/W00 49 670

AM286293

A31

F

B. globosus

Tondia, Niger

N14 28 348/W01 05 635

AM286294

A32

F

B. globosus

Thiekeene Hulle, Senegal

 

AM921808

A33

F

Bulinus sp

ADC farm, Kisumu, West Kenya (via DBL)

 

AM286297

A34

F

Bulinus sp

Lake Sagara, Tanzania (Dr E. Michel)

S05 15 084/E31 05 111

AM286298

A35

F

B. nasutus productus

Road to Cawente, Uganda

N01 49 341/E33 32 235

AM921815

A36

F

B. nasutus productus

Road to Cawente, Uganda

N01 49 341/E33 32 235

AM921816

A37

F

B. nasutus productus

Ihayabuyaga, Tanzania

 

AM286300

A38

F

B. nasutus productus

Njombe Rujewa, Tanzania, (Dr S. Walker)

 

AM921833

A39

F

B. nasutus productus

Ihayabuyaga, Tanzania

 

AM286301

A40

F

B. nasutus productus

Kahangara, Tanzania

 

AM286302

A41

F

B. nasutus nasutus

Vitonguji, Pemba Island, Tanzania

S05 14 027/E39 49 706

AM921810

A42

F

B. nasutus nasutus

Pujini Kikweche, Pemba Island, Tanzania

S05 18 843/E39 47 863

AM921822

A43

F

B. nasutus nasutus

Pujini, Pemba Island, Tanzania

S05 18 988/E39 48 667

AM921813

A44

F

B. nasutus nasutus

Vitonguji, Pemba Island, Tanzania

S05 14 027/E39 49 706

AM921809

A45

F

B. nasutus nasutus

Muyuni, Unguja, Tanzania

S06 22 707/E39 27 849

AM286299

A46

F

B. nasutus nasutus

Pemba Island, Tanzania

S05 10 272/E39 49 319

AM921812

A47

F

B. nasutus nasutus

Pemba Island, Tanzania

S05 10 272/E39 49 319

AM921811

A48

F

B. nasutus nasutus

Mafia Island, Tanzania

S07 50 838/E39 47 354

AM921831

A49

F

B. nasutus nasutus

Bovo, East Kenya

S04 28 054/E39 28 108

AM921849

A50

F

B. nasutus nasutus

Nimbodze, East Kenya

S04 28 317/E39 27 092

AM921841

A51

F

B. nasutus nasutus

Nimbodze, East Kenya

S04 28 323/E39 27 098

AM921846

F52

F

Bulinus sp

Road to Cawente, Uganda

N01 49 341/E33 32 235

AM921819

F53

F

B. camerunensis

Lake Barombi, Kotto, Cameroon

 

AM286309

F54

F

B. forskalii

Mogtedo barrage, Burkina Faso

N12 18 388 W00 49 670

AM286310

F55

F

B. forskalii

Satoni, Niger

 

AM286308

F56

L

B. forskalii

Dakar, Senegal

 

AM286307

F57

L

B. forskalii

City of São Tomé, São Tomé Island

 

AM286305

F58

L

B. forskalii

Quifangondo, Province of Bengo, Angola

 

AM286306

F59

F

Bulinus sp

Pemba Island, Tanzania

S04 55 682/E39 44 271

AM921832

F60

F

Bulinus sp

Kamwiju Kaloleni, East Kenya

 

AM921848

F61

L

B. cernicus

Mont Oreb, Mauritius

 

AM286303

F62

L

B. cernicus

Perebere, Mauritius

 

AM286304

F63

F

B. barthi

Kangagani, Pemba Island, Tanzania

S05 09 911/E39 49 527

AM921818

F64

F

B. barthi

Kanga swamp, Mafia Island, Tanzania

S07 43 358/E39 51 505

AM921814

F65

F

B. barthi

Kanga swamp, Mafia Island, Tanzania

S07 43 362/E39 51 505

AM921817

R66

L

B. wrighti

Oman (via Perpignan)

 

AM286318

T67

L

B. natalensis

Lake Sibaya, South Africa

 

AM286311

T68

L

B. natalensis

Lake Sibaya, South Africa

 

AM921835

T69

L

B. natalensis

Lake Sibaya, South Africa

 

AM921836

T70

F

B. tropicus

Njombe Kibena, Tanzania, (Dr S. Walker)

S09 12 229/E34 47 041

AM921842

T71

F

B. tropicus

Njombe Kibena, Tanzania, (Dr S. Walker)

S09 12 229/E34 47 041

AM921834

T72

F

B. tropicus

Njombe Kibena, Tanzania, (Dr S. Walker)

S09 12 229/E34 47 041

AM921837

T73

F

B. nyassanus

Kasankha, Monkey Bay, Lake Malawi

Transect line north: E07 00 595/N84 38 260 Transect line south: E07 00 617/N84 38 277

AM921838

T74

F

B. truncatus

Nyanguge, Tanzania

 

