Printer Friendly

Development of SCAR primers for PCR assay to detect Diplodia seriata.

1. Introduction

Grapevine decline causes serious economic losses to the wine industry worldwide [1]. Among the numerous fungi associated with grapevine decline, species of Botryosphaeriaceae are dominant [2,3]. They are well known as pathogens, saprophytes, and endophytes on a wide range of woody angiosperm and gymnosperm hosts [4, 5].

Identification of Botryosphaeriaceae spp. based on morphological characteristics remains a difficult task; therefore molecular sequence data and phylogenetic analysis are commonly used to confirm identifications [6-8]. Using these methods numerous species of Botryosphaeriaceae spp. have been identified and associated with grapevine decline worldwide, for instance, Diplodia seriata, D. mutila, Botryosphaeria dothidea, Neofusicoccum parvum, N. mediterraneum, N. australe, N. ribis, N. luteum, Lasiodiplodia theobromae, L. crassipora, D. viticola (Spencermartinsia viticola), Dothiorella sarmentorum, and D. iberica [1,4,5]. The development of restriction digest patterns following PCR amplification of the rDNA region has permitted the identification and detection of some Botryosphaeriaceae spp. [9]. Botryosphaeriaceae spp. were also identified based on sequencing of the ITS region although this sequence was not always sufficient to identify all species and sequences of other genes such as the elongation factor 1-alpha and beta tubulin which were required. These methods require the isolation of the fungi before DNA extraction and continue to be time-consuming and expensive.

Over the last two decades, newly established vineyards in Castilla y Leon (Spain) have shown an increasing percentage of plants with symptoms of wood decline. Research efforts allowed us to analyse grapevine samples from cankered and asymptomatic young and adult plants. Molecular methods were used to confirm the identification of D. seriata, which was one of the most abundant species found [2].

Molecular markers may be helpful in investigating numerous aspects of grapevine decline that still remain unclear, such as disease aetiology, epidemiology, taxonomy of the putative causal agents, and their genetic variability, and in improving diagnostic tools. In particular, random amplified polymorphic DNA (RAPD) markers were largely used for studying genetic variation in species such as Erysiphe graminis [10] and Uncinula necator [11]. RAPD markers were easy to perform and low in cost and no prior knowledge of the genome being investigated was required. RAPD markers also allowed the development of sequence characterised amplified region (SCAR) specific primer pairs, such as was published for Monilinia spp. [12] and Agrobacterium vitis [13]. In the case of grapevine decline Pollastro et al. [14] proposed SCAR primer pairs for the identification of Fomitiporia mediterranea and Phaeomoniella chlamydospora associated with esca and Phomopsis viticola, the causal agent of Phomopsis cane and leaf spot. Lardner et al. [15] published SCAR primers capable of amplifying DNA of Eutypa lata, the main causing agent of Eutypa dieback. The purpose of the present study was to develop SCAR specific primers, which could be used in conventional PCR to detect D. seriata.

2. Materials and Methods

2.1. Sample Analysis and Fungal Isolates. Fungi associated with grapevine decline were obtained from 381 vines. Fifty percent of the isolates were from Castilla y Leon, 47% from other Spanish regions, and 3% from other countries. Seventy-threepercentwere maturevine (>5 years). Sixty-four percent were grapevine branches. External symptoms were esca (22%), Eutypa dieback (34%), Petri disease/black food disease 2%, asymptomatic vines (19%), and others (23%). This study included 47 D. seriata. Fifty-seven isolates of other species were used as controls. Tables 1(a) and 1(b) show the isolates' names and where they were obtained. Eleven cultures were obtained from the Centraalbureau voor Schimmelcultures (CBS Fungal Collection, Utrecht, The Netherlands), Eutypella citricola (810) was a kind gift from Dr. J. Luque (IRTA, Barcelona, Spain). All isolates were grown on potato dextrose agar (PDA) (Merck, Darmstadt, Germany) at 25[degrees]C in darkness. Fungal isolation, morphological and molecular identification, restriction patterns, DNA sequencing, and sequence analysis were done [2].

2.2. Extraction and Purification of DNA. For rapid detection, fungi grapevine genomic DNA was extracted using Redextract-N-Amp plant PCR kit (Sigma, St. Louis, MO, USA) following the manufacturer's instructions.

Genomic DNA was purified from mycelium using the DNeasy plant minikit (QIAGEN, Cologne, Germany). All DNA samples were diluted to a working concentration of 10 ng/[micro]L.

