Suchergebnisse

A checklist of world species of Microgastrinae parasitoid wasps (Hymenoptera: Braconidae) is provided. A total of 81 genera and 2,999 extant species are recognized as valid, including 36 nominal species that are currently considered as species inquirendae. Two genera are synonymized under Apanteles. Nine lectotypes are designated. A total of 318 new combinations, three new replacement names, three species name amendments, and seven species status revised are proposed. Additionally, three species names are treated as nomina dubia, and 52 species names are considered as unavailable names (including 14 as nomina nuda). A total of three extinct genera and 12 extinct species are also listed. Unlike in many previous treatments of the subfamily, tribal concepts are judged to be inadequate, so genera are listed alphabetically. Brief diagnoses of all Microgastrinae genera, as understood in this paper, are presented. Illustrations of all extant genera (at least one species per genus, usually more) are included to showcase morphological diversity. Primary types of Microgastrinae are deposited in 108 institutions worldwide, although 76% are concentrated in 17 collections. Localities of primary types, in 138 countries, are reported. Recorded species distributions are listed by biogeographical region and by country. Microgastrine wasps are recorded from all continents except Antarctica; specimens can be found in all major terrestrial ecosystems, from 82°N to 55°S, and from sea level up to at least 4,500 m a.s.l. The Oriental (46) and Neotropical (43) regions have the largest number of genera recorded, whereas the Palaearctic region (28) is the least diverse. Currently, the highest species richness is in the Palearctic region (827), due to more historical study there, followed by the Neotropical (768) and Oriental (752) regions, which are expected to be the most species rich. Based on ratios of Lepidoptera and Microgastrinae species from several areas, the actual world diversity of Microgastrinae is expected to be between 30,000–50,000 species; although these ratios were mostly based on data from temperate areas and thus must be treated with caution, the single tropical area included had a similar ratio to the temperate ones. Almost 45,000 specimens of Microgastrinae from 67 different genera (83% of microgastrine genera) have complete or partial DNA barcode sequences deposited in the Barcode of Life Data System; the DNA barcodes represent 3,545 putative species or Barcode Index Numbers (BINs), as estimated from the molecular data. Information on the number of sequences and BINs per genus are detailed in the checklist. Microgastrinae hosts are here considered to be restricted to Eulepidoptera, i.e., most of the Lepidoptera except for the four most basal superfamilies (Micropterigoidea, Eriocranioidea, Hepialoidea and Nepticuloidea), with all previous literature records of other insect orders and those primitive Lepidoptera lineages being considered incorrect. The following nomenclatural acts are proposed: 1) Two genera are synonymyzed under Apanteles: Cecidobracon Kieffer & Jörgensen, 1910, new synonym and Holcapanteles Cameron, 1905, new synonym; 2) Nine lectotype designations are made for Alphomelon disputabile (Ashmead, 1900), Alphomelon nigriceps (Ashmead, 1900), Cotesia salebrosa (Marshall, 1885), Diolcogaster xanthaspis (Ashmead, 1900), Dolichogenidea ononidis (Marshall, 1889), Glyptapanteles acraeae (Wilkinson, 1932), Glyptapanteles guyanensis (Cameron, 1911), Glyptapanteles militaris (Walsh, 1861), and Pseudapanteles annulicornis Ashmead, 1900; 3) Three new replacement names are a) Diolcogaster aurangabadensis Fernandez-Triana, replacing Diolcogaster indicus (Rao & Chalikwar, 1970) [nec Diolcogaster indicus (Wilkinson, 1927)], b) Dolichogenidea incystatae Fernandez-Triana, replacing Dolichogenidea lobesia Liu & Chen, 2019 [nec Dolichogenidea lobesia Fagan-Jeffries & Austin, 2019], and c) Microplitis vitobiasi Fernandez-Triana, replacing Microplitis variicolor Tobias, 1964 [nec Microplitis varicolor Viereck, 1917]; 4) Three names amended are Apanteles irenecarrilloae Fernandez-Triana, 2014, Cotesia ayerzai (Brèthes, 1920), and Cotesia riverai (Porter, 1916); 5) Seven species have their status revised: Cotesia arctica (Thomson, 1895), Cotesia okamotoi (Watanabe, 1921), Cotesia ukrainica (Tobias, 1986), Dolichogenidea appellator (Telenga, 1949), Dolichogenidea murinanae (Capek & Zwölfer, 1957), Hypomicrogaster acarnas Nixon, 1965, and Nyereria nigricoxis (Wilkinson, 1932); 6) New combinations are given for 318 species: Alloplitis congensis, Alloplitis detractus, Apanteles asphondyliae, Apanteles braziliensis, Apanteles sulciscutis, Choeras aper, Choeras apollion, Choeras daphne, Choeras fomes, Choeras gerontius, Choeras helle, Choeras irates, Choeras libanius, Choeras longiterebrus, Choeras loretta, Choeras recusans, Choeras sordidus, Choeras stenoterga, Choeras superbus, Choeras sylleptae, Choeras vacillatrix, Choeras vacillatropsis, Choeras venilia, Cotesia asavari, Cotesia bactriana, Cotesia bambeytripla, Cotesia berberidis, Cotesia bhairavi, Cotesia biezankoi, Cotesia bifida, Cotesia caligophagus, Cotesia cheesmanae, Cotesia compressithorax, Cotesia delphinensis, Cotesia effrena, Cotesia euphobetri, Cotesia elaeodes, Cotesia endii, Cotesia euthaliae, Cotesia exelastisae, Cotesia hiberniae, Cotesia hyperion, Cotesia hypopygialis, Cotesia hypsipylae, Cotesia jujubae, Cotesia lesbiae, Cotesia levigaster, Cotesia lizeri, Cotesia malevola, Cotesia malshri, Cotesia menezesi, Cotesia muzaffarensis, Cotesia neptisis, Cotesia nycteus, Cotesia oeceticola, Cotesia oppidicola, Cotesia opsiphanis, Cotesia pachkuriae, Cotesia paludicolae, Cotesia parbhanii, Cotesia parvicornis, Cotesia pratapae, Cotesia prozorovi, Cotesia pterophoriphagus, Cotesia radiarytensis, Cotesia rangii, Cotesia riverai, Cotesia