AM286313

T75

F

B. truncatus

Posada, Sardinia (Prof. Marco Curini Galletti & Dr D.T.J. Littlewood)

N40 38 092/E09 40 522

AM286312

T76

L

B. truncatus

Mondego River, Coimbra, Portugal (Prof. M.A. Gracio)

 

AM286314

T77

F

B. truncatus

Mbane, Senegal

 

AM921806

T78

F

B. truncatus

Bouton Batt, Senegal

 

AM921807

T79

F

B. truncatus

Mogtedo barrage, Burkina Faso

N12 18 388/W00 49 670

AM286315

T80

F

B. truncatus

Satoni, Niger

N14 26 671/E01 07 257

AM286316

T81

F

B. truncatus

Satoni, Niger

N14 26 685/E01 07 316

AM286317

B. glabrata

 

B. glabrata

Brazil

 

AY380531

Extraction of genomic/mitochondrial DNA

Total genomic DNA was extracted from whole snail tissue in a manner similar to that outlined by Stothard et al [7] with minor modification. Snail tissue was homogenized in lysis buffer (100 mM Tris, 1.4 M NaCl, 16 mM EDTA, 2% hexadecyltrimethylammonium bromide [CTAB]). To this was added 20 μl of proteinase K (20 mg/ml) and the whole mixed in a rotisserie incubator at 55°C for 1.5 to 2.0 hours. Subsequently, an equal volume of chloroform/isoamyl alcohol (24:1) was added to the digest and gently mixed. Tubes containing the digest were then spun at 13,000 rpm for 10 minutes. The upper aqueous layer was removed using 'wide bore' pipette tips and nucleic acids were precipitated in 'Analar' grade absolute ethanol. Following precipitation for 15 minutes at -20°C, the DNA was centrifuged again at 13,000 rpm to form a pellet. The absolute ethanol was removed and the pellet washed in 70% ethanol before a final centrifugation at 13,000 rpm. The ethanol was then discarded and the pellet dried in a dry heating block at 90°C for 5 minutes before dissolution in an appropriate amount of purified water.

Amplification of cox1 and its2 fragments

The partial cox1 fragment was amplified in one, two or more sections from the mitochondrial component of extracted total genomic DNA using the polymerase chain reaction (PCR) and various combinations of the primers that are shown in Table 2 (see additional file 1, for PCR and sequencing primers that proved successful with particular isolates and Fig. 2 for approximate primer locations). Amplicons of its2 were generated in a single section using two primers ETTS1 and ETTS10 (see Table 2). Either an Applied Biosystems GeneAmp PCR System 2400 or 2700 thermal cycler were used throughout the project in combination with GE Healthcare 'Ready-To-Go' PCR beads. Upon reconstitution with an appropriate volume of template, primer and pure water to a total of 25 μl, each dissolved bead forms a solution containing 200 μM of each dNTP, 10 mM Tris-HCl, 50 mM KCl and 1.5 mM of MgCl2. Cycling conditions for both cox1 and its2 PCR reactions were as follows: one cycle of 94°C for 5 min, 45 cycles of 94°C for 15 sec, 40°C for 30 sec and 72°C for 45 sec (in the case of cox1 this was increased to 1 min for amplicons over 1000 bp) and a final single cycle of 72°C for 7 min. PCR fragments were separated on a 1% agarose gel and bands were excised using a scalpel blade. The recovered DNA was purified for sequencing using a QIAquick Gel Extraction Kit (Qiagen). Following quantification and a check for purity with a Nanodrop ND-1000 Spectrophotometer (Nanodrop Technologies Inc), sequencing reactions were performed directly on each PCR product using an Applied Biosystems Big Dye Kit version 1.1 and run on an Applied Biosystems 3730 DNA Analyzer. Resultant electropherograms were checked and cox1/its2 sequences edited using Sequencher 4.6 software (Gene Codes Corporation).
Table 2

Primers used for PCR amplification and sequencing

Primer name

Cytochrome oxidase subunit 1 – primer sequence

Forward or Reverse

Source

Asmit1 (AT1)

5' TTT TTT GGG CAT CCT GAG GTT TAT 3'

Forward

[26]

Asmit2 (AT2)

5' TAA AGA AAG AAC ATA ATG AAA ATG 3'

Reverse

[26]

CO1 (LC1490)

5' GGT CAA CAA ATC ATA AAG ATA TTG G 3'

Forward

[18]

CO2 (HCO2198)

5' TAA ACT TCA GGG TGA CCA AAA AAT CA 3'

Reverse

[18]

BulCox1 (BC1)

5' TTT TTG GWG TTT GAT GTG G 3'

Forward

NHM – current project

BulCox2 (BC2)

5' TGT GGT CTG GTA GGW ACC GG 3'

Forward

NHM – current project

BulCox3 (BC3)

5' CGT GGA AAW CTT ATA TCW GGW GC 3'

