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Short Communication
First report and molecular characterization of the dagger nematode, Xiphinema oxycaudatum (Nematoda, Dorylaimidae) from South Africa
expand article infoFisayo Y. Daramola‡, Rinus Knoetze§, Antoinette Swart|, Antoinette P. Malan‡
‡ Department of Conservation Ecology and Entomology, Stellenbosch, South Africa
§ Plant Protection Division, Agriculture Research Council, Stellenbosch, South Africa
| University of Johannesburg, Johannesburg, South Africa
¶ ARC-Plant Protection Research Institute, Queenswood, South Africa

Corresponding author: Fisayo Y. Daramola ( fdaramola@sun.ac.za )

Academic editor: Sergei Subbotin
© 2019 Fisayo Y. Daramola, Rinus Knoetze, Antoinette Swart, Antoinette P. Malan.
This is an open access article distributed under the terms of the Creative Commons Attribution License (CC BY 4.0), which permits unrestricted use, distribution, and reproduction in any medium, provided the original author and source are credited.
Citation: Daramola FY, Knoetze R, Swart A, Malan AP (2019) First report and molecular characterization of the dagger nematode, Xiphinema oxycaudatum (Nematoda, Dorylaimidae) from South Africa. ZooKeys 894: 1-17. https://doi.org/10.3897/zookeys.894.35281
ZooBank: urn:lsid:zoobank.org:pub:EA7DF133-216C-4872-9E9B-A3F73C9B6921
Open Access

Abstract

Plant-parasitic nematodes of the genus Xiphinema Cobb, 1913 comprise a complex group of nematode species, some of which are important vectors of plant viruses. During a field survey to determine the soil health of an abandoned honeybush (Cyclopia genistoides) monoculture, a high density of the dagger nematode, Xiphinema oxycaudatum Lamberti & Bleve-Zacheo, 1979 (Nematoda, Dorylaimidae), was observed in soil around the roots of honeybush plants in an abandoned farmland at Bereaville, an old mission station in the Western Cape province of South Africa. Soil samples were taken from the rhizosphere of plants and nematodes were extracted from the soil using a modified extraction tray method. Specimen of the dagger nematodes were processed for scanning electron microscopy, morphological and molecular analysis. Molecular profiling of the nematode species was done in order to give an accurate diagnosis and to effectively discriminate the nematode from other species within the Xiphinema americanum group. Phylogenetic analysis based on the D2D3 expansion segment of the 28S gene supported a close relationship of species within the americanum group, however, the protein-coding cytochrome oxidase (coxI) of the mitochondrial gene provided a useful tool for distinguishing the nematode from other species within the group. This study represents the first report of X. oxycaudatum from South Africa.

Keywords

coxI, D2D3, honeybush, molecular identification

Introduction

Dagger nematodes, belonging to the Xiphinema americanum-group, are economically important nematodes that may cause damage to agricultural crops, by means of direct feeding on plant roots and in transmitting plant viruses. Xiphinema oxycaudatum Lamberti & Bleve-Zacheo, 1979 (Nematoda, Dorylaimidae) is a polyphagous and cosmopolitan nematode, which was first described from the rhizosphere of oil palm, Elaies guineensis in Nigeria (Lamberti and Bleve-Zacheo 1979). A high population of this nematode species were found in soil around honeybush (Cyclopia genistoides), in an abandoned farmland (-34.0516, 19.5174) at Bereaville in the Western Cape province, South Africa.

Although many nematode species in the X. americanum-group are widespread in distribution, X. oxycaudatum is localized in Africa with a few reports from Asia and South America (Lamberti et al. 2000; Fadaei et al. 2003; Oliveira et al. 2003; Chen et al. 2005). In South Africa, Xiphinema species have been listed as one of the most common and abundant plant parasitic nematodes causing damage on grapevines and woody plants (Fourie et al. 2017). However, only a few species belonging to the Xiphinema americanum-group have been reported in the country, some of these include; X. americanum, X. brevicolle, X. diffusum, X. incognitum, and X. pachtaicum (Lamberti et al. 1995, 2002).

Honeybush is an exclusive African herbal tea with a distinctive honey aroma and it is a rich source of compounds with antimutagenic properties (Kokotkiewicz and Luczkiewics 2009). There is an increasing demand for honeybush production in South Africa, due to increased awareness of the health benefits obtainable from this unique tea (SAHTA 2011).