ruficoxis, Cotesia senegalensis, Cotesia seyali, Cotesia sphenarchi, Cotesia sphingivora, Cotesia transuta, Cotesia turkestanica, Diolcogaster abengouroui, Diolcogaster agama, Diolcogaster ambositrensis, Diolcogaster anandra, Diolcogaster annulata, Diolcogaster bambeyi, Diolcogaster bicolorina, Diolcogaster cariniger, Diolcogaster cincticornis, Diolcogaster cingulata, Diolcogaster coronata, Diolcogaster coxalis, Diolcogaster dipika, Diolcogaster earina, Diolcogaster epectina, Diolcogaster epectinopsis, Diolcogaster grangeri, Diolcogaster heterocera, Diolcogaster homocera, Diolcogaster indica, Diolcogaster insularis, Diolcogaster kivuana, Diolcogaster mediosulcata, Diolcogaster megaulax, Diolcogaster neglecta, Diolcogaster nigromacula, Diolcogaster palpicolor, Diolcogaster persimilis, Diolcogaster plecopterae, Diolcogaster plutocongoensis, Diolcogaster psilocnema, Diolcogaster rufithorax, Diolcogaster semirufa, Diolcogaster seyrigi, Diolcogaster subtorquata, Diolcogaster sulcata, Diolcogaster torquatiger, Diolcogaster tristiculus, Diolcogaster turneri, Diolcogaster vulcana, Diolcogaster wittei, Distatrix anthedon, Distatrix cerales, Distatrix cuspidalis, Distatrix euproctidis, Distatrix flava, Distatrix geometrivora, Distatrix maia, Distatrix tookei, Distatrix termina, Distatrix simulissima, Dolichogenidea agamedes, Dolichogenidea aluella, Dolichogenidea argiope, Dolichogenidea atreus, Dolichogenidea bakeri, Dolichogenidea basiflava, Dolichogenidea bersa, Dolichogenidea biplagae, Dolichogenidea bisulcata, Dolichogenidea catonix, Dolichogenidea chrysis, Dolichogenidea coffea, Dolichogenidea coretas, Dolichogenidea cyane, Dolichogenidea diaphantus, Dolichogenidea diparopsidis, Dolichogenidea dryas, Dolichogenidea earterus, Dolichogenidea ensiger, Dolichogenidea eros, Dolichogenidea evadne, Dolichogenidea falcator, Dolichogenidea gelechiidivoris, Dolichogenidea gobica, Dolichogenidea hyalinis, Dolichogenidea iriarte, Dolichogenidea lakhaensis, Dolichogenidea lampe, Dolichogenidea laspeyresiella, Dolichogenidea latistigma, Dolichogenidea lebene, Dolichogenidea lucidinervis, Dolichogenidea malacosomae, Dolichogenidea maro, Dolichogenidea mendosae, Dolichogenidea monticola, Dolichogenidea nigra, Dolichogenidea olivierellae, Dolichogenidea parallelis, Dolichogenidea pelopea, Dolichogenidea pelops, Dolichogenidea phaenna, Dolichogenidea pisenor, Dolichogenidea roepkei, Dolichogenidea scabra, Dolichogenidea statius, Dolichogenidea stenotelas, Dolichogenidea striata, Dolichogenidea wittei, Exoryza asotae, Exoryza belippicola, Exoryza hylas, Exoryza megagaster, Exoryza oryzae, Glyptapanteles aggestus, Glyptapanteles agynus, Glyptapanteles aithos, Glyptapanteles amenophis, Glyptapanteles antarctiae, Glyptapanteles anubis, Glyptapanteles arginae, Glyptapanteles argus, Glyptapanteles atylana, Glyptapanteles badgleyi, Glyptapanteles bataviensis, Glyptapanteles bistonis, Glyptapanteles borocerae, Glyptapanteles cacao, Glyptapanteles cadei, Glyptapanteles cinyras, Glyptapanteles eryphanidis, Glyptapanteles euproctisiphagus, Glyptapanteles eutelus, Glyptapanteles fabiae, Glyptapanteles fulvigaster, Glyptapanteles fuscinervis, Glyptapanteles gahinga, Glyptapanteles globatus, Glyptapanteles glyphodes, Glyptapanteles guierae, Glyptapanteles horus, Glyptapanteles intricatus, Glyptapanteles lamprosemae, Glyptapanteles lefevrei, Glyptapanteles leucotretae, Glyptapanteles lissopleurus, Glyptapanteles madecassus, Glyptapanteles marquesi, Glyptapanteles melanotus, Glyptapanteles melissus, Glyptapanteles merope, Glyptapanteles naromae, Glyptapanteles nepitae, Glyptapanteles nigrescens, Glyptapanteles ninus, Glyptapanteles nkuli, Glyptapanteles parasundanus, Glyptapanteles penelope, Glyptapanteles penthocratus, Glyptapanteles philippinensis, Glyptapanteles philocampus, Glyptapanteles phoebe, Glyptapanteles phytometraduplus, Glyptapanteles propylae, Glyptapanteles puera, Glyptapanteles seydeli, Glyptapanteles siderion, Glyptapanteles simus, Glyptapanteles speciosissimus, Glyptapanteles spilosomae, Glyptapanteles subpunctatus, Glyptapanteles thespis, Glyptapanteles thoseae, Glyptapanteles venustus, Glyptapanteles wilkinsoni, Hypomicrogaster samarshalli, Iconella cajani, Iconella detrectans, Iconella jason, Iconella lynceus, Iconella pyrene, Iconella tedanius, Illidops azamgarhensis, Illidops lamprosemae, Illidops trabea, Keylimepie striatus, Microplitis adisurae, Microplitis mexicanus, Neoclarkinella ariadne, Neoclarkinella curvinervus, Neoclarkinella sundana, Nyereria ituriensis, Nyereria nioro, Nyereria proagynus, Nyereria taoi, Nyereria vallatae, Parapanteles aethiopicus, Parapanteles alternatus, Parapanteles aso, Parapanteles atellae, Parapanteles bagicha, Parapanteles cleo, Parapanteles cyclorhaphus, Parapanteles demades, Parapanteles endymion, Parapanteles epiplemicidus, Parapanteles expulsus, Parapanteles fallax, Parapanteles folia, Parapanteles furax, Parapanteles hemitheae, Parapanteles hyposidrae, Parapanteles indicus, Parapanteles javensis, Parapanteles jhaverii, Parapanteles maculipalpis, Parapanteles maynei, Parapanteles neocajani, Parapanteles neohyblaeae, Parapanteles nydia, Parapanteles prosper, Parapanteles prosymna, Parapanteles punctatissimus, Parapanteles regalis, Parapanteles sarpedon, Parapanteles sartamus, Parapanteles scultena, Parapanteles transvaalensis, Parapanteles turri, Parapanteles xanthopholis, Pholetesor acutus, Pholetesor brevivalvatus, Pholetesor extentus, Pholetesor ingenuoides, Pholetesor kuwayamai, Promicrogaster apidanus, Promicrogaster briareus, Promicrogaster conopiae, Promicrogaster emesa, Promicrogaster grandicula, Promicrogaster orsedice, Promicrogaster repleta, Promicrogaster typhon, Sathon bekilyensis, Sathon flavofacialis, Sathon laurae, Sathon mikeno, Sathon ruandanus, Sathon rufotestaceus, Venanides astydamia, Venanides demeter, Venanides parmula, and Venanides symmysta.