Reverse

NHM – current project

BulCox4 (BC4)

5' GCW CCW GAT ATA AGW TTT CCA CG 3'

Forward

NHM – current project

BulCox5 (BC5)

5' CCT TTA AGA GGN CCT ATT GC 3'

Forward

NHM – current project

BulCox6 (BC6)

5' CAA TAA ACC CTA AAA TYC C 3'

Reverse

NHM – current project

BulCox7 (BC7)

5' GCA ATA GGT CCT CTT AAA GG 3'

Reverse

NHM – current project

BulCox8 (BC8)

5' GTA ATA AAA TTA ATW GCA CCT AAA A 3'

Reverse

NHM – current project

BulCox9 (BC9)

5' CCW CCT TCA TTT ATT TT 3'

Forward

NHM – current project

BulCox10 (BC10)

5' GCT AAA TGT AAA G 3'

Reverse

NHM – current project

BulCox11 (BC11)

5' TTT TGG DRT YTG RTG YGG 3'

Forward

NHM – current project

BulCox12 (BC12)

5' GCG TTG ACT CTT TTC AAC 3'

Forward

NHM – current project

BulCox13 (BC13)

5' CWT TRT AYW TAA TTT TTG G 3'

Forward

NHM – current project

BulCox14 (BC14)

5' GGA AAT CAG TAM AYA AAA CCA GC 3'

Reverse

NHM – current project

BulAsmit3 (BAT3)

5' CAT AAT GAA AAT GAG CAA CTA C 3'

Reverse

NHM – current project

BulAsmit4 (BAT4)

5' CAT AAT GAA AAT GAG C 3'

Reverse

NHM – current project

Primer name

Second internal transcribed spacer of the ribosomal gene complex – primer sequence

Forward or Reverse

Source

ETTS1

5' TGC TTA AGT TCA GCG GGT 3'

Reverse

[27]

ETTS10

5' GCA TAC TGC TTT GAA CAT CG 3'

Forward

[27]

https://static-content.springer.com/image/art%3A10.1186%2F1756-3305-1-15/MediaObjects/13071_2008_Article_15_Fig2_HTML.jpg
Figure 2

Locations of primers used for the cox1 fragment. Locations of primers used for cox1 PCR amplification and sequencing. Folmer and Asmit regions are indicated. Not to scale.

Phylogenetic analysis of sequence data

Following basic editing and analysis of compiled cox1 and its2 sequences on Sequencher 4.6, the sequences were used to perform BLAST searches [14] via the National Center for Biotechnology Information against GenBank and EMBL sequence databases in order to ensure that parasitic and other potential contaminant sequences had not been obtained in error. Sequences were then aligned and analysed using MEGA 3.1 [15] where alignment was undertaken using Clustal W [16]. The cox1 data for all taxa were analysed solely as nucleotides and subject to analysis by both Neighbour-Joining and Minimum Evolution methods using Kimura's 2 parameter model (K2P) for pair-wise distance calculations as this accommodates the difference in the rate of accumulation between transitions and transversions. The Minimum Evolution algorithm employed Close-Neighbour-Interchange (CNI – level 1) to explore the most optimal topology with the initial, temporary tree obtained by Neighbour-Joining. All gaps were deleted from the dataset using the 'complete deletion' option in MEGA 3.1 and the invertebrate mitochondrial code was used throughout. Nucleotide sequence data for its2 was analysed in a similar manner except that p-distance was employed instead of K2P.

The different forms of analysis were subject to bootstrapping (1000 repeats) as a means of testing the reliability of individual branches within the generated tree. Biomphalaria glabrata was used as an outgroup taxon upon which to root the structures. Sequence saturation for cox1 was visualized graphically, using the program DAMBE [17] that allows the number of differences between isolates or species in terms of transitional and transversional substitutions to be plotted against pair-wise distance values.

Sequences have been submitted to the EMBL database and have accession numbers [EMBL:AM286284 to AM286318, EMBL:AM921806 to AM921851 (cox1) and EMBL:AM921961 to AM921990 (its2)].

Results

Analysis of its2 sequence data

Twenty nine samples were selected for sequencing of an amplicon containing the 3' end of the 5.8S gene and the entire its2 region. This was undertaken in order to compare the phylogenetic signal of a nuclear marker with that of cox1 (see Fig. 3). Both loci were able to discriminate the 4 species groups in a Neighbour-Joining tree. The B. forskalii, B. reticulatus and B. truncatus/tropicus species groups resolved well, the main point of difference being F52 which in the its2 tree had closer affinity with the East African B. forskalii group snails. The B. africanus group within the its2 tree had short branch lengths with poor resolution and bootstrap values. Clear discrimination between B. nasutus nasutus and B. nasutus productus was not possible using the its2 data and sequence differences in this region are unlikely to be of value for the detection of hybridization events among isolates with overlapping geographic ranges. The its2 sequence data for B. wrighti were unusual in having two unique insertions relative to other Bulinus isolates, a short 16 bp insertion between fragment positions 219 and 234 and a larger 63 bp insertion between positions 248 and 310.
https://static-content.springer.com/image/art%3A10.1186%2F1756-3305-1-15/MediaObjects/13071_2008_Article_15_Fig3_HTML.jpg
Figure 3