In this study, the dagger nematodes found in soil around honeybush were identified with a combination of traditional morphological characterization and molecular techniques, based on the D2D3 expansion segment of the 28S gene and the protein-coding cytochrome oxidase (coxI) of the mitochondrial gene.

Methods

Sampling, nematode isolation, and processing

Soil samples were collected from three plots on the honeybush farmland, with five composite samples taken from each plot. Samples were taken from the rhizosphere of the plants, a depth of about 8 cm into the soil. Nematodes were extracted from the soil using a modified Whitehead and Hemming (1965) tray method and examined under a high-power compound microscope. Nematode specimens from a previously identified population of Xiphinema americanum Cobb, 1913 from a grapevine farm in the Western Cape was also included in the study. Nematodes were counted using a stereomicroscope and specimens collected for morphological study, scanning electron microscopy (SEM), and for molecular characterization of nematode species.

Light and scanning electron microscope observations

For light microscopy, nematode specimens were mounted on glass slides and observed under a compound microscope. Morphological characters were measured and light micrographs were taken with a Zeiss Axioskop 40 compound microscope equipped with a drawing tube. Adult females and juveniles were observed. Some of the morphometric features that were measured include total body length, oesophageal length, body diameter, stylet lengths (odontostyle and odontophore), lip region diameter, distance of basal guide ring from anterior, distance from anterior end to the vulva, width at vulva, and the tail length (Table 2). These measurements were used to calculate the characters; a, b, c, c’ and V.

Table 1.
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Primer combination.

Primer code Direction Sequence (5'–3') Amplified gene References
D2A Forward ACA AGT ACC GTG AGG GAA AGT TG 28S rRNA Nunn 1992
D3B Reverse TCG GAA GGA ACC AGC TAC TA Nunn 1992
ITS1 Forward TTGATTACGTCCCTGCCCTTT ITS rRNA Vrain et al. 1992
P28S Reverse TTTCACTCGCCGTTACTAAGG- Vrain et al. 1992
CO1F Forward GATTTTTTGGKCATCCWGARG COI He et al. 2005
CO1R Reverse CWACATAATAAGTATCATG COI
XIPHR1 Reverse ACAATTCCAGTTAATCCTCCTACC COI Lazarova et al. 2006
XIPHR2 Reverse GTACATAATGAAAATGTGCCAC COI Lazarova et al. 2006
Table 2.
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Morphometrical data of Xiphinema oxycaudatum from South Africa. Measurements are in µm, except where stated otherwise, in the form of: mean ± standard deviation (range).

Female Pre-adult Stage before pre-adult
n 11 6 1
L (mm) 1.80 ± 10.52 (1.60–1.94) 1.42 ± 8.79 (1.33–1.52) 128.5
a 46.87 ± 4.37 (39.9–55.3) 37.46 ± 2.90 (33.6–40.9) 42.8
b 6.14 ± 0.56 (4.8–6.9) 4.93 ± 0.78 (3.5–5.7) 5.2
c 50.34 ± 2.96 (45.4–55.3) 37.28 ± 4.48 (29.9–42.2) 37.3
c’ 1.43 ± 0.08 (1.3–1.6) 1.58 ± 0.10 (1.4–1.7) 1.6
V 49.82 ± 1.44 (47.8–52.4) – –
Odontostyle length 78.41 ± 5.12 (71–84) 64.9 ± 2.84 (61–68) 55
Odontophore length 56.14 ± 5.4 (46–66) 47.5 ± 0.84 (47–49) 43
Total stylet length 135.55 ± 5.41 (129.5–149.5) 112 ± 3.33 (111–117) 98
Replacement odontostyle length – 78.78 ± 3.87 (74–85) 59.5
Anterior to guide ring 67.36 ± 2.84 (64–73) 55.5 ± 2.89 (50.5–58–73) 51.5
Tail length 35.82 ± 2.74 (31–41) 37.00 ± 4.70 (31–44.5) 34.5
h (hyaline portion of tail); also J 12.91 ± 1.61 (10.5–15.5) 9.92 ± 1.02 (9–11) 11
h % (hyaline portion/tail length) 36.08 ± 3.85 (29–40.3) 26.93 ± 1.95 (23.7–29) 31.9
Lip region diameter 12.86 ± 0.87 (11.5–13.5) 11.5 ± 0.54 (11–12) 11
Lip region height 5.86 ± 0.32 (5.5–6.5) 5.42 ± 0.38 (5–6) 4.5
Body diameter at guide ring 28.64 ± 1.80 (26–31.5) 25.75 ± 2.95 (23.5–31.5) 24
Body diameter at base of pharynx 36.20 ± 2.52 (33–42) 34.67 ± 4.03 (33–41) 29
Body diameter at vulva or mid-body for juvenile 39.18 ± 2.57 (36.5–44) 37.90 ± 5.19 (31–44) 30
Body diameter at anus 25.18 ± 1.97 (20.5–27.5) 23.42 ± 2.25 (20–26) 21
Body diameter at beginning of hyaline portion of tail 13.50 ± 1.22 (11.5–16) 10.67 ± 0.61 (10–11.5) 9
Pre-rectum length 103.85 ± 47.37 (47–214) 55; 70 –
Rectum length 20.14 ± 4.61 (15–31.5) 23.13 ± 7.49 (17–34) –
Vagina length 14.68 ± 1.01 (12.5–16) – –