A checklist of world species of Microgastrinae parasitoid wasps (Hymenoptera: Braconidae) is provided. A total of 81 genera and 2,999 extant species are recognized as valid, including 36 nominal species that are currently considered as species inquirendae. Two genera are synonymized under Apanteles. Nine lectotypes are designated. A total of 318 new combinations, three new replacement names, three species name amendments, and seven species status revised are proposed. Additionally, three species names are treated as nomina dubia, and 52 species names are considered as unavailable names (including 14 as nomina nuda). A total of three extinct genera and 12 extinct species are also listed. Unlike in many previous treatments of the subfamily, tribal concepts are judged to be inadequate, so genera are listed alphabetically. Brief diagnoses of all Microgastrinae genera, as understood in this paper, are presented. Illustrations of all extant genera (at least one species per genus, usually more) are included to showcase morphological diversity. Primary types of Microgastrinae are deposited in 108 institutions worldwide, although 76% are concentrated in 17 collections. Localities of primary types, in 138 countries, are reported. Recorded species distributions are listed by biogeographical region and by country. Microgastrine wasps are recorded from all continents except Antarctica; specimens can be found in all major terrestrial ecosystems, from 82°N to 55°S, and from sea level up to at least 4,500 m a.s.l. The Oriental (46) and Neotropical (43) regions have the largest number of genera recorded, whereas the Palaearctic region (28) is the least diverse. Currently, the highest species richness is in the Palearctic region (827), due to more historical study there, followed by the Neotropical (768) and Oriental (752) regions, which are expected to be the most species rich. Based on ratios of Lepidoptera and Microgastrinae species from several areas, the actual world diversity of Microgastrinae is expected to be between 30,000–50,000 species; although these ratios were mostly based on data from temperate areas and thus must be treated with caution, the single tropical area included had a similar ratio to the temperate ones. Almost 45,000 specimens of Microgastrinae from 67 different genera (83% of microgastrine genera) have complete or partial DNA barcode sequences deposited in the Barcode of Life Data System; the DNA barcodes represent 3,545 putative species or Barcode Index Numbers (BINs), as estimated from the molecular data. Information on the number of sequences and BINs per genus are detailed in the checklist. Microgastrinae hosts are here considered to be restricted to Eulepidoptera, i.e., most of the Lepidoptera except for the four most basal superfamilies (Micropterigoidea, Eriocranioidea, Hepialoidea and Nepticuloidea), with all previous literature records of other insect orders and those primitive Lepidoptera lineages being considered incorrect. The following nomenclatural acts are proposed: 1) Two genera are synonymyzed under Apanteles: Cecidobracon Kieffer & Jörgensen, 1910, new synonym and Holcapanteles Cameron, 1905, new synonym; 2) Nine lectotype designations are made for Alphomelon disputabile (Ashmead, 1900), Alphomelon nigriceps (Ashmead, 1900), Cotesia salebrosa (Marshall, 1885), Diolcogaster xanthaspis (Ashmead, 1900), Dolichogenidea ononidis (Marshall, 1889), Glyptapanteles acraeae (Wilkinson, 1932), Glyptapanteles guyanensis (Cameron, 1911), Glyptapanteles militaris (Walsh, 1861), and Pseudapanteles annulicornis Ashmead, 1900; 3) Three new replacement names are a) Diolcogaster aurangabadensis Fernandez-Triana, replacing Diolcogaster indicus (Rao & Chalikwar, 1970) [nec Diolcogaster indicus (Wilkinson, 1927)], b) Dolichogenidea incystatae Fernandez-Triana, replacing Dolichogenidea lobesia Liu & Chen, 2019 [nec Dolichogenidea lobesia Fagan-Jeffries & Austin, 2019], and c) Microplitis vitobiasi Fernandez-Triana, replacing Microplitis variicolor Tobias, 1964 [nec Microplitis varicolor Viereck, 1917]; 4) Three names amended are Apanteles irenecarrilloae Fernandez-Triana, 2014, Cotesia ayerzai (Brèthes, 1920), and Cotesia riverai (Porter, 1916); 5) Seven species have their status revised: Cotesia arctica (Thomson, 1895), Cotesia okamotoi (Watanabe, 1921), Cotesia ukrainica (Tobias, 1986), Dolichogenidea appellator (Telenga, 1949), Dolichogenidea murinanae (Capek & Zwölfer, 1957), Hypomicrogaster acarnas Nixon, 1965, and Nyereria nigricoxis (Wilkinson, 1932); 6) New combinations are given for 318 species: Alloplitis congensis, Alloplitis detractus, Apanteles asphondyliae, Apanteles braziliensis, Apanteles sulciscutis, Choeras aper, Choeras apollion, Choeras daphne, Choeras fomes, Choeras gerontius, Choeras helle, Choeras irates, Choeras libanius, Choeras longiterebrus, Choeras loretta, Choeras recusans, Choeras sordidus, Choeras stenoterga, Choeras superbus, Choeras sylleptae, Choeras vacillatrix, Choeras vacillatropsis, Choeras venilia, Cotesia asavari, Cotesia bactriana, Cotesia bambeytripla, Cotesia berberidis, Cotesia bhairavi, Cotesia biezankoi, Cotesia bifida, Cotesia caligophagus, Cotesia cheesmanae, Cotesia compressithorax, Cotesia delphinensis, Cotesia effrena, Cotesia euphobetri, Cotesia elaeodes, Cotesia endii, Cotesia euthaliae, Cotesia exelastisae, Cotesia hiberniae, Cotesia hyperion, Cotesia hypopygialis, Cotesia hypsipylae, Cotesia jujubae, Cotesia lesbiae, Cotesia levigaster, Cotesia lizeri, Cotesia malevola, Cotesia malshri, Cotesia menezesi, Cotesia muzaffarensis, Cotesia neptisis, Cotesia nycteus, Cotesia oeceticola, Cotesia oppidicola, Cotesia opsiphanis, Cotesia pachkuriae, Cotesia paludicolae, Cotesia parbhanii, Cotesia parvicornis, Cotesia pratapae, Cotesia prozorovi, Cotesia pterophoriphagus, Cotesia radiarytensis, Cotesia rangii, Cotesia riverai, Cotesia