Comparison of cox1 and its2 Neighbour-Joining trees for Bulinus. Comparison of Neighbour-Joining trees for cox1 and its2 data (cox1 – 1010 sites and its2 – 394 sites). Kimura 2-parameter distance has been used for cox1 and p-distance for its2. Substitutions include both transitions and transversions and 1000 bootstrap replicates have been performed. Bootstrap values below 50 are not shown. B. africanus group isolates are shown in red, B. forskalii in green, B. reticulatus in black and B. truncatus/tropicu s in blue. See Table 1 for origins of isolates.

Analysis of cox1 sequence data

The sequence of the mitochondrial cox1 gene within Bulinus was found to be highly variable. The nucleotide composition regarding this genus was AT rich (69.4%) which is in close agreement with previous work [12]. In order to test which areas of the cox1 amplicon gave the best phylogenetic signal, the fragment was analysed in its entirety, using the first 644 bp and also the final 387 bp. Stothard and Rollinson [9] and Jones et al [12] used the latter section of the cox1 sequence and this corresponds to the region encompassed by primers Asmit1 (AT1) and Asmit2 (AT2) shown in Fig. 2. The first 644 bp covers an area comparable to the sequence bounded by the Folmer primers LCO1490 (CO1) and HCO2198 (CO2) [18] and which has been used previously for barcoding studies [19]. Figure 4 shows three Neighbour-Joining trees generated for each region using both transitional and transversional substitutions. Resolution of the tree improves as progressively longer stretches of sequence are included in the analysis. However, saturation analysis of the 'Asmit' and 'Folmer' regions show that both are subject to saturation of transitional events suggesting that inclusion of transversional substitutions only in the calculation would present a more accurate estimate of isolate relationships within the genus. Figure 5 shows a graph where mean, pair-wise genetic distances of the two areas calculated from transversional substitutions only are compared with the corresponding distance matrix co-ordinates for the complete fragment. In this manner, the variability of genetic distance figures for the 'Asmit' and 'Folmer' regions relative to the complete fragment may be shown. For small genetic distance values correspondence is good between the three regions, however, as distances increase in size those associated with the 'Asmit' fragment tend to drift away from the corresponding complete sequence derived genetic distance values within the mid-range of the 'x' axis. Distances of the 'Folmer' region also exhibit a degree of variation when compared with those of the complete fragment but to a smaller extent. Additionally, a short span of genetic distance values between approximately 0.058 and 0.064 is entirely missing within the dataset. To a lesser degree this is reflected in a smaller region between 0.013 and 0.018. Figure 6 shows the same procedure undertaken for transitional substitutions where correspondence of distance values for the 'Asmit' and 'Folmer' areas again 'drifts' with increasing genetic distance relative to the complete fragment. However, whilst the overall number of pairs contributing to each distance figure is considerably less than in Fig. 5, the numerical variation of distance values present in the matrices is far greater, particularly between the ranges 0.035 to 0.077. Neighbour-Joining and Minimum Evolution trees were therefore generated for the dataset using transversions from the complete fragment sequence in order to obtain the maximum resolution possible. The resultant trees contained divisions corresponding to the four species groups (see Figs 7 &8).
https://static-content.springer.com/image/art%3A10.1186%2F1756-3305-1-15/MediaObjects/13071_2008_Article_15_Fig4_HTML.jpg
Figure 4

Three regions of the cox1 fragment compared using Neighbour-Joining trees. Comparison of Neighbour-Joining trees using Kimura 2-parameter distance for 'Asmit' (final 387 sites), 'Folmer' (first 644 sites) and 'complete' (1009 sites) sections of the cox1 gene. Substitutions include both transitions and transversions and 1000 bootstrap replicates have been performed. Bootstrap values below 50 are not shown. B. africanus group isolates are shown in red, B. forskalii in green, B. reticulatus in black and B. truncatus/tropicu s in blue. See Table 1 for origins of isolates.

https://static-content.springer.com/image/art%3A10.1186%2F1756-3305-1-15/MediaObjects/13071_2008_Article_15_Fig5_HTML.jpg
Figure 5

Comparison of regional cox1 genetic distances using transversions only. Plot showing mean, pair-wise genetic distance values of the 'Asmit' and 'Folmer' regions using transversions only as compared with the corresponding values for the complete fragment. Number of pairs contributing to each value is shown graphically.

https://static-content.springer.com/image/art%3A10.1186%2F1756-3305-1-15/MediaObjects/13071_2008_Article_15_Fig6_HTML.jpg
Figure 6