Specimen samples for SEM were handpicked, fixed overnight in 2% Glutaraldehyde and dehydrated in increasing concentrations of ethanol. The nematode specimens were chemically dried with Hexamethyldisilizane (HMDS) in a fume hood and kept in a desiccator overnight. Nematodes were mounted on double-sided carbon tapes on Al stubs and were sputter coated with Pd/Au at a thickness of 100Ǻ layer for 10 min.

A Zeiss Merlin FESEM (Carl Zeiss Microscopy, USA) was used to generate electron images at 3kV accelerating voltage using InLens SE and SE2 detection and a probe current of 100–150 pA. Images were captured in TIF format using a pixel averaging noise reduction algorithm.

DNA extraction, PCR, and sequencing

DNA was extracted from single adult female nematodes using a modified method of Nguyen (2007). The polymerase chain reaction (PCR) to confirm the identity of the nematode specie was carried out by the amplification of the internal transcribed spacer (ITS) region, the D2D3 expansion segment of the 28S gene of the ribosomal DNA, and the portion of the cytochrome oxidase (coxI) gene of the mitochondrial DNA. PCR of the ITS region was carried out as described by Chen et al. 2005 using KAPA2G 40 Robust HotStart ReadyMix (KAPA Biosystems) with the primer combination of S-ITS1 (5'-TTGATTACGTCCCTGCCCTTT-3') and 28S (5'-TTTCACTCGCCGTTACTAAGG-3'). Amplification was carried out in a thermal cycler with the following cycling condition; 1 cycle at 94 °C for 4 min, followed by 30 cycles at 94 °C for 30 sec, 52 °C for 30 sec, and 72 °C for 2 min 30 sec, and ending with one cycle at 72 °C for 7 min and finally kept at 4 °C. PCR amplification of the D2-D3 expansion segments of the 28S rDNA gene was carried out with the primer set D2A (5'-ACA AGT ACC GTG AGG GAA AGT TG-3') and D3B (5'-TCG GAA GGA ACC AGC TAC TA-3') with the cycling condition of 4 min at 94 °C, followed by 35 cycles of 1 min at 94 °C, 1 min at 55 °C, and 1 min 30 sec at 72 °C, and a final extension at 72 °C for 10 min (Orlando et al. 2016). The portion of the partial coxI of the mitochondrial gene was amplified using a primer combination of the forward primer, COIF (5'-GATTTTTTGGKCATCCWGARG-3') with the reverse primer, XIPHR2 (5'-GTACATAATGAAAATGTGCCAC-3') as described by Lazarova et al. (2006). The thermal condition includes 1 cycle of 94°C for 1 min, 50 °C for a further 1 min and 72 °C for 2 min. This was followed by 40 cycles of 94 °C for 1 min, 45 °C for 1 min and 72 °C for 2 min. PCR was ended with a final extension phase of 94 °C for 1 min, 45 °C for 1 min and 72 °C for 5 min.