ruficoxis, Cotesia senegalensis, Cotesia seyali, Cotesia sphenarchi, Cotesia sphingivora, Cotesia transuta, Cotesia turkestanica, Diolcogaster abengouroui, Diolcogaster agama, Diolcogaster ambositrensis, Diolcogaster anandra, Diolcogaster annulata, Diolcogaster bambeyi, Diolcogaster bicolorina, Diolcogaster cariniger, Diolcogaster cincticornis, Diolcogaster cingulata, Diolcogaster coronata, Diolcogaster coxalis, Diolcogaster dipika, Diolcogaster earina, Diolcogaster epectina, Diolcogaster epectinopsis, Diolcogaster grangeri, Diolcogaster heterocera, Diolcogaster homocera, Diolcogaster indica, Diolcogaster insularis, Diolcogaster kivuana, Diolcogaster mediosulcata, Diolcogaster megaulax, Diolcogaster neglecta, Diolcogaster nigromacula, Diolcogaster palpicolor, Diolcogaster persimilis, Diolcogaster plecopterae, Diolcogaster plutocongoensis, Diolcogaster psilocnema, Diolcogaster rufithorax, Diolcogaster semirufa, Diolcogaster seyrigi, Diolcogaster subtorquata, Diolcogaster sulcata, Diolcogaster torquatiger, Diolcogaster tristiculus, Diolcogaster turneri, Diolcogaster vulcana, Diolcogaster wittei, Distatrix anthedon, Distatrix cerales, Distatrix cuspidalis, Distatrix euproctidis, Distatrix flava, Distatrix geometrivora, Distatrix maia, Distatrix tookei, Distatrix termina, Distatrix simulissima, Dolichogenidea agamedes, Dolichogenidea aluella, Dolichogenidea argiope, Dolichogenidea atreus, Dolichogenidea bakeri, Dolichogenidea basiflava, Dolichogenidea bersa, Dolichogenidea biplagae, Dolichogenidea bisulcata, Dolichogenidea catonix, Dolichogenidea chrysis, Dolichogenidea coffea, Dolichogenidea coretas, Dolichogenidea cyane, Dolichogenidea diaphantus, Dolichogenidea diparopsidis, Dolichogenidea dryas, Dolichogenidea earterus, Dolichogenidea ensiger, Dolichogenidea eros, Dolichogenidea evadne, Dolichogenidea falcator, Dolichogenidea gelechiidivoris, Dolichogenidea gobica, Dolichogenidea hyalinis, Dolichogenidea iriarte, Dolichogenidea lakhaensis, Dolichogenidea lampe, Dolichogenidea laspeyresiella, Dolichogenidea latistigma, Dolichogenidea lebene, Dolichogenidea lucidinervis, Dolichogenidea malacosomae, Dolichogenidea maro, Dolichogenidea mendosae, Dolichogenidea monticola, Dolichogenidea nigra, Dolichogenidea olivierellae, Dolichogenidea parallelis, Dolichogenidea pelopea, Dolichogenidea pelops, Dolichogenidea phaenna, Dolichogenidea pisenor, Dolichogenidea roepkei, Dolichogenidea scabra, Dolichogenidea statius, Dolichogenidea stenotelas, Dolichogenidea striata, Dolichogenidea wittei, Exoryza asotae, Exoryza belippicola, Exoryza hylas, Exoryza megagaster, Exoryza oryzae, Glyptapanteles aggestus, Glyptapanteles agynus, Glyptapanteles aithos, Glyptapanteles amenophis, Glyptapanteles antarctiae, Glyptapanteles anubis, Glyptapanteles arginae, Glyptapanteles argus, Glyptapanteles atylana, Glyptapanteles badgleyi, Glyptapanteles bataviensis, Glyptapanteles bistonis, Glyptapanteles borocerae, Glyptapanteles cacao, Glyptapanteles cadei, Glyptapanteles cinyras, Glyptapanteles eryphanidis, Glyptapanteles euproctisiphagus, Glyptapanteles eutelus, Glyptapanteles fabiae, Glyptapanteles fulvigaster, Glyptapanteles fuscinervis, Glyptapanteles gahinga, Glyptapanteles globatus, Glyptapanteles glyphodes, Glyptapanteles guierae, Glyptapanteles horus, Glyptapanteles intricatus, Glyptapanteles lamprosemae, Glyptapanteles lefevrei, Glyptapanteles leucotretae, Glyptapanteles lissopleurus, Glyptapanteles madecassus, Glyptapanteles marquesi, Glyptapanteles melanotus, Glyptapanteles melissus, Glyptapanteles merope, Glyptapanteles naromae, Glyptapanteles nepitae, Glyptapanteles nigrescens, Glyptapanteles ninus, Glyptapanteles nkuli, Glyptapanteles parasundanus, Glyptapanteles penelope, Glyptapanteles penthocratus, Glyptapanteles philippinensis, Glyptapanteles philocampus, Glyptapanteles phoebe, Glyptapanteles phytometraduplus, Glyptapanteles propylae, Glyptapanteles puera, Glyptapanteles seydeli, Glyptapanteles siderion, Glyptapanteles simus, Glyptapanteles speciosissimus, Glyptapanteles spilosomae, Glyptapanteles subpunctatus, Glyptapanteles thespis, Glyptapanteles thoseae, Glyptapanteles venustus, Glyptapanteles wilkinsoni, Hypomicrogaster samarshalli, Iconella cajani, Iconella detrectans, Iconella jason, Iconella lynceus, Iconella pyrene, Iconella tedanius, Illidops azamgarhensis, Illidops lamprosemae, Illidops trabea, Keylimepie striatus, Microplitis adisurae, Microplitis mexicanus, Neoclarkinella ariadne, Neoclarkinella curvinervus, Neoclarkinella sundana, Nyereria ituriensis, Nyereria nioro, Nyereria proagynus, Nyereria taoi, Nyereria vallatae, Parapanteles aethiopicus, Parapanteles alternatus, Parapanteles aso, Parapanteles atellae, Parapanteles bagicha, Parapanteles cleo, Parapanteles cyclorhaphus, Parapanteles demades, Parapanteles endymion, Parapanteles epiplemicidus, Parapanteles expulsus, Parapanteles fallax, Parapanteles folia, Parapanteles furax, Parapanteles hemitheae, Parapanteles hyposidrae, Parapanteles indicus, Parapanteles javensis, Parapanteles jhaverii, Parapanteles maculipalpis, Parapanteles maynei, Parapanteles neocajani, Parapanteles neohyblaeae, Parapanteles nydia, Parapanteles prosper, Parapanteles prosymna, Parapanteles punctatissimus, Parapanteles regalis, Parapanteles sarpedon, Parapanteles sartamus, Parapanteles scultena, Parapanteles transvaalensis, Parapanteles turri, Parapanteles xanthopholis, Pholetesor acutus, Pholetesor brevivalvatus, Pholetesor extentus, Pholetesor ingenuoides, Pholetesor kuwayamai, Promicrogaster apidanus, Promicrogaster briareus, Promicrogaster conopiae, Promicrogaster emesa, Promicrogaster grandicula, Promicrogaster orsedice, Promicrogaster repleta, Promicrogaster typhon, Sathon bekilyensis, Sathon flavofacialis, Sathon laurae, Sathon mikeno, Sathon ruandanus, Sathon rufotestaceus, Venanides astydamia, Venanides demeter, Venanides parmula, and Venanides symmysta.