2.3. Development of SCAR Markers

2.3.1. RAPD Amplification. The PCR reaction mix was prepared following the commercial recommendation of Illustra GE Healthcare puReTaq Ready-To-Go PCR Beads (Amersham, Buckinghamshire, UK) supplemented with 1mM of Mg[Cl.sub.2] as described by [16], 0.7 [micro]M of primer, and 50 ng of DNA template in a final volume of 25 [micro]L. The PCR reaction was run according to [17]. Each run included as control a reaction without DNA. Each primer-template combination was tested at least twice. PCR amplifications were performed using a Gene Amp 7200 thermocycler (Applied Biosystems, Foster City, CA, USA) with the primers detailed below. After amplification, the total volume of the reaction of each PCR product was separated by electrophoresis in 1.5% agarose (low EEO, Conda Pronadisa, Madrid, Spain) gels in 1xTAE (Trisacetate-EDTA). After electrophoresis (0.5 V [cm.sup.-1]) the gels were stained with 0.5 [micro]g/mL ethidium bromide, visualized, and photographed using a UV transilluminator. A preselection of the 20 OPERON primers (Operon Technologies, La Jolla, CA, USA) of the OPA, OPD, and OPE series was made using the DNA of 23 isolates of D. seriata, five isolates of D. mutila, three isolates of N. parvum, one isolate of B. dothidea, and one isolate of D. iberica. Primers allowed patterns with distinguishable and reproducible bands to be preselected. Then fragment size and proximity of other bands were additional criteria for selecting the most specific marker for D. seriata. Each RAPD marker was treated and analysed [17].

2.3.2. DNA Cloning. Eleven D. seriata isolates, Napa-c, CBS112555a, Y46-1-1b, Y62-1-1c, Y79-4-3a, Y90-10-1a, Y1034-3a, Y112-24-1a, Y116-10-1c, V14-2a, and R21-1a (Table 1(a)), were used for cloning assays. The selected isolates represented the combination of the most variable geographic origin from our collection and different grapevine ages and included both isolates from both cankers and asymptomatic plants. OPE-20 RAPD markers specific for each isolate were separated by electrophoresis on 1.5% of agarose gel (TAE) and the 1200 bp fragment common to all D. seriata isolates was recovered, eluted, and purified using the commercial Kit GE Healthcare GFX PCR DNA and Gel Band Purification. DNA fragment was cloned by Sistemas Genomicos Agroalimentaria, Paterna, Spain. From each isolate five white/positive colonies of transformed Escherichia coli-DH5a were sequenced. The sequences were then analysed using the CLUSTALW ( program and SCAR primers were designed on the basis of the obtained sequences using

2.4. PCR Amplification Using the SCAR Primers

2.4.1. PCR Specificity. The specificity of each primer pair was tested in amplification tests with purified and/or extracted DNA of 47 D. seriata isolates. Nontargeted DNAs of 57 isolates belonging to fungi associated with grapevine decline from our collection such as twelve Botryosphaeriaceae spp.: D. mutila, B. dothidea, L. theobromae, D. sarmentorum, D. iberica, D. viticola, D. coryli, N. parvum, N. australe, N. mediterraneum, N. luteum, and N. ribis, fourteen other fungi species: P. chlamydospora, Phaeoacremonium aleophilum, Cylindrocarpon macrodidymum, C. liriodendri, C. olidum, C. pauciseptatum, P. viticola, E. lata, Eutypella citricola, Cryptovalsa ampelina, Cadophora luteoolivacea, Fomitiporia mediterranea, Fomitiporella coryophilli, and Stereum hirsutum, isolates of other fungi belonging to the genera of Fusarium, Alternaria, Acremonium, Didymella, Phomopsis, Epicoccum, Psathyrella, Ceratobasidium, and Pestalotia, and Vitis vinifera cvs. Tempranillo and Viura were tested.

The PCR reaction mix was done following the commercial recommendation of Redextract-n-Amp plant PCR kit with the indicated modification: 4 [micro]L of the commercial mix, 0.4 [micro]M of each primer, and 1 [micro]L of template (purified or extracted DNA) in a final volume of 10 [micro]L. PCR reactions were then carried out according to the following basic scheme: the reaction mix was denatured at 95[degrees]C for 5 min, followed by 35 cycles of 30 sec at 94[degrees]C (denaturing), 45 sec at the annealing temperature of 57[degrees]C for DS3.8 S3-DS3.8 R6 or at 60[degrees]C for DS3.8 S3-DS3.8 R4,45 sec at 72[degrees]C (extension), and a final extension phase of 7 min at 72[degrees]C. After amplification, the PCR products were separated by electrophoresis in 1.5% agarose gels in 1xTBE (Tris-borate-EDTA). The gels were stained and visualised as described above.

2.4.2. PCR Sensitivity. The sensitivity of SCAR DS3.8 S3-DS3.8 R6 and DS3.8 S3-DS3.8 R4 primers was ascertained in PCR reactions with D. seriata CBS719.85 and Y207-1-1c. Assays were performed as three independent experiments. The following dilutions of DNA were used as template: 1, 0.1, 0.01, [10.sup.-3], [10.sup.-4], and [10.sup.-5] ng/[micro]L. For these assays only purified DNA-DNeasy QIAGEN-was used.