Comparison of regional cox1 genetic distances using transitions only. Plot showing mean, pair-wise genetic distance values of the 'Asmit' and 'Folmer' regions using transitions only as compared with the corresponding values for the complete fragment. Number of pairs contributing to each value is shown graphically.

https://static-content.springer.com/image/art%3A10.1186%2F1756-3305-1-15/MediaObjects/13071_2008_Article_15_Fig7_HTML.jpg
Figure 7

Neighbour-Joining tree for Bulinus isolates using the complete cox1 fragment, transversions only. Neighbour-Joining tree for the complete cox1 fragment (1009 sites) using Kimura 2-parameter distance and utilizing transversional substitutions only. 1000 bootstrap replicates have been performed. Bootstrap values below 50 are not shown. B. africanus group isolates are shown in red, B. forskalii in green, B. reticulatus in black and B. truncatus/tropicu s in blue. See Table 1 for origins of isolates.

https://static-content.springer.com/image/art%3A10.1186%2F1756-3305-1-15/MediaObjects/13071_2008_Article_15_Fig8_HTML.jpg
Figure 8

Minimum Evolution tree for Bulinus isolates using the complete cox1 fragment, transversions only. Minimum Evolution tree for the complete cox1 fragment (1009 sites) using Kimura 2-parameter distance and utilizing transversional substitutions only. 1000 bootstrap replicates have been performed. Bootstrap values below 50 are not shown. B. africanus group isolates are shown in red, B. forskalii in green, B. reticulatus in black and B. truncatus/tropicu s in blue. See Table 1 for origins of isolates.

Discussion

B. africanus species group

Classification within this complex is probably the most difficult of the four Bulinus snail species groups. The cox1 sequence data for samples within this group revealed an extensive degree of genetic variation throughout the continent (see the designation 'A' in Figs 7 &8). There are three areas within the data set that may be used as reference points for interpretation of Figs 7 &8. The first is identified by sample code A23, a snail from Kinyasini, Unguja, which on the basis of previous work [8, 9, 20], represents the species known as B. globosus. The second are samples of B. africanus, from South Africa, namely, A28 and A29 and the third are those specimens labelled A35 to A40 and A41 to A51 representing B. nasutus productus and B. nasutus nasutus, respectively. The split of B. nasutus into two subspecies as recognised previously [2] may be clearly seen in Figs 7 &8 with B. nasutus productus being represented by samples from inland sites in Uganda and Tanzania and B. nasutus nasutus present in coastal Kenya and the Islands of Unguja, Pemba and Mafia. The molecular data support the view that these forms are closely related species and it would seem acceptable to consider them as B. productus and B. nasutus.

One of the most interesting facts to emerge is the division between samples of B. globosus from West and East Africa and the rather surprising finding that B. africanus has closer affinities to the West African B. globosus samples. B. globosus has the greatest geographical range of any member of this species group and it does seem that greater attention must be given to specific status and distribution. The cox1 barcode for B. africanus may be helpful in discriminating snails where species overlap especially when morphological differences are often difficult to determine, hence samples A9 and A10 identified as B. globosus can be distinguished from A28 and A29, B. africanus. The two species differ in the penis sheath, which is bigger in B. africanus being longer and/or thicker than the preputium [2] but such characters have been found unreliable for species discrimination [10].

Kenyan specimens from the Kisumu region used by Raahauge and Kristensen [10] have been included in the present study (A11 to A13 & A33). Utilizing RAPD profiles and PCR-RFLP results, these authors concluded that those samples labelled in Figs 7 &8 as A11 to A13 all appeared to be local variants of the same species and this conclusion is confirmed in the present analysis with all of the snails identified as B. globosus. In addition, they also showed that another sample screened in their study (ADC farm, Kisumu), labelled in Figs 7 &8 as A33, was different from the other Kisumu specimens and this has also been supported.

B. forskalii species group

The group as a whole splits into two main sections, namely, snails from West Africa i.e. Cameroon, Bukina Faso, Niger, Senegal, São Tomé and Angola (F53 to F58) and those from the eastern side, East Kenya, Pemba, Mafia and Mauritius (F59 to 65). Additionally, isolate F52 from Uganda although sharing a common ancestor with East and West African B. forskalii group isolates, is quite distinct from the other species. However, only one specimen has been examined and more samples from this locality in Uganda are required for further study. The its2 tree showed F52 to have a closer relationship with East African members of the B. forskalii group. Within this group certain isolates are of known species and can be used as reference points, namely F58, which is B. forskalii, F61 and F62 both being B. cernicus from Mauritius and F63 to F65 from Pemba and Mafia considered by the authors as B. barthi.