A checklist of world species of Microgastrinae parasitoid wasps (Hymenoptera: Braconidae) is provided. A total of 81 genera and 2,999 extant species are recognized as valid, including 36 nominal species that are currently considered as species inquirendae. Two genera are synonymized under Apanteles. Nine lectotypes are designated. A total of 318 new combinations, three new replacement names, three species name amendments, and seven species status revised are proposed. Additionally, three species names are treated as nomina dubia, and 52 species names are considered as unavailable names (including 14 as nomina nuda). A total of three extinct genera and 12 extinct species are also listed. Unlike in many previous treatments of the subfamily, tribal concepts are judged to be inadequate, so genera are listed alphabetically. Brief diagnoses of all Microgastrinae genera, as understood in this paper, are presented. Illustrations of all extant genera (at least one species per genus, usually more) are included to showcase morphological diversity. Primary types of Microgastrinae are deposited in 108 institutions worldwide, although 76% are concentrated in 17 collections. Localities of primary types, in 138 countries, are reported. Recorded species distributions are listed by biogeographical region and by country. Microgastrine wasps are recorded from all continents except Antarctica; specimens can be found in all major terrestrial ecosystems, from 82°N to 55°S, and from sea level up to at least 4,500 m a.s.l. The Oriental (46) and Neotropical (43) regions have the largest number of genera recorded, whereas the Palaearctic region (28) is the least diverse. Currently, the highest species richness is in the Palearctic region (827), due to more historical study there, followed by the Neotropical (768) and Oriental (752) regions, which are expected to be the most species rich. Based on ratios of Lepidoptera and Microgastrinae species from several areas, the actual world diversity of Microgastrinae is expected to be between 30,000–50,000 species; although these ratios were mostly based on data from temperate areas and thus must be treated with caution, the single tropical area included had a similar ratio to the temperate ones. Almost 45,000 specimens of Microgastrinae from 67 different genera (83% of microgastrine genera) have complete or partial DNA barcode sequences deposited in the Barcode of Life Data System; the DNA barcodes represent 3,545 putative species or Barcode Index Numbers (BINs), as estimated from the molecular data. Information on the number of sequences and BINs per genus are detailed in the checklist. Microgastrinae hosts are here considered to be restricted to Eulepidoptera, i.e., most of the Lepidoptera except for the four most basal superfamilies (Micropterigoidea, Eriocranioidea, Hepialoidea and Nepticuloidea), with all previous literature records of other insect orders and those primitive Lepidoptera lineages being considered incorrect. The following nomenclatural acts are proposed: 1) Two genera are synonymyzed under Apanteles: Cecidobracon Kieffer & Jörgensen, 1910, new synonym and Holcapanteles Cameron, 1905, new synonym; 2) Nine lectotype designations are made for Alphomelon disputabile (Ashmead, 1900), Alphomelon nigriceps (Ashmead, 1900), Cotesia salebrosa (Marshall, 1885), Diolcogaster xanthaspis (Ashmead, 1900), Dolichogenidea ononidis (Marshall, 1889), Glyptapanteles acraeae (Wilkinson, 1932), Glyptapanteles guyanensis (Cameron, 1911), Glyptapanteles militaris (Walsh, 1861), and Pseudapanteles annulicornis Ashmead, 1900; 3) Three new replacement names are a) Diolcogaster aurangabadensis Fernandez-Triana, replacing Diolcogaster indicus (Rao & Chalikwar, 1970) [nec Diolcogaster indicus (Wilkinson, 1927)], b) Dolichogenidea incystatae Fernandez-Triana, replacing Dolichogenidea lobesia Liu & Chen, 2019 [nec Dolichogenidea lobesia Fagan-Jeffries & Austin, 2019], and c) Microplitis vitobiasi Fernandez-Triana, replacing Microplitis variicolor Tobias, 1964 [nec Microplitis varicolor Viereck, 1917]; 4) Three names amended are Apanteles irenecarrilloae Fernandez-Triana, 2014, Cotesia ayerzai (Brèthes, 1920), and Cotesia riverai (Porter, 1916); 5) Seven species have their status revised: Cotesia arctica (Thomson, 1895), Cotesia okamotoi (Watanabe, 1921), Cotesia ukrainica (Tobias, 1986), Dolichogenidea appellator (Telenga, 1949), Dolichogenidea murinanae (Capek & Zwölfer, 1957), Hypomicrogaster acarnas Nixon, 1965, and Nyereria nigricoxis (Wilkinson, 1932); 6) New combinations are given for 318 species: Alloplitis congensis, Alloplitis detractus, Apanteles asphondyliae, Apanteles braziliensis, Apanteles sulciscutis, Choeras aper, Choeras apollion, Choeras daphne, Choeras fomes, Choeras gerontius, Choeras helle, Choeras irates, Choeras libanius, Choeras longiterebrus, Choeras loretta, Choeras recusans, Choeras sordidus, Choeras stenoterga, Choeras superbus, Choeras sylleptae, Choeras vacillatrix, Choeras vacillatropsis, Choeras venilia, Cotesia asavari, Cotesia bactriana, Cotesia bambeytripla, Cotesia berberidis, Cotesia bhairavi, Cotesia biezankoi, Cotesia bifida, Cotesia caligophagus, Cotesia cheesmanae, Cotesia compressithorax, Cotesia delphinensis, Cotesia effrena, Cotesia euphobetri, Cotesia elaeodes, Cotesia endii, Cotesia euthaliae, Cotesia exelastisae, Cotesia hiberniae, Cotesia hyperion, Cotesia hypopygialis, Cotesia hypsipylae, Cotesia jujubae, Cotesia lesbiae, Cotesia levigaster, Cotesia lizeri, Cotesia malevola, Cotesia malshri, Cotesia menezesi, Cotesia muzaffarensis, Cotesia neptisis, Cotesia nycteus, Cotesia oeceticola, Cotesia oppidicola, Cotesia opsiphanis, Cotesia pachkuriae, Cotesia paludicolae, Cotesia parbhanii, Cotesia parvicornis, Cotesia pratapae, Cotesia prozorovi, Cotesia pterophoriphagus, Cotesia radiarytensis, Cotesia rangii, Cotesia riverai, Cotesia ruficoxis, Cotesia senegalensis, Cotesia seyali, Cotesia sphenarchi, Cotesia sphingivora, Cotesia transuta, Cotesia turkestanica, Diolcogaster abengouroui, Diolcogaster agama, Diolcogaster ambositrensis, Diolcogaster anandra, Diolcogaster annulata, Diolcogaster