2.4.3. D. seriata Detection in Infected Wood Samples. Twelve Vitis vinifera (cv. Tempranillo grafted onto 110R-rootstocks) vines were inoculated with each of the D. seriata isolates Y103-4-2a and Y207-1-1c. 00E4 Twelve control plants were inoculated with a sterile agar plug (PDA). For the inoculation a wound was produced in the trunk of the vine, and an agar plug containing or not an actively growing culture of each isolate was placed on the wound and covered with parafilm. All grapevines were maintained in a greenhouse at 20-25[degrees]C. After four months, the D. seriata was reisolated and identified. These fungi could be reisolated 1 cm over the inoculation point and incipient wood symptoms could be observed. The effectiveness of the inoculation was evaluated using the conventional method of fungi isolation [2], consisting of cutting six wood chips (approx. diam. 1-2 mm; approx. length 0.5-1 cm) that were placed on malt extract agar plates-MEA (Merck, Darmstadt, Germany), and incubated at 25[degrees]C in darkness until fungi grew to an extent that could be isolated and placed on PDA plates. As above PDA plates were incubated and grown colonies were morphologically and molecularly identified using the primers pair described in this study (DS3.8 S3-DS3.8 R6 and DS3.8 S3-DS3.8 R4). The inoculated plants used in this study correspond to plants in which the inoculated fungi were isolated and identified from the six wood chips placed on MEA. Three wood chips were cut from four control plants and from four plants infected with each isolate. DNA purification was performed with one chip of each grapevine using the QIAGEN kit as described above. The second chip from each was placed in a tube containing 1mL of malt extract (ME) medium, and the third chip was incubated in 1 mL sterile water. After 2 days at 25[degrees]C in darkness, conventional PCR was performed under the conditions described above with 2 [micro]L of purified DNA, 2 [micro]L of the incubation ME, or 2 [micro]L of the incubation water.

SCAR primers were validated under field conditions. Throughout field prospection eight samples of Vitis vinifera branches were excised from vines exhibiting black dead arm or Eutypa diebacksymptoms. Seven samples were collected in Cigales and Toro (Spain) and one sample came from Portugal. Wood chips were excised from these naturally infected wood samples showing a dark area. Diplodia seriata was detected following the same procedure as described before for inoculated wood: fungi morphological identification, wood chip DNA purification, incubations, and PCR amplifications.

3. Results

Among the numerous species associated with grapevine decline, Botryosphaeriaceae spp. are the dominant with more than 540 isolates obtained from 381 samples. Molecular identification of 127 isolates of Botryosphaeriaceae using restriction patterns and ITS sequencing revealed that 65% of them were D. seriata. Diplodia mutila represented 6% and other species of Botryosphaeriaceae were identified in lesser percentages. All these methods are time-consuming, so, in order to improve the molecular identification, PCR specific primers were developed.

3.1. RAPD Analysis. The high resolution achieved with RAPD enabled the characterisation of intraspecific variation. In an initial screening, primers that provided reproducible patterns were selected; of the 20 primers in each of the OPA, OPD, and OPE kits, seven decamer primers were selected: OPA-2, OPD-2, -8, and -16, OPE-3, -19, and -20 to study single-spore cultures of the 23 selected D. seriata isolates, five D. mutila, three N. parvum, one B. dothidea, and one D. iberica and absence of DNA. Amplification with the selected primers provided 6-15 clear and reproducible bands. The product sizes obtained ranged from approximately 350 to 3000 bp. The combined results for the seven decamer RAPD primers produced 75 markers, generating ten genetically distinct groups of D. seriata isolates (data not shown) that indicated moderate genetic variation among the isolates studied in the present work.


Amplified products with OPE-20 generated four common fragments of about 1900,1200,960, and 795 bp and eight polymorphic fragments of about 2150,1800,1520,1480,1180, 870, 615, and 500 bp for D. seriata. D. mutila isolate gave a different pattern of bands and no band was amplified in absence of DNA template (Figure 1). N. parvum, B. dothidea, and D. iberica gave also different patterns (data not shown).

3.2. PCR Amplification Using the SCAR Primers. Species-specific markers common to all assayed isolates of D. seriata were searched. The OPE20-1200 bp fragment present in D. seriata isolates (indicated by an arrow in Figure 1) was selected. The 1200 bp fragment from eleven different D. seriata isolates (Table 1(a)) was cloned. Five positive colonies from each isolate were sequenced. Four fragments were obtained. A fragment (namely, DS3.8) of 1207 bp was selected. The sequence of the fragment DS3.8 was used to design five primers that were tested in five combinations. Each SCAR-primer pair was tested in an amplification experiment to establish appropriate operative conditions using DNA of D. seriata, D. mutila, B. dothidea, N. parvum, L. theobromae, and D. sarmentorum species present in Castilla y Leon and N. ribis. Afterwards three primers (DS3.8 S3 sense and DS3.8 R6 and DS3.8 R4 reverse) were selected and combined for conventional PCR: DS3.8 S3-DS3.8 R6 and DS3.8 S3-DS3.8 R4 producing 634 bp and 233 bp amplicons, respectively. Primer sequences are shown in Table 2. The experiments made it possible to select two primer pairs in the fragment DS3.8 which yielded the most reproducible results and a single band with strong fluorescence.