Sequence and phylogenetic analysis

PCR products were purified using the Nucleo-Fast Purification System (Macherey Nagel, Waltham, Massachusetts, USA). Sequencing of the purified DNA was performed in both directions with the Big Dye Terminator V1.3 sequencing kit, followed by the use of electrophoresis on the 3730× 1DNA Analyser (Applied Biosystems) at the DNA Sequencing Unit (Central Analytical Facilities, Stellenbosch University). The Software CLC Main Workbench 7.3 (http://www.clcbio.com) was used for sequence assembly and editing. Newly obtained partial coxI sequences of X. oxycaudatum and X. americanum were deposited on the GenBank database with accession numbers MK211480 and MK956813 respectively. DNA sequences obtained for the D2D3 expansion segment of X. oxycaudatum was also deposited with accession numbers MK947997, MK966417, and MK988554.

The newly obtained DNA sequences were used for BLASTN (Altschul et al. 1997) comparison against GenBank sequences. DNA sequences from the top BLASTN matches, and other nematode sequences, were downloaded from GenBank and aligned using Multiple Alignment using Fast Fourier Transform (MAFTT).

The evolutionary history of the coxI region of the mitochondrial gene and D2D3 expansion segment of the 28S gene was inferred using the maximum parsimony (MP). The most parsimonious tree is shown. Evolutionary analyses were conducted in MEGA X version 10.0.5 (Kumar et al. 2018) and the confidence intervals for the various branching patterns in the trees were measured using bootstraps (Felsenstein 1985) with 1000 replicates. Estimates of the evolutionary divergence between sequences was done using pairwise distance analysis.

Results

Xiphinema oxycaudatum was observed in high numbers from samples taken from the abandoned honeybush farmland with a mean population density of about 510/250 cm3 soil.

Observations with SEM provided detailed information on some intrinsic features of the nematode such as the stirrup-shaped amphidial pouch, slit-like aperture, caudal pores and vagina opening (Fig. 1).

Figure 1. 

Scanning electron micrographs of Xiphinema oxycaudatum A–C head region with stirrup-shaped amphidial pouch and slit-like aperture, vulva opening and tail showing a caudal pore. Scale bars: 2 µm.

The morphological features of the nematodes are similar to those described from Nigeria (Lamberti and Bleve-Zacheo 1979; Bos and Loof 1983). Both adult females and juveniles were observed. The habitus of the nematodes are spiral or C-shaped with a head that is slightly offset. Adult females are between 1600–1800 µm long. They are more ventrally curved at the posterior end than the anterior. The vulva is located slightly above 50% of the body length; the ovary is amphi-didelphic with long oviduct and short uteri. The tail is conoid with bluntly rounded terminus. The juvenile stages are similar to adult females, but with a smaller body size. They also possess more pointed and sharper conoid tails. No male was found.

Description

Female: Body strongly curved ventrally into close C-shape. Cuticle 2.7 µm wide at mid-body, 6.5 µm at dorsal side of tail, radial striations visible on tail end. Lip region demarcated from body by slight depression (Fig. 2). Position of pharyngeal gland nuclei and outlets (as percentage of bulb length): DO = 9.21 (6.5–11); DN = 15.05 (10.1–18.2); DN–DO = 5.83 (3.6–7.3); SN1 = 59.07 (49.3–67.8); SO = 64.54 (49.3–74.3); SN1–SO = 5.42 (0–11); SN2 = 62.86 (59.1–69.3); SN2–SO = 11.25 (5–18.3). Neck region 288.75 ± 20.16 (265–310) µm long; cardia small, hemispherical to conoid in shape. Female reproductive system typical of X. americanum lineage (ovaries with symbionts, long oviducts, short uteri), each branch about two corresponding vulva diameters long. Tail conoid, dorsally convex, ventrally slightly arcuate with rounded terminus, two caudal pores on each lateral side.

Figure 2. 

Light microscopy of Xiphinema oxycaudatum A–D head region, female reproductive system with didelphic ovary, tail region and vulva. Scale bars: 10 µm (A, C, D), 20 µm (B).

