@article{schappe_albornoz_turner_jones_2020, title={Co-occurring Fungal Functional Groups Respond Differently to Tree Neighborhoods and Soil Properties Across Three Tropical Rainforests in Panama}, volume={79}, ISSN={["1432-184X"]}, DOI={10.1007/s00248-019-01446-z}, abstractNote={Abiotic and biotic drivers of co-occurring fungal functional guilds across regional-scale environmental gradients remain poorly understood. We characterized fungal communities using Illumina sequencing from soil cores collected across three Neotropical rainforests in Panama that vary in soil properties and plant community composition. We classified each fungal OTU into different functional guilds, namely plant pathogens, saprotrophs, arbuscular mycorrhizal (AM), or ectomycorrhizal (ECM). We measured soil properties and nutrients within each core and determined the tree community composition and richness around each sampling core. Canonical correspondence analyses showed that soil pH and moisture were shared potential drivers of fungal communities for all guilds. However, partial the Mantel tests showed different strength of responses of fungal guilds to composition of trees and soils. Plant pathogens and saprotrophs were more strongly correlated with soil properties than with tree composition; ECM fungi showed a stronger correlation with tree composition than with soil properties; and AM fungi were correlated with soil properties, but not with trees. In conclusion, we show that co-occurring fungal guilds respond differently to abiotic and biotic environmental factors, depending on their ecological function. This highlights the joint role that abiotic and biotic factors play in determining composition of fungal communities, including those associated with plant hosts.}, number={3}, journal={MICROBIAL ECOLOGY}, author={Schappe, Tyler and Albornoz, Felipe E. and Turner, Benjamin L. and Jones, F. Andrew}, year={2020}, month={Apr}, pages={675–685} }
 @article{thiessen_schappe_zaccaron_conner_koebernick_jacobson_huseth_2020, title={First Report of Cotton Leafroll Dwarf Virus in Cotton Plants Affected by Cotton Leafroll Dwarf Disease in North Carolina}, volume={104}, ISSN={0191-2917 1943-7692}, url={http://dx.doi.org/10.1094/PDIS-02-20-0335-PDN}, DOI={10.1094/PDIS-02-20-0335-PDN}, abstractNote={HomePlant DiseaseVol. 104, No. 12First Report of Cotton Leafroll Dwarf Virus in Cotton Plants Affected by Cotton Leafroll Dwarf Disease in North Carolina PreviousNext DISEASE NOTES OPENOpen Access licenseFirst Report of Cotton Leafroll Dwarf Virus in Cotton Plants Affected by Cotton Leafroll Dwarf Disease in North CarolinaLindsey D. Thiessen, Tyler Schappe, Marcio Zaccaron, Kassie Conner, Jenny Koebernick, Alana Jacobson, and Anders HusethLindsey D. Thiessen†Corresponding author: L. D Thiessen; E-mail Address: ldthiess@ncsu.eduhttp://orcid.org/0000-0001-5029-0139North Carolina State University, Raleigh, NC 27695Search for more papers by this author, Tyler SchappeNorth Carolina State University, Raleigh, NC 27695Search for more papers by this author, Marcio ZaccaronAuburn University, Auburn, AL 36849Search for more papers by this author, Kassie ConnerAlabama Cooperative Extension System, Auburn University, Auburn, AL 36849Search for more papers by this author, Jenny KoebernickAuburn University, Auburn, AL 36849Search for more papers by this author, Alana JacobsonAuburn University, Auburn, AL 36849Search for more papers by this author, and Anders HusethNorth Carolina State University, Raleigh, NC 27695Search for more papers by this author AffiliationsAuthors and Affiliations Lindsey D. Thiessen1 † Tyler Schappe1 Marcio Zaccaron2 Kassie Conner3 Jenny Koebernick2 Alana Jacobson2 