3.3. PCR Specificity. Both primer pairs produced a unique band of the expected size (634 bp and 233 bp) for 47 D. seriata isolates using Redextract-N-Amp plant PCR kit (Table 1(a)). No specific fragments were obtained with any of the 57 isolates of 28 species other than D. seriata obtained and identified from symptomatic and asymptomatic grapevines. No specific fragments were obtained when Vitis vinifera was used as the DNA template. Figure 2(a) showed the result of PCR amplification using DS3.8 S3-DS3.8 R4 primers with DNA of nine D. seriata isolates and nine DNA of other species (D. mutila, N. parvum, B. dothidea, L. theobromae, D. sarmentorum, D. iberica, N. luteum, P chlamydospora, and P aleophilum). Figure 2(b) showed the result of PCR amplification using DS3.8 S3-DS3.8 R6 primers with DNA of the same isolates as before.

The specificity of the reaction was implemented using the DNA from other fungal species together (D. mutila, N. parvum, D. sarmentorum, P. aleophilum, P chlamydospora, C. pauciseptatum, and Alternaria sp.) and the DNA of D. seriata: CBS719.85. The PCR conditions established for each primer pair produced only the expected amplicon (data not shown).



3.4. PCR Sensitivity. The PCR efficiency for each primer pair was assayed with D. seriata purified genomic DNA. The 10fold serial dilutions from genomic DNA were prepared from concentrated samples to obtain a broad range of dilutions (1, 0.1, 0.01, [10.sup.-3], [10.sup.-4], and [10.sup.-5] ng/[micro]L). Each dilution was analyzed in triplicate with two different isolates. The serial dilutions of CBS719.85 genomic DNA were represented in Figure 3(a) using DS3.8 S3-DS3.8 R4 primers and Figure 3(b) with DS3.8 S3-DS3.8 R6 primers. A clear band remained visible in lane 5 for primers combination DS3.8 S3-R4 (233 bp) and in line 6 for primer combination DS3.8 S3-R6 (634 bp), establishing the detection limits in 1 pg and 0.1 pg of DNA, respectively.

3.5. Detection ofD. seriata in Wood Samples. DNA purified from wood chips obtained from naturally infected grapevines or from grapevines inoculated with two different D. seriata isolates showed the expected 634 bp and 233 bp fragments using DS3.8 S3-DS3.8 R6 and DS3.8 S3-DS3.8 R4, respectively, for all samples. No amplification was observed with wood inoculated with a PDA plug containing no mycelium (Table 3). These results confirmed the above identification done using conventional methods consisting of the culturing of six wood chips in culture medium for each inoculated plant and morphological identification of the isolated fungi. Positive amplification of D. seriata in 62.5% to 75% of reactions was obtained with wood chips incubated for 2 days in culture medium with no DNA purification (Table 3). Field samples showing BDA and Eutypa dieback symptoms as well as grapevines inoculated with the Y103-4-2a or with Y207-1-1c isolate returned 634 bp and 233 bp fragments using DS3.8 S3-DS3.8 R6 and DS3.8 S3-DS3.8 R4, respectively. A positive reaction was found with three samples for each isolate and BDA symptoms and with two samples of plant showing Eutypa dieback. When incubation was performed in water for 2 days, the amplification result was lower (positive detection in 25% to 37.5% of reactions).

4. Discussion

Morphological identification of Botryosphaeriaceae spp. requires the work of specialists and time until the isolates produce spores that not always allow for the discrimination between genera and/or species. Based on the mycelium aspect, colour and growth on PDA medium 540 isolates from our collection were assigned as different species of the family Botryosphaeriaceae. Spores morphology helps in Botryosphaeriaceae spp. identification. However, nowadays molecular methods facilitate fungi identification. Sequencing and other molecular biology and PCR methods improve fungi identification, as well as studies of epidemiology and phylogeny. The development of restriction digest patterns following PCR amplification of the rDNA region has permitted the identification of some Botryosphaeriaceae spp. [9]. ITS sequence of D. seriata allowed the differentiation among different Botryosphaeriaceae spp. [9,18-20]. However, it has not been possible to apply ITS alone to identify a Botryosphaeriaceae sp. Elongation factor 1-alpha and beta tubulin genes sequences allowed molecular differentiation among Botryosphaeriaceae spp. [21]. Restriction enzymes analyses and sequencing require manipulating the amplified products and increase the risk of contamination. Moreover they are time-consuming and more expensive than a conventional PCR with specific primers that reduce the identification steps in a single reaction.

Using restriction enzymes analyses and ITS sequencing methods the identification of 127 isolates of our collection was confirmed; 65% of them belong to D. seriata species. Preliminary RAPD enabled the characterisation of intraspecific variation of the most abundant Botryosphaeriaceae spp. found in Castilla y Leon grapevines. Taking into account all this information for the confirmation of the identification of the remaining isolates of our collection, SCAR primers were designed following the indication found in [10-14]. An OPE20 RAPD fragment of around 1200 bp was present in all D. seriata isolates and absent in the tested samples of D. mutila, N. parvum, B. dothidea, or D. iberica, so it was cloned. Among the cloned fragments a fragment of 1207 bp was selected and three primers allowed two combinations for conventional PCR. SCAR primers are available for easier identification of D. seriata.