bambeyi, Diolcogaster bicolorina, Diolcogaster cariniger, Diolcogaster cincticornis, Diolcogaster cingulata, Diolcogaster coronata, Diolcogaster coxalis, Diolcogaster dipika, Diolcogaster earina, Diolcogaster epectina, Diolcogaster epectinopsis, Diolcogaster grangeri, Diolcogaster heterocera, Diolcogaster homocera, Diolcogaster indica, Diolcogaster insularis, Diolcogaster kivuana, Diolcogaster mediosulcata, Diolcogaster megaulax, Diolcogaster neglecta, Diolcogaster nigromacula, Diolcogaster palpicolor, Diolcogaster persimilis, Diolcogaster plecopterae, Diolcogaster plutocongoensis, Diolcogaster psilocnema, Diolcogaster rufithorax, Diolcogaster semirufa, Diolcogaster seyrigi, Diolcogaster subtorquata, Diolcogaster sulcata, Diolcogaster torquatiger, Diolcogaster tristiculus, Diolcogaster turneri, Diolcogaster vulcana, Diolcogaster wittei, Distatrix anthedon, Distatrix cerales, Distatrix cuspidalis, Distatrix euproctidis, Distatrix flava, Distatrix geometrivora, Distatrix maia, Distatrix tookei, Distatrix termina, Distatrix simulissima, Dolichogenidea agamedes, Dolichogenidea aluella, Dolichogenidea argiope, Dolichogenidea atreus, Dolichogenidea bakeri, Dolichogenidea basiflava, Dolichogenidea bersa, Dolichogenidea biplagae, Dolichogenidea bisulcata, Dolichogenidea catonix, Dolichogenidea chrysis, Dolichogenidea coffea, Dolichogenidea coretas, Dolichogenidea cyane, Dolichogenidea diaphantus, Dolichogenidea diparopsidis, Dolichogenidea dryas, Dolichogenidea earterus, Dolichogenidea ensiger, Dolichogenidea eros, Dolichogenidea evadne, Dolichogenidea falcator, Dolichogenidea gelechiidivoris, Dolichogenidea gobica, Dolichogenidea hyalinis, Dolichogenidea iriarte, Dolichogenidea lakhaensis, Dolichogenidea lampe, Dolichogenidea laspeyresiella, Dolichogenidea latistigma, Dolichogenidea lebene, Dolichogenidea lucidinervis, Dolichogenidea malacosomae, Dolichogenidea maro, Dolichogenidea mendosae, Dolichogenidea monticola, Dolichogenidea nigra, Dolichogenidea olivierellae, Dolichogenidea parallelis, Dolichogenidea pelopea, Dolichogenidea pelops, Dolichogenidea phaenna, Dolichogenidea pisenor, Dolichogenidea roepkei, Dolichogenidea scabra, Dolichogenidea statius, Dolichogenidea stenotelas, Dolichogenidea striata, Dolichogenidea wittei, Exoryza asotae, Exoryza belippicola, Exoryza hylas, Exoryza megagaster, Exoryza oryzae, Glyptapanteles aggestus, Glyptapanteles agynus, Glyptapanteles aithos, Glyptapanteles amenophis, Glyptapanteles antarctiae, Glyptapanteles anubis, Glyptapanteles arginae, Glyptapanteles argus, Glyptapanteles atylana, Glyptapanteles badgleyi, Glyptapanteles bataviensis, Glyptapanteles bistonis, Glyptapanteles borocerae, Glyptapanteles cacao, Glyptapanteles cadei, Glyptapanteles cinyras, Glyptapanteles eryphanidis, Glyptapanteles euproctisiphagus, Glyptapanteles eutelus, Glyptapanteles fabiae, Glyptapanteles fulvigaster, Glyptapanteles fuscinervis, Glyptapanteles gahinga, Glyptapanteles globatus, Glyptapanteles glyphodes, Glyptapanteles guierae, Glyptapanteles horus, Glyptapanteles intricatus, Glyptapanteles lamprosemae, Glyptapanteles lefevrei, Glyptapanteles leucotretae, Glyptapanteles lissopleurus, Glyptapanteles madecassus, Glyptapanteles marquesi, Glyptapanteles melanotus, Glyptapanteles melissus, Glyptapanteles merope, Glyptapanteles naromae, Glyptapanteles nepitae, Glyptapanteles nigrescens, Glyptapanteles ninus, Glyptapanteles nkuli, Glyptapanteles parasundanus, Glyptapanteles penelope, Glyptapanteles penthocratus, Glyptapanteles philippinensis, Glyptapanteles philocampus, Glyptapanteles phoebe, Glyptapanteles phytometraduplus, Glyptapanteles propylae, Glyptapanteles puera, Glyptapanteles seydeli, Glyptapanteles siderion, Glyptapanteles simus, Glyptapanteles speciosissimus, Glyptapanteles spilosomae, Glyptapanteles subpunctatus, Glyptapanteles thespis, Glyptapanteles thoseae, Glyptapanteles venustus, Glyptapanteles wilkinsoni, Hypomicrogaster samarshalli, Iconella cajani, Iconella detrectans, Iconella jason, Iconella lynceus, Iconella pyrene, Iconella tedanius, Illidops azamgarhensis, Illidops lamprosemae, Illidops trabea, Keylimepie striatus, Microplitis adisurae, Microplitis mexicanus, Neoclarkinella ariadne, Neoclarkinella curvinervus, Neoclarkinella sundana, Nyereria ituriensis, Nyereria nioro, Nyereria proagynus, Nyereria taoi, Nyereria vallatae, Parapanteles aethiopicus, Parapanteles alternatus, Parapanteles aso, Parapanteles atellae, Parapanteles bagicha, Parapanteles cleo, Parapanteles cyclorhaphus, Parapanteles demades, Parapanteles endymion, Parapanteles epiplemicidus, Parapanteles expulsus, Parapanteles fallax, Parapanteles folia, Parapanteles furax, Parapanteles hemitheae, Parapanteles hyposidrae, Parapanteles indicus, Parapanteles javensis, Parapanteles jhaverii, Parapanteles maculipalpis, Parapanteles maynei, Parapanteles neocajani, Parapanteles neohyblaeae, Parapanteles nydia, Parapanteles prosper, Parapanteles prosymna, Parapanteles punctatissimus, Parapanteles regalis, Parapanteles sarpedon, Parapanteles sartamus, Parapanteles scultena, Parapanteles transvaalensis, Parapanteles turri, Parapanteles xanthopholis, Pholetesor acutus, Pholetesor brevivalvatus, Pholetesor extentus, Pholetesor ingenuoides, Pholetesor kuwayamai, Promicrogaster apidanus, Promicrogaster briareus, Promicrogaster conopiae, Promicrogaster emesa, Promicrogaster grandicula, Promicrogaster orsedice, Promicrogaster repleta, Promicrogaster typhon, Sathon bekilyensis, Sathon flavofacialis, Sathon laurae, Sathon mikeno, Sathon ruandanus, Sathon rufotestaceus, Venanides astydamia, Venanides demeter, Venanides parmula, and Venanides symmysta. ; This is an open access article distributed under the terms of the CC0 Public Domain Dedication. The attached file is the published pdf.