Anders Huseth1 1North Carolina State University, Raleigh, NC 27695 2Auburn University, Auburn, AL 36849 3Alabama Cooperative Extension System, Auburn University, Auburn, AL 36849 Published Online:8 Oct 2020https://doi.org/10.1094/PDIS-02-20-0335-PDNAboutSectionsView articlePDFSupplemental ToolsAdd to favoritesDownload CitationsTrack Citations ShareShare onFacebookTwitterLinked InRedditEmailWechat View articleDuring the 2019 growing season, cotton (Gossypium hirsutum L.) plants in North Carolina were observed to have virus-like symptoms including leaf rugosity, leaf curling, and shortened upper internodes, consistent with cotton leafroll dwarf disease (CLRDD) associated with cotton leafroll dwarf virus (CLRDV, family Luteoviridae, genus Polerovirus) (Avelar et al. 2020). Sentinel plots planted on June 17, 2019, at the Sandhills Research Station in Moore County, NC, exhibited CLRDD symptoms, and disease incidence was estimated at 75% on a 0.1-ha field. Cotton aphids (Aphis gossypii Glover), the reported vector of CLRDV (Heilsnis et al. 2020; McLaughlin et al. 2020; Michelotto and Busoli 2007), were detected on plants throughout the growing season. Samples (n = 24) were collected from sentinel plots on September 20, 2019, to test for CLRDV through reverse transcription PCR. Each sample represented five symptomatic plants collected from a single plot. Total RNA was extracted from the petiole tissue of each sample using a Qiagen RNeasy Plant Mini kit (Qiagen, Germantown, MD), following the manufacturer’s recommendations. The cDNA was synthesized using a SuperScript IV first-strand synthesis system (ThermoFisher Scientific, Waltham, MA) and amplified with CLRDV-specific PCR primers CLRDV3675F/Pol3982R (Sharman et al. 2015) targeting a 310-bp genome segment of ORF3-5. Seven CLRDV-positive samples were further amplified with two additional primer sets specifically designed to detect CLRDV: AL674F/AL1407R (Avelar et al. 2019), targeting a 733-bp portion of the ORF0-ORF1, and CLPOF/CLPOR (Cascardo et al. 2015), amplifying an 880-bp fragment spanning the ORF0. Nucleotide BLAST searches showed that the best matches for all sequences in this study were derived from CLRDV with a range of pairwise identity of 99.2 to 100% for all genome segments. From symptomatic samples (n = 14), the isolated virus was confirmed as CLRDV in several cotton varieties, including Deltapine 1646 B2XF (GenBank accessions MN958131 [ORF3-5], MN958147 [ORF0-ORF1], MN958138 [ORF0], MN958133 [ORF3-5], MN958145 [ORF0-ORF1], and MN958140 [ORF0]), Phytogen 480 W3FE (MN958134 [ORF3-5], MN958144 [ORF0-ORF1], and MN958141 [ORF0]), Stoneville 5471 GLTP (MN958135 [ORF3-5], MN958143 [ORF0-ORF1], and MN958142 [ORF0]), and Nextgen 5711 B3XF (MN958130 [ORF3-5], MN958148 [ORF0-ORF1], MN958137 [ORF0], MN958132 [ORF3-5], MN958146 [ORF0-ORF1], MN958139 [ORF0], and MN958136 [ORF3-5]). CLRDD is a newly named disease of cotton in the United States that was first reported in Alabama (Avelar et al. 2019), Georgia (Tabassum et. al. 2019), Mississippi (Aboughanem-Sabanadzovic et. al. 2019), and Texas (Alabi et al. 2020). Although the virus has been reported with variable impacts, losses can be extensive in some fields that are affected (Avelar et al. 2019). North Carolina produced over one million bales of cotton in 2019, and given reported losses among fields with high disease incidence, CLRDV has the potential to significantly reduce cotton yield and quality for the state if it becomes widespread.The author(s) declare no conflict of interest.References:Aboughanem-Sabanadzovic, N., et al. 2019. Plant Dis. 103:1798. https://doi.org/10.1094/PDIS-01-19-0017-PDN Link, ISI, Google ScholarAlabi, O. J., et