The primers specificity was ascertained with the positive amplification of 47 isolates of D. seriata and the absence of specific fragments amplification with 57 isolates belonging to 28 different species. The sensitivity of the two PCR established the limit of D. seriata detection between 1 and 0.1 pg/[micro]L DNA. The sensitivity of SCAR primers published by Pollastro et al. [14] produced specific band with 0.1-1 ng of the target DNA. The PCR system described here improves and facilitates D. seriata identification. The easy and rapid detection of D. seriata will be an important advantage to guarantee the pathogen-free status of the propagated material in grapevine nurseries. The diagnostic methods described here improve previous techniques. To facilitate the diagnosis and taking into account our previous publication (Martin et al. [22]), wood chip samples were incubated in liquids. These liquids were then used as the DNA template in the PCR. Diplodia seriata PCR provided positive signals in 62.5% to 75% and 25% to 37.5% of the samples incubated in culture medium and water, respectively. To our knowledge, this is the first report of the use of conventional PCR for D. seriata detection in incubation liquid without DNA extraction and without a fungal isolation procedure. All isolates were 100% detected in wood chips after DNA purification by PCR and conventional isolation methods. More investigation is required to confirm these results. Detection of D. seriata without the need for fungal isolation reduces the analysis times to two days and reduces associated costs.

5. Conclusions

Two primer pairs named DS3.8 S3-DS3.8 R6 and DS3.8 S3-DS3.8 R4 were designed to perform a specific amplification of the pathogen D. seriata, one of the most common fungal species associated with grapevine decline. A single product of 634 bp and 233 bp, respectively, was obtained for D. seriata isolates but never from DNA of other 28 fungal species. A high sensitivity of the SCAR primers designed was found. These two conventional PCR were demonstrated to be useful in the specific detection of D. seriata on naturally and artificially infected grapevine wood without fungal isolation. Therefore a new simple, cheap, rapid, and specific diagnostic tool has been described for D. seriata. Moreover, the results of this study can be applied to other woody hosts for which this fungus has been reported as a pathogen.

Conflict of Interests

The authors declare that there is no conflict of interests regarding the publication of this paper.


This work was funded by the Instituto Nacional de Investigacion y Tecnologia Agraria y Alimentarias (INIA RTA2007-07) and by FEDER and CE funds. Laura Martin was supported by Programa Personal Tecnico de Apoyo, Ministerio de Education y Ciencia (PTA-2003-01-01001), and Maria Teresa Martin was supported by Contratos Doctores Sistema INIA-CCAA (37, DR07-0161).


[1] S. Savocchia, C. C. Steel, B. J. Stodart, and A. Somers, "Pathogenicity of Botryosphaeria species isolated from declining grapevines in sub tropical regions of Eastern Australia," Vitis, vol. 46, no. 1, pp. 27-32, 2007.

[2] M. T. Martin and R. Cobos, "Identification of fungi associated with grapevine decline in Castillo y Leon (Spain)," Phytopathologia Mediterranea, vol. 46, no. 1, pp. 18-25, 2007

[3] J. R. Urbez-Torres, P. Adams, J. Kamas, and W. D. Gubler, "Identification, incidence, and pathogenicity of fungal species associated with grapevine dieback in Texas," The American Journal of Enology and Viticulture, vol. 60, no. 4, pp. 497-507, 2009.

[4] J. M. van Niekerk, P. W. Crous, J. Z. Groenewald, P. H. Fourie, and F. Halleen, "DNA phylogeny, morphology and pathogenicity of Botryosphaeria species on grapevines," Mycologia, vol. 96, no. 4, pp. 781-798, 2004.

[5] A. Taylor, G. E. S. J. Hardy, P Wood, and T. Burgess, "Identification and pathogenicity of Botryosphaeria species associated with grapevine decline in Western Australia," Australasian Plant Pathology, vol. 34, no. 2, pp. 187-195, 2005.

[6] P W. Crous, B. Slippers, M. J. Wingfield et al., "Phylogenetic lineages in the Botryosphaeriaceae," Studies in Mycology, vol. 55, pp. 235-253, 2006.

[7] A. J. L. Phillips, P W. Crous, and A. Alves, "Diplodia seriata, the anamorph of "Botryosphaeria" obtusa," Fungal Diversity, vol. 25, pp. 141-155, 2007

[8] J. de Wet, B. Slippers, O. Preisig, B. D. Wingfield, and M. J. Wingfield, "Phylogeny of the Botryosphaeriaceae reveals patterns of host association," Molecular Phylogenetics and Evolution, vol. 46, no. 1, pp. 116-126, 2008.

[9] A. Alves, A. J. L. Phillips, I. Henriques, and A. Correia, "Evaluation of amplified ribosomal DNA restriction analysis as a method for the identification of Botryosphaeria species," FEMS Microbiology Letters, vol. 245, no. 2, pp. 221-229, 2005.

[10] J. M. McDermott, U. Brandle, F. Dutly et al., "Genetic variation in powdery mildew of barley: development of RAPD, SCAR, and VNTR markers," Phytopathology, vol. 84, no. 11, pp. 1316-1321,1994.