Fewer isolates of the B. forskalii group have been tested and analysed as compared with the B. africanus group and so it might be imprudent to draw too many specific conclusions from the data. However, using fifteen allozyme loci from B. camerunensis, B. forskalii and B. senegalensis, Mimpfoundi & Greer [6] could find no differences between the two former species and suggested that the validity of B. camerunensis as a separate species might be open to question. Jones et al [12] used ITS1, RAPDs and cox1 to show that B. camerunensis clustered unequivocally with B. forskalii confirming that the taxonomic position of B. camerunensis is debatable. Only a single example of this species was available for our analysis (F53) although it came from the same area as that examined in Mimpfoundi's paper, namely, Lake Barombi, Kotto. The isolate shared genetic characteristics with B. forskalii from other West African countries such as Burkina Faso (F54) and Niger (F55), re-emphasising its questionable taxonomic status.

Bulinus forskalii from the island of São Tomé (F57) is responsible for the transmission of S. guiniensis and in this analysis grouped most closely to B. forskalii (F58) from Angola with both being well differentiated from other West African B. forskalii. Brown [21] was of the opinion that it was appropriate to identify the snails from São Tomé as extreme conchological variants of B. forskalii. Interestingly, in the analysis of Jones et al [12]B. forskalii from São Tomé clustered with B. crystallinus also from Angola. There is a need to sample and characterize more thoroughly B. forskalii group snails from Angola to assess their relationship with snails from São Tomé and West Africa as it appears that there may be more than one species involved.

B. cernicus from the island of Mauritius was once regarded as a form of B. forskalii, however, significant morphological differences with the latter were noted [2]. The current data reinforces the view that B. cernicus should be considered a separate species from both B. forskalii and B. barthi. Isolates F59 and F60 are also distinct from B. forskalii, B. barthi and B. cernicus. Stothard et al [22] sequenced the short 'Asmit' region for a snail collected from Mafia Island (SF369612). Although covering only a third of the current sequence for F59 and F60 the corresponding data match exactly and imply that this particular un-named Bulinus species is present in Pemba, Mafia and also East Kenya.

B. truncatus/tropicus species group

Both Figs 7 and 8 confirm the position of B. nyassanus in the B. truncatus/tropicus complex and this species together with the cluster comprising B. tropicus, B. natalensis and B. truncatus appear to derive from a common ancestor. However, the conjecture by Nascetti & Bullini [5] that possible hybridization between B. tropicus and B. natalensis might have given rise to B. truncatus cannot be confirmed by the Minimum Evolution tree (Fig. 8). The observation by Brown [2] that there were indications of a "significant biological difference" between B. tropicus and B. natalensis is supported. The cluster representing B. truncatus in Figs 7 &8 has very short branch lengths implying that the hybridization event which Goldman et al. [3] suggested gave rise to this tetraploid is a relatively recent phenomenon.

B. reticulatus group

There are only two recognised species within this group and it has only been possible to examine one of them, B. wrighti. This species has a characteristic cox1 sequence which positions the group close to the B. truncatus/tropicus complex.

Barcoding

The sequence information presented here is not a typical 'barcode' in so far as the sequence is longer than most barcodes which are usually around 650 bp in length [19, 23, 24]. Moreover, the generated PCR fragments have been amplified and sequenced using a wide variety of different primers due to the highly variable nature of the sequence. A pan-species group/isolate barcode in the usual 'sense' might be possible to locate but requires a common set of primers to be designed which will amplify all species within the genus for a particular cox1 region and that the area so determined mirrors the results generated by the current longer sequence. For this reason, a Neighbour-Joining tree (Fig. 9) has been generated for the area of Bulinus cox1 which corresponds approximately with the 'Folmer' barcode region. Agreement of Fig. 9 with Figs 7 &8 whilst not identical is very close and provides hope that this region could be used for barcoding Bulinus species in future.
https://static-content.springer.com/image/art%3A10.1186%2F1756-3305-1-15/MediaObjects/13071_2008_Article_15_Fig9_HTML.jpg
Figure 9

Neighbour-Joining tree for Bulinus isolates using the 'Folmer' cox1 fragment, transversions only. Neighbour-Joining tree using transversional substitutions only for the cox1 'Folmer' region. Calculation parameters are the same as for Figure 7. This region is proposed for potential use as a barcode. Bootstrap values below 50 are not shown. B. africanus group isolates are shown in red, B. forskalii in green, B. reticulatus in black and B. truncatus/tropicu s in blue. See Table 1 for origins of isolates.

The advantages [19] and disadvantages [25] over the use of barcoding, and the utilization of a single mitochondrial gene such as cox1 for identification and phylogenetic purposes have been the subject of considerable debate. It is accepted that a range of both nuclear and mitochondrial markers are required to provide a more accurate estimate of evolutionary history. However, a technique for routine screening which is relatively quick, cost effective and reproducible is essential given that resources are limited. The selected area of sequence from the cox1 gene appears to achieve this by forming a framework upon which a classification can begin to be constructed. Previous studies have used cox1 in the phylogenetic evaluation of Bulinus, namely, Stothard & Rollinson [9], Stothard et al. [11] and Jones et al. [12] and, in this respect, the current project is not unique, however, the sequences used in the present paper are three times the length of those previously employed and the range of Bulinus isolates/species much more extensive. The study is ongoing and undoubtedly as more taxa are acquired and sequences added to the database, the shape of the Neighbour-Joining and Minimum Evolution trees as shown in Figs 7 &8 will progressively alter and become more informative.