al. 2020. Plant Dis. 104:998. https://doi.org/10.1094/PDIS-09-19-2008-PDN Link, ISI, Google ScholarAvelar, S., et al. 2019. Plant Dis. 103:592. https://doi.org/10.1094/PDIS-09-18-1550-PDN Link, ISI, Google ScholarAvelar, S., et al. 2020. Plant Dis. 104:780. https://doi.org/10.1094/PDIS-06-19-1316-RE Link, ISI, Google ScholarCascardo, R. S., et al. 2015. Virol. J. 12:123. https://doi.org/10.1186/s12985-015-0356-7 Crossref, ISI, Google ScholarHeilsnis, B., et al. 2020. Proc. Beltwide Cotton Conf., Austin, TX. Google ScholarMcLaughlin, A. K., et al. 2020. Proc. Beltwide Cotton Conf., Austin, TX. Google ScholarMichelotto, M. D., and Busoli, A. C. 2007. Campinas 66:441. Google ScholarSharman, M., et al. 2015. Australas. Plant Dis. Notes 10:24. https://doi.org/10.1007/s13314-015-0174-1 Crossref, ISI, Google ScholarTabassum, A., et al. 2019. Plant Dis. 103:1803. https://doi.org/10.1094/PDIS-12-18-2197-PDN Link, ISI, Google ScholarThe author(s) declare no conflict of interest.DetailsFiguresLiterature CitedRelated Vol. 104, No. 12 December 2020SubscribeISSN:0191-2917e-ISSN:1943-7692 DownloadCaptionUredinia of Phragmidium violaceum on European blackberry (K. J. Evans et al.). Photo credit: L. Morin. Strawberry fruit rot caused by Sclerotinia sclerotiorum (M. V. Marin and N. A. Peres). Photo credit: M. V. Marin. Metrics Downloaded 897 times Article History Issue Date: 1 Dec 2020Published: 8 Oct 2020First Look: 26 Jun 2020Accepted: 23 Jun 2020 Page: 3275 Information© 2020 The American Phytopathological SocietyKeywordscotton leafroll dwarf viruscottonCLRDVviruses and viroidsThe author(s) declare no conflict of interest.PDF downloadCited ByInvestigating the effects of planting date and Aphis gossypii management on reducing the final incidence of cotton leafroll dwarf virusCrop Protection, Vol. 158Complete Genome Sequence of Cotton Leafroll Dwarf Virus Infecting Cotton in Oklahoma, USAMicrobiology Resource Announcements, Vol. 11, No. 7First Report of Cotton Leafroll Dwarf Virus Infecting Hibiscus syriacus in South KoreaDavaajargal Igori, Ah-Young Shin, Se Eun Kim, Suk-Yoon Kwon, and Jae Sun Moon5 February 2022 | Plant Disease, Vol. 0, No. jaCotton Leafroll Dwarf Virus US Genomes Comprise Divergent Subpopulations and Harbor Extensive Variability5 November 2021 | Viruses, Vol. 13, No. 11Effect of Cotton Leafroll Dwarf Virus on Physiological Processes and Yield of Individual Cotton Plants1 October 2021 | Frontiers in Plant Science, Vol. 12Genome analysis of cotton leafroll dwarf virus reveals variability in the silencing suppressor protein, genotypes and genomic recombinants in the USA7 July 2021 | PLOS ONE, Vol. 16, No. 7Natural host range, incidence on overwintering cotton and diversity of cotton leafroll dwarf virus in Georgia USACrop Protection, Vol. 144}, number={12}, journal={Plant Disease}, publisher={Scientific Societies}, author={Thiessen, Lindsey D. and Schappe, Tyler and Zaccaron, Marcio and Conner, Kassie and Koebernick, Jenny and Jacobson, Alana and Huseth, Anders}, year={2020}, month={Dec}, pages={3275} }
 @article{schappe_ritchie_thiessen_2020, title={First Report of Serratia marcescens Causing a Leaf Spot Disease on Industrial Hemp (Cannabis sativa)}, volume={104}, ISBN={1943-7692}, DOI={10.1094/PDIS-04-19-0782-PDN}, abstractNote={In the 2017 and 2018 growing seasons (between May and October), several cultivars of industrial hemp plants grown for flowers in greenhouse production from four North Carolina counties showed symptoms of an angular leaf spot on leaves, stems, and flower parts. Lesions were initially small, dark brown, 1 to 3 mm in size, and vein-limited. As the disease progressed, lesions coalesced to form larger regions