[11] C. Delye and M.-F. Corio-Costet, "Origin of primary infections of grape by Uncinula necator: RAPD analysis discriminates two biotypes," Mycological Research, vol. 102, no. 3, pp. 283-288, 1998.

[12] I. Gell, J. Cubero, and P. Melgarejo, "Two different PCR approaches for universal diagnosis of brown rot and identification of Monilinia spp. in stone fruit trees," Journal of Applied Microbiology, vol. 103, no. 6, pp. 2629-2637, 2007

[13] S. H. Lim, J. G. Kim, and H. W. Kang, "Novel SCAR primers for specific and sensitive detection of Agrobacterium vitis strains," Microbiological Research, vol. 164, no. 4, pp. 451-460, 2009.

[14] S. Pollastro, C. Dongiovanni, A. Abbatecola, M. A. de Guido, R. M. de Miccolis Angelini, and F. Faretra, "Specific SCAR primers for fungi associated with wood decay of grapevine," Phytopathologia Mediterranea, vol. 40, no. 3, pp. 362-368, 2001.

[15] R. Lardner, B. E. Stummer, M. R. Sosnowski, and E. S. Scott, "Molecular identification and detection of Eutypa lata in grapevine," Mycological Research, vol. 109, no. 7, pp. 799-808, 2005.

[16] L. Martin, L. E. Saenz de Miera, and M. T. Martin, "AFLP and RAPD characterization of Phaeoacremonium aleophilum associated with Vitis vinifera decline in Spain," Journal of Phytopathology, vol. 162, no. 4, pp. 245-257, 2014.

[17] R. Cobos and M. T. Martin, "Molecular characterisation of Phaeomoniella chlamydospora isolated from grapevines in Castilla y Leon (Spain)," Phytopathologia Mediterranea, vol. 47, no. I, pp. 20-27, 2008.

[18] S. Denman, P. W. Crous, J. E. Taylor, J. Kang, I. Pascoe, and M. J. Wingfield, "An overview of the taxonomic history of Botryosphaeria, and a re-evaluation of its anamorphs based on morphology and ITS rDNa phylogeny," Studies in Mycology, vol. 45, pp. 129-140, 2000.

[19] S. Denman, P. W. Crous, J. Z. Groenewald, B. Slippers, B. D. Wingfield, and M. J. Wingfield, "Circumscription of Botryosphaeria species associated with Proteaceae based on morphology and DNA sequence data," Mycologia, vol. 95, no. 2, pp. 294-307, 2003.

[20] P. A. Barber, T. J. Burgess, G. E. S. J. Hardy, B. Slippers, P. J. Keane, and M. J. Wingfield, "Botryosphaeria species from Eucalyptus in Australia are pleoanamorphic, producing Dichomera synanamorphs in culture," Mycological Research, vol. 109, no. 12, pp. 1347-1363, 2005.

[21] J.-K. Liu, R. Phookamsak, M. Doilom et al., "Towards a natural classification of Botryosphaeriales," Fungal Diversity, vol. 57, no. 1, pp. 149-210, 2012.

[22] M. T. Martin, R. Cobos, L. Martin, and L. Lopez-Enriquez, "Real-Time PCR Detection of Phaeomoniella chlamydospora and Phaeoacremonium aleophilum," Applied and Environmental Microbiology, vol. 78, no. 11, pp. 3985-3991, 2012.

M. T. Martin, M. J. Cuesta, and L. Martin

Instituto Tecnologico Agrario de Castilla y Leon-Zamaduenas, Carretera de Burgos Km 119, 47071 Valladolid, Spain

Correspondence should be addressed to M. T. Martin;

Received 28 April 2014; Revised 8 July 2014; Accepted 9 July 2014; Published 28 September 2014

Academic Editor: Giampiero Vale
TABLE 1: (a) Forty-seven isolates of Diplodia seriata used in this
study. Isolates used in RAPD analysis are shown in bold. Eleven
D. seriata isolates (*) were used for cloning essays. (b) Fifty-seven
isolates used as control in this study. Isolates used in RAPD analysis
are shown in bold.