Bovine coccidiosis is caused by protozoa of the genus Eimeria. These protozoa mainly affect young animals, causing a decrease in production and consequent economic losses. The routine diagnosis is made through morphological observation of the oocysts, which has several limitations. The objective of the present study was to develop a qPCR technique for the diagnose of Eimeria spp. in cattle. For this purpose, the 18S rRNA region of the DNA of these parasites was selected, since it is a region with low variability among the species. The qPCR was developed using the SYBR Green, resulting in a PCR with a high sensitivity, able to amplify samples containing only one oocyst of Eimeria spp. of bovines. The feasibility of using qPCR in the diagnosis of the Eimeria Genus is demonstrated in this study, once this technique shows to be less laborious and needs less skills for diagnostic training when compared to the technique conventionally used in theroutine (micromorphometry).

Leishmaniasis is a widespread parasitic disease that occurs as a result of infection with a unicellular parasite belonging to the genus Leishmania. Diagnosis by conventional methods is inaccurate and is not sensitive to confirm the genus infection. Here, we have investigated a methods for Leishmania genus diagnosis, which includes the technique of polymerase chain reaction to detect the presence of the parasite at in vitro for promastigote cultures using three genus-specific primer pairs to amplify HSP70, ITS, and ITS2. The results showed single band of ~1422, ~1020, and ~550 respectively. This study has proved the ability of these primer pairs to detect Leishmania infection and recommend them to be used for detection of leishmaniasis in hospitals and research centers.

13 páginas, 3 figuras, 2 tablas ; Schistosomiasis is a disease of great medical and veterinary importance in tropical and subtropical regions caused by different species of parasitic flatworms of the genus Schistosoma. The emergence of natural hybrids of schistosomes indicate the risk of possible infection to humans and their zoonotic potential, specifically for Schistosoma haematobium and S. bovis. Hybrid schistosomes have the potential to replace existing species, generate new resistances, pathologies and extending host ranges. Hybrids may also confuse the serological, molecular and parasitological diagnosis. Currently, LAMP technology based on detection of nucleic acids is used for detection of many agents, including schistosomes. Here, we evaluate our previously developed species-specific LAMP assays for S. haematobium, S. mansoni, S. bovis and also the genus-specific LAMP for the simultaneous detection of several Schistosoma species against both DNA from pure and, for the first time, S. haematobium x S. bovis hybrids. Proper operation was evaluated with DNA from hybrid schistosomes and with human urine samples artificially contaminated with parasites' DNA. LAMP was performed with and without prior DNA extraction. The genus-specific LAMP properly amplified pure Schistosoma species and different S. haematobium-S. bovis hybrids with different sensitivity. The Schistosoma spp.-LAMP method is potentially adaptable for field diagnosis and disease surveillance in schistosomiasis endemic areas where human infections by schistosome hybrids are increasingly common ; This research was funded by the Institute of Health Carlos III, ISCIII, Spain (www.isciii.es), grants: RICET RD16/0027/0018 (A.M.), PI19/01727 (P.F.-S.), European Union cofinancing by FEDER (Fondo Europeo de Desarrollo Regional) 'Una manera de hacer Europa'. We also acknowledge support by the Predoctoral Fellowship Program of University of Salamanca and cofinancing by Santander Bank, and Predoctoral Fellowship Program of Junta de Castilla y León cofinancing by Fondo Social Europeo ; Peer reviewed

Leishmaniasis, also known as "papalomoyo", is a chronic parasitic infectious disease caused by a flagellated protozoan of the genus Leishmania, which has more than 20 species. Its presentation and clinical manifestations are variable and depend on the species and the immunological status of the host. The most affected populations are children and young adults under 20 years of age. According to its clinical manifestations, it can be divided into the following presentations: cutaneous, visceral, and mucocutaneous, the first of these being the one with the best prognosis. Among the risk factors for this disease are poverty, malnutrition, migration, inadequate housing conditions, and people who perform rural work, like farmers, agriculturists, or military. The diagnosis can be presumptive or definitive, the clinical characteristics of the disease are key for the presumptive diagnosis and the direct smear is the most used laboratory method, its main objective is to achieve the visualization of amastigotes in the clinical sample. Leishmaniasis is known as "the great imitator" since its clinical manifestations are compatible with multiple pathologies, so differential diagnoses must be made with various diseases. The management of this pathology will vary depending on the type of species and the resistances present. ; La leishmaniosis también conocida como "papalomoyo" es una enfermedad infecciosa crónica parasitaria causada por un protozoo flagelado del género Leishmania, el cual cuenta con más de 20 especies. Su presentación y manifestaciones clínicas son variables, y dependen de la especie y el estado inmunológico del huésped. La población más afectada son los niños y los adultos jóvenes menores de 20 años. Según sus manifestaciones clínicas se puede dividir en: cutánea, visceral y mucocutánea, siendo la de mejor pronóstico la primera de estas. Dentro de los factores de riesgo para esta enfermedad se encuentra: pobreza, desnutrición, migración, condiciones de vivienda inadecuadas y personas que realizan trabajos rurales, como agricultores, granjeros o militares. El diagnóstico puede ser presuntivo o definitivo, las características clínicas de la enfermedad son clave para el diagnóstico presuntivo y el frotis directo es el método de laboratorio más utilizado, cuyo principal objetivo es lograr la visualización de amastigotes en la muestra clínica. La leishmaniosis es conocida como "la gran imitadora" ya que su clínica es compatible con diversas patologías, por lo que debe realizarse diagnóstico diferencial con varias enfermedades. El manejo de dicha patología va a variar dependiendo del tipo de especie y las resistencias presentes.