of necrosis that engulfed large portions of leaves, and whole plants were lost to disease. Red bacterial ooze was observed streaming from the plant tissues. Bacterial colonies growing on potato dextrose agar (PDA) were raised and dark-pink colored. The Gram stain indicated gram-negative bacilli. A representative isolate (called strain T2) was used to inoculate Cannabis sativa L. ‘Carmagnola’. Two-week-old seedlings (n = 6) were inoculated with a bacterial suspension (OD₆₀₀ = 0.1, approximately 10⁸ CFU/ml) using a PreVal hand sprayer; additional seedlings (n = 6) were inoculated with sterile water to serve as the negative control. Plants were incubated at 23°C for 21 days in a growth chamber with a 12-h photoperiod. After 8 days, dark brown-black lesions similar to those described above were observed on inoculated leaves. Control plants remained symptomless. The pathogen of interest was the only microorganism reisolated from lesions, and after transferring onto PDA, colonies were identical in morphology to those isolated from the original diseased plants. Molecular identification was conducted by first extracting DNA from the representative isolate T2 using the DNeasy Powersoil kit (Qiagen, Hilden, Germany). The 16S ribosomal RNA region (Klindworth et al. 2013) and the RNA polymerase β-subunit (rpoB) gene (Mollet et al. 1997) were PCR amplified. Amplicons were sequenced at the North Carolina State Genomic Sciences Laboratory, and sequences for each gene from the isolate assessed (T2) were deposited to GenBank (accessions MK598699 and MN400982 for 16S rRNA and rpoB, respectively). NCBI-BLAST searches (Altschul et al. 1997) showed the highest similarity (99.6% identity) with 16S rRNA of Serratia marcescens subsp. sakuensis and 99.6% pairwise identity to rpoB of S. marcescens strain B3R3 (GenBank accession KU894791). Based on pathogenicity, morphology, and molecular identification, the unknown bacterial isolate was identified as S. marcescens. Because industrial hemp is increasingly grown across the United States for cannabidiol production, this disease could pose significant challenges and cause yield reduction in affected plants. Additionally, this pathogen could be of human health concern should it survive hemp processing practices, because there are strains that affect humans.}, number={4}, journal={PLANT DISEASE}, author={Schappe, T. and Ritchie, D. F. and Thiessen, L. D.}, year={2020}, month={Apr}, pages={1248–1249} }
 @article{thiessen_schappe_cochran_hicks_post_2020, title={Surveying for Potential Diseases and Abiotic Disorders of Industrial Hemp (Cannabis sativa) Production}, volume={21}, ISSN={["1535-1025"]}, DOI={10.1094/PHP-03-20-0017-RS}, abstractNote={ Industrial hemp (Cannabis sativa L.) has recently been reintroduced as an agricultural commodity in the United States, and, through state-led pilot programs, growers and researchers have been investigating production strategies. Diseases and disorders of industrial hemp in the United States are largely unknowns because record-keeping and taxonomy have improved dramatically in the last several decades. In 2016, North Carolina launched a pilot program to investigate industrial hemp, and diseases and abiotic disorders were surveyed in 2017 and 2018. Producers, consultants, and agricultural extension agents submitted samples to the North Carolina Department of Agriculture and Consumer Services Agronomic Services Division (n = 572) and the North Carolina Plant Disease and Insect Clinic (n = 117). Common field diseases found included Fusarium foliar and flower blights (Fusarium graminearum), Fusarium wilt (Fusarium oxysporum), and Helminthosporium leaf spot (Exserohilum rostratum). Greenhouse diseases were primarily caused by Pythium spp. and Botrytis cinerea. Common environmental disorders were attributed to excessive rainfall flooding roots and poor root development of transplanted clones. }, number={4}, journal={PLANT HEALTH PROGRESS}, author={Thiessen, Lindsey D. and Schappe, Tyler and Cochran, Sarah and Hicks, Kristin and Post, Angela R.}, year={2020}, pages={321–332} }