Species                         Strain              Location

Diplodia seriata              CBS719.85c           New Zealand
D. seriata                     * Napa-c          California, USA
D. seriata                    *CBS112555a           Portugal
D. seriata                     *Y46-1-1b         Cigales, Spain
D. seriata                     Y46-8-1b          Cigales, Spain
D. seriata                     *Y62-1-1c         Arribes, Spain
D. seriata                     Y63-4-1b          Arribes, Spain
D. seriata                     *Y79-4-3a     Ribera del Duero, Spain
D. seriata                     Y84-1-1a            Toro, Spain
D. seriata                     Y87-3-1c          Arribes, Spain
D. seriata                     Y87-8-1a          Arribes, Spain
D. seriata                    *Y90-10-1a         Navarra, Spain
D. seriata                     Y103-3-3b       Extremadura, Spain
D. seriata                    *Y103-4-3a       Extremadura, Spain
D. seriata                     Y111-27-1         Arribes, Spain
D. seriata                    *Y112-24-1a        Arribes, Spain
D. seriata                    *Y116-10-1a        Arribes, Spain
D. seriata                    Y116-27-96         Arribes, Spain
D. seriata                     Y121-15-4         Arribes, Spain
D. seriata                    Y122-44-91         Arribes, Spain
D. seriata                    Y125-12-1b         Arribes, Spain
D. seriata                    Y126-73-91         Arribes, Spain
D. seriata                    Y126-83-91         Arribes, Spain
D. seriata                     Y128-3-1b         Galicia, Spain
D. seriata                     Y161-1-1          Alicante, Spain
D. seriata                     Y163-11-1         Alicante, Spain
D. seriata                    Y163-13-1a         Alicante, Spain
D. seriata                    Y168-21-1b         Alicante, Spain
D. seriata                     Y169-11-1         Alicante, Spain
D. seriata                     Y169-18-1         Alicante, Spain
D. seriata                     Y169-18-2         Alicante, Spain
D. seriata                     Y170-8-1          Alicante, Spain
D. seriata                     Y171-3-1          Alicante, Spain
D. seriata                     Y172-12-1         Alicante, Spain
D. seriata                     Y172-19-3         Alicante, Spain
D. seriata                     Y173-14-1         Alicante, Spain
D. seriata                     Y173-17-1         Alicante, Spain
D. seriata                     Y178-1-1          La Rioja, Spain
D. seriata                    Y178-11-1a         La Rioja, Spain
D. seriata                     Y180-20-1         La Rioja, Spain
D. seriata                     Y181-9-1       Tierra de Leon, Spain
D. seriata                    Y181-13-1b      Tierra de Leon, Spain
D. seriata                     Y181-21-1      Tierra de Leon, Spain
D. seriata                     Y213-8-2c         Cordoba, Spain
D. seriata                    Y221-14-3a          Rueda, Spain
D. seriata                      *V14-2a          Nursery, Spain
D. seriata                      *R21-la          Nursery, Spain


Species                         Strain              Location

Diplodia mutila                CBS431.82         The Netherlands
D. mutila                      Y50-5-1c      Ribera del Duero, Spain
D. mutila                      Y50-7-2b      Ribera del Duero, Spain
D. mutila                      Y60-7-2a       Tierra de Leon, Spain
D. mutila                      Y63-1-1b          Arribes, Spain
D. mutila                      Y113-7-1          Arribes, Spain
D. mutila                     Y117-10-1b         Arribes, Spain
D. mutila                      Y122-10-1         Arribes, Spain
D. mutila                      Y167-9-1          Alicante, Spain
Neofusicoccum parvum          CBS110301a            Portugal
N. parvum                      INIA352c           Madrid, Spain
N. parvum                      Y57-8-1b          Nursery, Spain
N. parvum                      Y91-3-1a          Nursery, Spain
N. parvum                      Y108-9-1        Extremadura, Spain
N. parvum                      Y159-24-1    Castilla La Mancha, Spain
N. parvum                      Y187-8-1      Ribera del Duero, Spain
Botryosphaeria dothidea        Sonoma_c          California, USA
B. dothidea                    CBS110302            Portugal
B. dothidea                    Y264-19-1         Nursery, Spain
Dothiorella iberica            Y51-4-3a      Tierra de Leoon, Spain
D. iberica                      Y81-1-2      Ribera del Duero, Spain
D. iberica                     Y190-3-3      Ribera del Duero, Spain
Dothiorella sarmentorum        CBS120.41             Norway
D. sarmentorum                 Y51-4-3b          Arribes, Spain
D. sarmentorum                 Y262-12-1         Nursery, Spain
Lasiodiplodiatheobromae        CBS110.11               nd
L. theobromae                  Y512-03-1         Nursery, Spain
Neofusicoccum luteum           CBS110299            Portugal
Neofusicoccum australe         Y264-21-1         Nursery, Spain
Phaeoacremonium aleophilum    CBS631.94b              Italy
P. aleophilum                 Y082-02-5c           Toro, Spain
Phaeomoniella chlamydospora    CBS101359              Italy
P. chlamydospora               Y170-03-1         Alicante, Spain
Cylindrocarpon macrodidymum    V049-01c          Nursery, Spain
C. macrodidymum                Y266-10-1         Nursery, Spain
C. liriodendri                Y111-07-2c         Arribes, Spain
C. liriodendri                 Y262-27-1         Nursery, Spain
C. olidum                      Y160-23-2    Castilla La Mancha, Spain
C. olidum                     Y160-57-1a    Castilla La Mancha, Spain
C. olidum                      Y264-22-1         Nursery, Spain
C. pauciseptatum               S018-03-1        Salamanca, Spain
C. pauciseptatum               S020-02-2        Salamanca, Spain
Phomopsis viticola             Y529-07-1         Nursery, Spain
P. viticola                    Y264-17-1         Nursery, Spain
Eutypa lata                    Y249-4-4            Toro, Spain
Fomitiporia mediterranea       Y255-14-1     Ribera del Duero, Spain
Stereum hirsutum               Y112-29-1         Arribes, Spain
Cryptovalsa ampelina           Y231-05-4     Ribera del Duero, Spain
Cadophora luteoolivacea        Y160-56-2    Castilla La Mancha, Spain
Fomitiporella coryophilli      Y234-11-2          Rueda, Spain
D. coryli                      Y291-24-1     Tierra de Leoon, Spain
Eutypella citricola               810           Barcelona, Spain
Fusarium oxysporum             Y239-1-5           Rueda, Spain
Alternaria solani              CBS109157               USA
Acremonium sp.                 Y161-9-2          Alicante, Spain
Epicoccum sp.                  TP32-1C1         Valladolid, Spain
Psathyrella sp.                Y266-4-1          Nursery, Spain

TABLE 2: SCAR primer sequences used in this study for the
conventional PCR detection of Diplodia seriata.