Relationship

The specimens from South Africa agree well with the type description of X. oxycaudatum (Table 2) but are slightly longer (1.6–1.94 mm vs 1.5–1.7 mm); the vulva is situated more anterior in one specimen (47.8% vs 51–54%) and have a wider head region (11.5–13.5 µm vs 9–10 µm). However, the South African specimens are closer to the description of X. oxycaudatum from Iran (Fadaei et al. 2003) especially in the body length (1.6–1.9 mm in Iranian specimens) and more anterior position of vulva in some females (45.5–54% in Iranian specimens). The wider head region in the South African specimens are considered to be an intraspecific variation. The pre-adult stage juvenile from South Africa agrees well with the description of this stage described from Iran (Fadaei et al. 2003). One juvenile was found, which apparently falls in a stage before the pre-adult juvenile. It can be distinguished from the pre-adult stage, by the shorter replacement odontostyle (59 µm vs 74–84 µm in pre-adult juvenile). The specimens from South Africa are also near X. peruvianum Lamberti & Bleve-Zacheo, 1979, but can be distinguished by the shorter odontostyle (71–84 µm vs 85–92 µm and the shape of the tail (gradually tapered, conoid vs not so gradually tapered, almost subdigitate).

The phylogenetic relationships within the X. americanum-group species inferred from the analysis of D2D3 expansion segments of 28S and the partial mitochondrial coxI gene using MP are given in Figures 3 and 4 respectively. The D2D3 alignment was 710 base pairs long and included 59 X. americanum-group sequences with two outgroup sequences (X. index and Longidorus crataegi). Phylogenetic analysis of the D2D3 expansion region revealed a high similarity of almost 100% with some species in the americanum-group. Nearly identical sequences were obtained from the studied species, with interspecific divergence ranging from 0 to 0.25%. The MP tree showed two supported clades. Clade I (72%) includes: X. pachtaicum, X. incertum, X. pachydermum, X. parapachydermum, Xiphinema sp., X. simile, X. browni, and other nematode species. Clade II (100%) comprised of X. brevicolle species complex (Orlando et al. 2016): X. citricolum, X. americanum, X. californicum, X. rivesi, X. laevistriatum, and other species. Relationship within this clade was not well resolved. Intra-specific variation with about 2–3 indel events was also observed in the X. oxycaudatum sequences. The genetic relationship of the newly obtained sequences with reference sequences obtained from the National Centre for Biotechnology Information (NCBI) is illustrated in Figure 3.

Figure 3. 

Phylogenetic relationship within species of the Xiphinema americanum-group, based on analysis of the D2D3 regions with maximum parsimony (MP) using Xiphinema index and Longidorus crataegi as outgroups. Newly obtained sequence is indicated by bold letters.

Figure 4. 

Phylogenetic relationship within species of the Xiphinema americanum-group, based on analysis of the coxI regions with maximum parsimony (MP), using Pratylenchus bolivianus and Caenorhabditis elegans as outgroups. Newly obtained sequences are indicated by bold letters.

Species delimitation of X. oxycaudatum within the X. americanum group was achieved by analysing the coxI sequence alignment which comprised of 66 X. americanum group sequences and two other sequences, Pratylenchus bolivianus and Caenorhabditis elegans as outgroups. The alignment length was 298 base pairs long. Although there was no available sequence of the partial coxI gene of X. oxycaudatum on the NCBI database for comparison, the sequence showed a similarity of 86.19% and 82.48% with X. peruvianum and X. rivesi respectively. The pair-wise distance of X. oxycaudatum to the closely related Brazilian population of X. peruvianum is 245 base pairs differences (Table 3). Newly obtained X. americanum sequence showed a high similarity of 98.84% to the South African isolate (AM086690) with only four nucleotide differences. Estimates of the evolutionary divergence between the newly obtained sequence and some closely related ones is shown in Table 3. The number of base differences per sequence from between sequences are indicated.

Table 3.
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Pairwise distances of COI regions between Xiphinema oxycaudatum and some closely related sequences within the Xiphinema americanum group. The number of base differences per sequence from between sequences are shown.