Declarations

Acknowledgements

The work was funded in part by the EU contract no: 032203 (A multidisciplinary alliance to optimize schistosomiasis control and transmission surveillance in sub-Saharan Africa).

The authors wish to thank the following for samples used in this work; Professor C. Appleton, University of Kwa-Zulu, Natal, Professor M.A. Gracio, Instituto de Higiene e Medicina Tropical, Lisbon, Dr E. Michel, Natural History Museum, London, Dr T.K. Kristensen, Institute for Health Research and Development, Copenhagen, Dr S. Walker, Queen's University of Belfast, Professor K de Kock, North-West University, South Africa, Professor Marco Curini Galletti, Università di Sassari, Sardinia and Dr D.T.J Littlewood, Natural History Museum, London. We are grateful to our colleagues Michael Anderson for the provision of snail cultures and to Julia Llewellyn-Hughes for operation of the Applied Biosystems 3730 DNA Analyser.

Authors’ Affiliations

(1)
Department of Zoology, Natural History Museum, South Kensington

References

  1. Rollinson D, Stothard JR, Southgate VR: Interactions between intermediate snail hosts of the genus Bulinus and schistosomes of the Schistosoma haematobium group. Parasitol. 2001, 123: S245-S260. 10.1017/S0031182001008046.Google Scholar
  2. Brown DS: Freshwater Snails of Africa and their Medical Importance. Taylor & Francis. 1994Google Scholar
  3. Goldman MA, LoVerde PT, Chrisman CL: Hybrid origin of polyploidy in freshwater snails of the genus Bulinus (Mollusca: Planorbidae). Evolution. 1983, 37: 592-600. 10.2307/2408272.View ArticleGoogle Scholar
  4. Rollinson D, Southgate VR: Enzyme analysis of Bulinus africanus group snails (Mollusca: Planorbidae) from Tanzania. Trans R Soc Trop Med Hyg. 1979, 73: 667-672. 10.1016/0035-9203(79)90017-8.View ArticlePubMedGoogle Scholar
  5. Nascetti G, Bullini L: Genetic differentiation in the Mandahlbarthia truncata complex (Gastropoda: Planorbidae). Parassitologia. 1980, 22: 269-274.PubMedGoogle Scholar
  6. Mimpfoundi R, Greer J: Allozyme comparisons among species of the Bulinus forskalii group (Gastropoda: Planorbidae) in Cameroon. J Moll Stud. 1989, 55: 405-410. 10.1093/mollus/55.3.405.View ArticleGoogle Scholar
  7. Stothard JR, Hughes S, Rollinson D: Variation within the internal transcribed spacer (ITS) of ribosomal DNA genes of intermediate snail hosts within the genus Bulinus (Gastropoda: Planorbidae). Acta Trop. 1996, 61: 19-29. 10.1016/0001-706X(95)00137-4.View ArticlePubMedGoogle Scholar
  8. Stothard JR, Mgeni AF, Alawi KS, Savioli L, Rollinson D: Observations on shell morphology, enzymes and random amplified polymorphic DNA (RAPD) in Bulinus africanus group snails (Gastropoda: Planorbidae) in Zanzibar. J Moll Stud. 1997, 63: 489-503. 10.1093/mollus/63.4.489.View ArticleGoogle Scholar
  9. Stothard JR, Rollinson D: Partial DNA sequences from the mitochondrial cytochrome oxidase subunit I (COI) gene can differentiate the intermediate snail hosts Bulinus globosus and B. nasutus (Gastropoda: Planorbidae). J Nat Hist. 1997, 31: 727-737. 10.1080/00222939700770361.View ArticleGoogle Scholar
  10. Raahauge P, Kristensen TK: A comparison of Bulinus africanus group species (Planorbidae; Gastropoda) by use of the internal transcribed spacer 1 region combined by morphological and anatomical characters. Acta Trop. 2000, 75: 85-94. 10.1016/S0001-706X(99)00086-8.View ArticlePubMedGoogle Scholar
  11. Stothard JR, Brémond P, Andriamaro L, Sellin B, Sellin E, Rollinson D: Bulinus species on Madagascar: molecular evolution, genetic markers and compatibility with Schistosoma haematobium. Parasitol. 2001, 123: S261-S275. 10.1017/S003118200100806X.View ArticleGoogle Scholar
  12. Jones CS, Rollinson D, Mimpfoundi J, Ouma J, Kariuki HC, Noble LR: Molecular evolution of freshwater snail intermediate hosts within the Bulinus forskalii group. Parasitol. 2001, 123: S277-S292. 10.1017/S0031182001008381.Google Scholar