 @article{thiessen_schappe_2019, title={First Report of Exserohilum rostratum Causing Foliar Blight of Industrial Hemp (Cannabis saliva)}, volume={103}, ISSN={["1943-7692"]}, DOI={10.1094/PDIS-08-18-1434-PDN}, abstractNote={HomePlant DiseaseVol. 103, No. 6First Report of Exserohilum rostratum Causing Foliar Blight of Industrial Hemp (Cannabis sativa) PreviousNext DISEASE NOTES OPENOpen Access licenseFirst Report of Exserohilum rostratum Causing Foliar Blight of Industrial Hemp (Cannabis sativa)L. D. Thiessen and T. SchappeL. D. Thiessen†Corresponding author: L. D. Thiessen; E-mail Address: ldthiess@ncsu.eduNorth Carolina State University, Raleigh, NC, 27695Search for more papers by this author and T. SchappeNorth Carolina State University, Raleigh, NC, 27695Search for more papers by this authorAffiliationsAuthors and Affiliations L. D. Thiessen † T. Schappe North Carolina State University, Raleigh, NC, 27695 Published Online:3 Apr 2019https://doi.org/10.1094/PDIS-08-18-1434-PDNAboutSectionsSupplemental ToolsAdd to favoritesDownload CitationsTrack Citations ShareShare onFacebookTwitterLinked InRedditEmailWechat In the 2017 and 2018 growing seasons (between May and October), industrial hemp plants of several cultivars including those grown for fiber, seed, and flower from numerous counties in North Carolina showed foliar, stem, and floral blight symptoms. Plants were collected from samples submitted to the North Carolina State University Plant Disease and Insect Clinic. Lesions on leaves were round, brown to black, with dark margins. Inside of each lesion, abundant conidia were found. Conidia were rostrate, ellipsoidal to narrowly obclavate, straight or slightly curved, olive-brown, with a protuberant, cylindrical hilum at the base. Conidia were 7 to 12 septate and 75.64 ± 8.31 × 15.61 ± 1.41 µm. Conidiophores were cylindrical, olivaceous-brown with swollen conidiogenous cells containing circular conidial scars. Isolates were obtained by transferring single spores to water agar and then transferring to potato dextrose agar (PDA). On PDA, mycelia were initially white, turning dark brown to black after 2 to 3 days. To fulfill Koch’s postulates, a representative isolate of Exserohilum rostratum (syn. Setospaeria rostrata) was used to inoculate Cannabis sativa L. ‘Carmagnola’. Two-week-old seedlings (n = 6) were inoculated with a conidial suspension (106/ml) using a PreVal hand sprayer, and inoculated seedlings were compared with a water control plant. Plants were incubated at 23°C for 21 days in a growth chamber with a 12-h photoperiod. After 8 days, dark brown lesions were found on inoculated leaves. Lesions were small and varied from 5 mm to 1 cm. After 3 weeks, lesions were surface sterilized in 10% bleach solution for 1 min, rinsed with sterile deionized water, and placed onto PDA. The pathogen of interest was the only microorganism reisolated from lesions, and spores were identical in morphology to those originally isolated. Molecular identification was conducted by first extracting DNA from a representative pure culture using the DNeasy Powersoil kit (Qiagen, Hilden, Germany). The ITS1, 5.8S, and ITS2 regions were amplified via polymerase chain reaction using ITS1f (Gardes and Bruns 1993) and ITS4 (White et al. 1990) primers, and the RPB2 