Species 1 2 3 4 5 6 7 8 9 10 11 12 13 14 15 16 17 18 19 20 21 22 23 24 25 26 27 28 29 30 31
1 X._ oxyca udatum_(South_Africa_M K211480)
2 X._rivesi_(USA_Florida_KX263104) 98
3 Xiphinema _sp._(USA_Florida _KX263101) 99 52
4 X._ tarjanense_ (USA_Florida_AM086694) 103 45 32
5 Xiphinema _sp._(lran_MK 202796) 105 56 66 56
6 X._georgianum_(USA_Florida_AM086695) 106 56 65 56 65
7 X._incognitum_(China_AM086705) 107 68 63 58 65 72
8 X._brevicolle_(Russia_KX263107) 107 76 68 62 62 72 55
9 X._rivesi_(Spain_JQ990060) 110 53 47 53 57 75 61 70
10 X._lambertii_ (Czech_Republic_H M163208) 112 77 74 79 72 75 63 62 73
11 X._brevicolle_(Brazil_AM086707) 118 69 70 74 69 81 66 77 77 82
12 X._luci_(Spa in_KY816627) 120 65 70 63 67 63 78 81 61 74 82
13 X._taylori_(Slovakia_AM086703) 120 69 66 70 61 69 71 43 72 71 81 71
14 X._ citricolum_(USA_Florida _AM086693) 122 61 58 59 57 67 68 67 68 71 79 59 73
15 X._florida e_ (USA_Florida_AM086696) 127 69 72 64 72 64 82 81 78 87 85 64 81 63
16 X._rivesi_ (USA_Arkansa s_AM086697) 128 69 70 65 70 66 84 79 74 85 85 62 81 69 6
17 X._diffusum_(China_AM086701) 120 62 65 61 63 67 69 54 67 71 79 76 56 71 88 86
18 X._diffusum_(Brazil_AM086699) 122 63 64 58 62 64 65 50 67 70 79 74 55 71 83 81 11
19 X._asta regiense_(Spain_KP268977) 132 113 108 113 102 116 103 105 116 105 106 112 106 119 122 122 116 116
20 X._simile_(Slova kia_AM086708) 135 94 105 106 84 108 97 102 98 94 108 99 101 97 104 103 101 106 123
21 X._peruvianum_ (Brazil_AM086712) 245 211 212 243 203 247 250 218 230 259 252 233 250 250 250 248 243 245 241 247
22 X._peruvianum_(USA_ Georgia_AM086692) 272 234 241 255 224 265 268 242 254 279 267 258 264 266 269 269 263 266 256 264 72
23 X._america num_(South_Africa_M K956813) 98 48 52 47 57 58 59 58 56 67 74 50 64 32 58 61 58 58 97 94 236 240
24 X._america num_(South_Africa_AM086690) 119 57 59 53 60 64 67 63 62 75 83 56 71 34 67 69 66 63 114 98 248 268 4
25 X. _americanum_(USA_Florida _AM086691) 273 243 244 260 234 284 279 247 266 286 282 256 274 274 272 272 279 277 267 278 260 291 239 276
26 X._america num_ (USA_California _KX263065) 226 238 241 216 229 235 228 239 244 243 239 236 232 228 226 226 233 232 236 233 224 246 205 232 50
27 X._america num_ (USA_California _KX26305 7) 232 247 249 221 235 247 239 245 250 253 248 242 238 236 236 236 243 242 245 239 224 249 213 240 6 47
28 X._america num_(USA_Alabama_K X263058) 244 242 247 226 230 244 242 245 244 259 246 248 243 243 246 244 244 246 245 237 65 33 223 247 271 262 263
29 X._america num_ (USA_California _KX263064) 247 237 243 227 225 245 241 243 245 259 250 249 246 244 247 245 247 249 251 236 63 28 223 248 271 257 256 35
30 X._america num_ (USA_California _KX263060) 250 242 247 232 230 250 248 251 250 265 252 254 249 249 252 250 250 252 250 243 65 34 229 253 274 262 263 0 36
31 X._america num_ (USA_California _KX263063) 253 242 247 235 230 253 251 251 253 268 255 257 252 252 255 253 253 255 252 246 65 35 232 256 277 262 263 0 37 0
32 X._ina equale_ (Czech_Republic_H M163207) 264 249 258 258 233 279 270 259 286 287 278 272 272 265 267 267 269 269 283 270 259 290 241 272 76 69 67 279 281 282 285

Phylogenetic analysis of the aligned sequences revealed five major subclades within the studied americanum-group. They include: X. americanum, X. californicum, Xiphinema sp., X. brevicolle complex, and X. pachtaicum. Xiphinema oxycaudatum was closely related to Xiphinema sp. (Iran) and the Brazilian population of X. peruvianum. Within the 50% majority rule consensus MP tree, no significant difference was obtained in the two closely related species. However, sequences obtained from the coxI mitochondrial gene clearly discriminates X. oxycaudatum from other species within the X. americanum-group. The genetic relationship of this sequence with reference sequences obtained from the NCBI is illustrated in Figure 4.