  13. Jorgensen A, Jorgensen LVG, Kristensen TK, Madsen H, Stothard JR: Molecular phylogenetic investigations of Bulinus (Gastropoda: Planorbidae) in Lake Malawi with comments on the topological incongruence between DNA loci. Zoologica Scripta. 2007, 36: 577-585. 10.1111/j.1463-6409.2007.00298.x.View ArticleGoogle Scholar
  14. Altschul SF, Gish W, Miller W, Myers EW, Lipman DJ: Basic local alignment search tool. J Mol Biol. 1990, 215: 403-410.View ArticlePubMedGoogle Scholar
  15. Kumar S, Tamura K, Nei M: MEGA3: Integrated Software for Molecular Evolutionary Genetics Analysis and Sequence Alignment. Brief Bioinform. 2004, 5: 150-163. 10.1093/bib/5.2.150.View ArticlePubMedGoogle Scholar
  16. Thompson JD, Higgins DG, Gibson T: CLUSTAL W: improving the sensitivity of progressive multiple sequence alignment through sequence weighting, position-specific gap penalties and weight matrix choice. Nucleic Acids Res. 1994, 22: 4673-80. 10.1093/nar/22.22.4673.PubMed CentralView ArticlePubMedGoogle Scholar
  17. Xia X, Xie Z: DAMBE: Software package for data analysis in molecular biology and evolution. J Hered. 2001, 92: 371-373. 10.1093/jhered/92.4.371.View ArticlePubMedGoogle Scholar
  18. Folmer O, Black M, Hoeh W, Lutz R, Vrijenhoek R: DNA primers for amplification of mitochondrial cytochrome c oxidase subunit I from diverse metazoan invertebrates. Mol Mar Biol Biotechnol. 1994, 3: 294-299.PubMedGoogle Scholar
  19. Hebert PDN, Cywinska A, Ball SL, deWaard JR: Biological identifications through DNA barcodes. Proc Biol Sci. 2003, 270 (1512): 313-321. 10.1098/rspb.2002.2218.PubMed CentralView ArticlePubMedGoogle Scholar
  20. Stothard JR, Mgeni AF, Khamis S, Seto E, Ramsan M, Rollinson D: Urinary schistosomiasis in schoolchildren on Zanzibar Island (Unguja), Tanzania: a parasitological survey supplemented with questionnaires. Trans R Soc Trop Med Hyg. 2002, 96: 507-514. 10.1016/S0035-9203(02)90421-9.View ArticlePubMedGoogle Scholar
  21. Brown DS: Freshwater snails of São Tomé, with special reference to Bulinus forskalii (Ehrenberg), host of Schistosoma intercalatum. Hydrobiologia. 1991, 209: 141-153.View ArticleGoogle Scholar
  22. Stothard JR, Loxton JL, Rollinson D: Freshwater snails on Mafia Island, Tanzania with special emphasis upon the genus Bulinus (Gastropoda: Planorbidae). J Zool Lond. 2002, 257: 353-364. 10.1017/S095283690200095X.View ArticleGoogle Scholar
  23. Hebert PDN, Penton EH, Burns JM, Janzen DH, Hallwachs W: Ten species in one: DNA barcoding reveals cryptic species in the neotropical skipper butterfly Astraptes fulgerator. Proc Natl Acad Sci U S A. 2004, 101 (41): 14812-14817. 10.1073/pnas.0406166101.PubMed CentralView ArticlePubMedGoogle Scholar
  24. Hebert PDN, Stoeckle MY, Zemlak TS, Francis CM: Identification of birds through DNA barcodes. PLoS Biol. 2004, 2: e312-10.1371/journal.pbio.0020312.PubMed CentralView ArticlePubMedGoogle Scholar
  25. Ballard JWO, Whitlock MC: The incomplete natural history of mitochondria. Mol Ecol. 2004, 13: 729-744. 10.1046/j.1365-294X.2003.02063.x.View ArticlePubMedGoogle Scholar
  26. Bowles J, Blair D, McManus DP: Genetic variants within the genus Echinococcus identified by mitochondrial DNA sequencing. Mol Biochem Parasitol. 1992, 54: 165-174. 10.1016/0166-6851(92)90109-W.View ArticlePubMedGoogle Scholar
  27. Kane RA, Rollinson D: Repetitive sequences in the ribosomal DNA internal transcribed spacer of Schistosoma haematobium, Schistosoma intercalatum and Schistosoma mattheei. Mol Biochem Parasitol. 1994, 63: 153-156. 10.1016/0166-6851(94)90018-3.View ArticlePubMedGoogle Scholar

Copyright

© Kane et al; licensee BioMed Central Ltd. 2008

This article is published under license to BioMed Central Ltd. This is an Open Access article distributed under the terms of the Creative Commons Attribution License (http://creativecommons.org/licenses/by/2.0), which permits unrestricted use, distribution, and reproduction in any medium, provided the original work is properly cited.

Advertisement