gene was amplified using the bRPB2-6F and bRPB2-7R primers (Matheny 2005). Amplicons were purified using AmpureXP magnetic beads and sequenced using Sanger sequencing at the North Carolina State Genomic Sciences Lab. Forward and reverse raw sequences were trimmed, and a consensus sequence was generated and aligned with ITS and RPB2 sequences of 19 representative isolates of all Setosphaeria species (syn. Exserohilum) in GenBank using MUSCLE (Edgar 2004). A maximum likelihood phylogenetic tree was constructed using PhyML 3.2.2 (Guindon et al. 2010) with 500 bootstrap replicates. In addition, NCBI-BLAST searches (Altschul et al. 1997) of the ITS and RPB2 sequences showed the greatest identity with Setosphaeria longirostrata (99.8% pairwise identity, syn. E. rostratum) and S. rostrata (99.5% pairwise identity, syn. E. rostratum), respectively. Sequence data for ITS1 from the isolate assessed was deposited to GenBank (accession MH779469). Based on the morphological (Seifert and Gams 2011) and molecular identification using three barcoding regions, the fungal isolates were identified as E. rostratum (syn. S. rostrata). As industrial hemp acreage increases in the United States, this disease could limit yield and quality of industrial hemp flower production.The author(s) declare no conflict of interest.References:Altschul, S. F., et al. 1997. Nucleic Acids Res. 25:3389. https://doi.org/10.1093/nar/25.17.3389 Crossref, ISI, Google ScholarEdgar, R. C. 2004. Nucleic Acids Res. 32:1792. https://doi.org/10.1093/nar/gkh340 Crossref, ISI, Google ScholarGardes, M., and Bruns, T. D. 1993. Mol. Ecol. 2:113. https://doi.org/10.1111/j.1365-294X.1993.tb00005.x Crossref, ISI, Google ScholarGuindon, S., et al. 2010. Syst. Biol. 59:307. https://doi.org/10.1093/sysbio/syq010 Crossref, ISI, Google ScholarMatheny, P. B. 2005. Mol. Phylogenet. Evol. 35:1. https://doi.org/10.1016/j.ympev.2004.11.014 Crossref, ISI, Google ScholarSeifert, K. A., and Gams, W. 2011. Persoonia Mol. Phylogeny Evol. Fungi. 27:119. https://doi.org/10.3767/003158511X617435 Crossref, Google ScholarWhite, T. J., et al. 1990. Page 315 in: PCR Protocols: A Guide to Methods and Applications. Academic Press, San Diego, CA. Crossref, Google ScholarThe author(s) declare no conflict of interest.DetailsFiguresLiterature CitedRelated Vol. 103, No. 6 June 2019SubscribeISSN:0191-2917e-ISSN:1943-7692 DownloadCaptionGreen mottle mosaic and leaf deformation symptoms on watermelon (Sui, Li, Shamimuzzaman, Wu, and Ling). Photo credit: K.-S. Ling. Postharvest rot on cucumber caused by Ceratocystis fimbriata (Li, Xu, Zhang, Song, Xie, Sun, and Huang). Photo credit: H. Song. Metrics Article History Issue Date: 6 Jun 2019Published: 3 Apr 2019First Look: 9 Jan 2019Accepted: 7 Jan 2019 Pages: 1414-1414 Information© 2019 The American Phytopathological SocietyThe author(s) declare no conflict of interest.Cited bySetosphaeria rostrata (leaf spot of grasses)CABI Compendium, Vol. CABI CompendiumDieback and Leaf Spot in Box Elder (Acer negundo) Caused by Exserohilum rostratumCheng-long Liu, Xiang-rong Zheng, and Feng-mao Chen9 November 2021 | Plant Disease, Vol. 105, No. 10Molecular Diagnostics and Pathogenesis of Fungal Pathogens on Bast Fiber Crops18 March 2020 | Pathogens, Vol. 9, No. 3Surveying for Potential Diseases and Abiotic Disorders of Industrial Hemp (Cannabis sativa) ProductionLindsey D. Thiessen, Tyler Schappe, Sarah Cochran, Kristin Hicks, and Angela R. Post14 October 2020 | Plant Health Progress, Vol. 21, No. 4Full Issue PDF25 January 2022 | Plant Health Progress, Vol. 21, No. 4}, number={6}, journal={PLANT DISEASE}, author={Thiessen, L. D. and Schappe, T.}, year={2019}, month={Jun}, pages={1414–1414} }