Discussion

Precise identification of nematode species and knowledge of their distribution is important for effective phytosanitary and management options. Species identification of nematodes within the Xiphinema americanum group is often difficult and complicated due to overlapping of morphological features and phenotypic plasticity. The taxonomy of this group of nematodes is often regarded as controversial and subjective (Luc et al. 1998; Orlando et al. 2016), and there is a possibility to confuse and misidentify species within the group.

Some key morphological features that have been frequently used as diagnostic keys for differentiating between species within the Xiphinema americanum group include the lip region, odontostyle length, position of C, tail shape, and length (Lamberti and Bleve-Zacheo 1979; Lamberti and Carone 1991). However, in more recent times, identification has been done in combination with molecular tools with indications of mitochondrial marker cytochrome oxidase subunit 1 (coxI) as a barcode for species identification and a tool for resolving the complexity in identifying cryptic americanum species (Palomares-Rius et al. 2017).

Although the molecular analysis, based on the D2D3 region of the nematodes species in the present study revealed low interspecific variation in the nematodes within the X. americanum group, two distinct clades were evident from the phylogenetic tree. X. oxycaudatum was separated in a group from other Xiphinema species with a strong statistical support. This was also evident from previous studies where low interspecific variation within the X. americanum-group has been reported (He et al. 2005; Orlando et al. 2016). They indicated that X. americanum-group species formed two highly supported clades, X. americanum and X. pachtaicum (sensu Lamberti and Ciano 1993). Oliveira et al. (2004) also obtained nearly identical result with analysis of the 18 rDNA sequences where species belonging to the X. americanum-group formed a single group separated from the other Xiphinema species. He however suggested that 18S rDNA does not provide a useful marker to discriminate Xiphinema in the americanum group at the species level. This was also confirmed by Zasada et al. (2014), who showed that 18S rDNA sequence data did not provide taxonomic clarity among some populations of X. americanum. In the present study, the sequences obtained from the ITS region were of poor quality and were not used for phylogenetic analysis.

The protein coding mitochondrial gene, cytochrome oxidase subunit I (coxI), has been described as a reliable and preferred molecular barcode and a useful tool for highlighting the intra-specie variation within some species of X. americanum-group (Lazarova et al. 2006; Gutiérrez-Gutiérrez et al. 2012; Lazarova et al. 2016; Orlando et al. 2016; Palomares-Rius et al. 2017). In the present study, coxI gene was used to reconstruct the phylogenetic relationship within the species; thus, in combination with morphological identification, it provided a useful tool for delimitation and discrimination of X. oxycaudatum from other species within the americanum-group.

This study represents the first report of X. oxycaudatum in association with honeybush in South Africa. The South African population is both morphometrically and genetically similar to X. peruvianum. Meza et al. (2011) indicated that a high homology exists between Chile population of X. peruvianum and X. oxycaudatum identified from Taiwan. The South African population are similar to X. peruvianum but are distinguished by their shorter odontostyle and tail shape. This nematode species has been reported in association with a wide range of cultivated plants from Nigeria, Kenya, Iran, Pakistan, Brazil, and Taiwan (Lamberti and Bleve-Zacheo 1979; Bos and Loof 1983; Coomans and Heyns 1997; Fadaei et al. 2003; Oliveira et al. 2003; Chen et al. 2005). Our record of X. oxycaudatum, in association with Cyclopia spp. from South Africa, will add a new record to this list.

Nematodes belonging to the Xiphinema americanum-group are cosmopolitan in their distribution and have phytopathological importance with some species being implicated as vectors of important plant viruses. High numbers of X. oxycaudatum that were recorded from the honeybush farmland in South Africa could have resulted from high multiplication rate of nematodes due to availability of a suitable host, presence of some attractants in the soil, and some edaphic factors. The occurrence of X. oxycaudatum in such high density recorded in this study is disturbing and suggests that a damage potential may exist, which could have future implications on the budding honeybush tea industry.

To our knowledge, this will be the first documented report of the occurrence of X. oxycaudatum in South Africa.

Acknowledgements

The authors would like to thank Chantelle Girgan for her contribution to photography and Rhoda Malgas for her expert advice.

The financial assistance of the Human resources for Industry Programme (THRIP: TP14062571871) and the National Research Foundation (NRF) (grant no: 99679) towards this research is hereby acknowledged. Opinions expressed and conclusions arrived at, are those of the authors and are not necessarily to be attributed to the NRF.

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