Target           Name          Type                 Sequence

Fragment 3.8   DS3.8 S3   Forward primer   5'-ATCCTCATACTACGGCACGG-3'
               DS3.8 R4   Reverse primer   5'-ccgtagtctcccctttcctc-3'
               DS3.8 R6   Reverse primer    5'-AACGGTGACCCATTCCAC-3'

TABLE 3: Detection of Diplodia seriata in wood chips.

                            Wood chips    Purified DNA

                                          DS3.8 S3-   DS3.8 S3-
                                          DS3.8 R6    DS3.8 R4

Inoculated vines           Y103-4-2a-1        +           +
                           Y103-4-2a-2        +           +
                           Y103-4-2a-3        +           +
                           Y103-4-2a-4        +           +
                           Y207-1-1c-1        +           +
                           Y207-1-1c-2        +           +
                           Y207-1-1c-3        +           +
                           Y207-1-1c-4        +           +
                              PDA-1           -           -
                              PDA-2           -           -
                              PDA-3           -           -
                              PDA-4           -           -
Successful reaction                         100%        100%
Naturally infected vines      BDA-1           +           +
                              BDA-2           +           +
                              BDA-3           +           +
                              BDA-4           +           +
                           E. dieback-1       +           +
                           E. dieback-2       +           +
                           E. dieback-3       +           +
                           E. dieback-4       +           +
Successful reaction                         100%        100%

                            Wood chips    2 days of incubation


                                          DS3.8 S3-   DS3.8 S3-
                                          DS3.8 R6    DS3.8 R4

Inoculated vines           Y103-4-2a-1        +           +
                           Y103-4-2a-2        -           -
                           Y103-4-2a-3        +           +
                           Y103-4-2a-4        +           +
                           Y207-1-1c-1        -           -
                           Y207-1-1c-2        +           +
                           Y207-1-1c-3        +           +
                           Y207-1-1c-4        +           +
                              PDA-1           -           -
                              PDA-2           -           -
                              PDA-3           -           -
                              PDA-4           -           -
Successful reaction                          75%         75%
Naturally infected vines      BDA-1           -           -
                              BDA-2           +           +
                              BDA-3           +           +
                              BDA-4           +           +
                           E. dieback-1       +           +
                           E. dieback-2       +           +
                           E. dieback-3       -           -
                           E. dieback-4       -           -
Successful reaction                         62.5%       62.5%

                            Wood chips    2 days of incubation


                                          DS3.8 S3-   DS3.8 S3-
                                          DS3.8 R6    DS3.8 R4

Inoculated vines           Y103-4-2a-1        -           -
                           Y103-4-2a-2        -           -
                           Y103-4-2a-3        -           -
                           Y103-4-2a-4        -           -
                           Y207-1-1c-1        -           -
                           Y207-1-1c-2        +           +
                           Y207-1-1c-3        +           +
                           Y207-1-1c-4        -           -
                              PDA-1           -           -
                              PDA-2           -           -
                              PDA-3           -           -
                              PDA-4           -           -
Successful reaction                          25%         25%
Naturally infected vines      BDA-1           -           -
                              BDA-2           +           +
                              BDA-3           -           -
                              BDA-4           +           +
                           E. dieback-1       -           -
                           E. dieback-2       +           +
                           E. dieback-3       -           -
                           E. dieback-4       -           -
Successful reaction                         37.5%       37.5%

BDA: black dead arm; E. dieback: Eutypa dieback. +: positive
amplification of the expected fragment, with DS3.8 S3-DS3.8 R6
(634 bp) and with DS3.8 S3-DS3.8 R4 (233bp). -: no amplification.
COPYRIGHT 2014 Hindawi Limited
No portion of this article can be reproduced without the express written permission from the copyright holder.
Copyright 2014 Gale, Cengage Learning. All rights reserved.

Article Details
Printer friendly Cite/link Email Feedback
Title Annotation:Research Article
Author:Martin, M.T.; Cuesta, M.J.; Martin, L.
Publication:International Scholarly Research Notices
Article Type:Report
Geographic Code:4EUSP
Date:Jan 1, 2014
Previous Article:Characteristics of primary cutaneous T-cell lymphoma in Iran: a 10-year retrospective study.
Next Article:Behavioral pattern during dental pain in intellectually disabled children: a comparative study.

Terms of use | Privacy policy | Copyright © 2018 Farlex, Inc. | Feedback | For webmasters