Aquaculture is one of the sectors of animal husbandry with the fastest growth rate. However, the increase in the sector's production chain without proper management can result in factors that favor the development of diseases, especially infectious diseases caused by bacteria. Many factors, such as agriculture or industry resides, improper use of antibiotics in animals or humans, have contributed to increased environmental pressure and the appearance of antibiotic-resistant bacteria, while residues from these drugs can remain in the carcasses and in water a risk to public and environmental health. From that, we identified the bacterial genus/species and their bacterial resistance to antibiotics from samples received from fish disease outbreaks for bacteriosis diagnosis between January 2017 and October 2020. Isolated bacteria were subjected to the Kirby and Bauer sensitivity test for five classes of antibiotics (penicillins, fluoroquinolones, aminoglycosides, amphenicols, and tetracyclines). Of the 181 analyzed outbreaks, 232 bacteria were isolated, including Streptococcus spp., Aeromonas spp., Edwardsiella spp., Plesiomonas shigelloides, Pseudomonas aeruginosa, Chromobacterium violaceum, Flavobacterium spp., Citrobacter spp., Enterococcus spp., Vibrio spp., Enterobacter spp., Chryseobacterium meningosepticum. Of the 232 bacteria, 40 strains were classified as multidrug resistant (MDR), with Plesiomonas shigelloides, Aeromonas spp., and Edwardsiella spp. representing more than half of this number (22/total). With several bacteria demonstrating resistance to Brazilian aquaculture-legalized drugs (tetracycline and florfenicol), it is mandatory to research, not only for alternatives to the use of antibiotics, but also for other drugs effective against the main circulating bacterial pathogens. In addition, vigilance over the occurrence of resistant bacteria is necessary, considering the appearance of zoonotic bacteria with multi-resistant characteristics, becoming a public health concern.

The newly recorded genus and species to China, Harpagoxenus sublaevis (Nylander), is reported from Da Hinggan Ling, northeastern China. Diagnosis of the genus and description of the species are provided based on a Chinese specimen. A key to the 3 known species of the genus of the world is prepared based on the worker caste.

Possibility of Using Cutover Peat Bogs in Bioindication of Environmental State / Elena S. Novoselova, Lyudmila N. Shikhova, and Eugene M. Lisitsyn -- Paleopalinology Studies of Conditions of Peatlands Formation on European Northeast of Russia / Ksenya A. Zubkova, Lyudmila N. Shikhova, and Eugene M. Lisitsyn -- Use of Artemia salina Biomarkers for the Evaluation of the Effect of Static Magnetic Fields / Irina I. Rudneva and Valentin G. Shaida -- Theoretical and Applied Aspects of Mutations Induction for Improving Agricultural Plants / Nina A. Bome, Larissa I. Weisfeld, Natalia N. Kolokolova, Nikolay V. Tetyannikov, Maral U. Utebayev, and Alexander Y. Bome -- Enzymatic Activity of Bacteria Bacillus subtilis: Assessment Using Phosphemidum / Irina V. Pak, Oleg V. Trofimov, Larissa I. Weisfeld, and Rizvan D. Rustamov -- Cytogenetic Characteristics of Seed Seedlings of Rhododendron ledebourii, Introduced in the Botanical Garden of Voronezh State University / Tatyana V. Vosrikova, Juliya V. Burmenko, and Vladislav N. Kalaev -- Anthropogenic Pollution Influence on the Antioxidant Activity in Leaves and on the Cytogenic Structures in the Seedlings of the Representatives of the Rhododendron Genus / Tatyana V. Vosrikova, Juliya V. Burmenko, Vladislav N. Kalaev, and Vladimir N. Sorokopudov -- Cytogenetic Indices, Germination Ability, and Content of Total Protein in Seed Progeny of Betula pendula from Various Areas of Voronezh City with Different Levels of Anthropogenic Pressure / Tatyana V. Vostrikova, Olga A. Zemlyanukhina, and Vladislav N. Kalaev -- Photoindication of Plant Nitrogen Nutrition / Rafail A. Afanas'ev, Genrietta E. Merzlaya, and Michail O. Smirnov -- Revegetation and Launching Self-Restoration Process of the Disturbed Landscape Along the Transport Corridor in Western Siberia / Nina A. Bome, Nikolai G. Ivanov, Marina V. Semenova, Lee A. Newman, and Alexander Y. BOME -- Pigment Content in Plant Leaves as a Bio-Indicator of Adaptability to Growing Conditions / Eugene M. Lisitsyn -- Some Indirect Methods for Predicting the Rooting Ability of Apple Tree (Malus spp) Stem Cuttings / Olga A. Opalko and Anatoly Iv. Opalko.

The genus Capripoxvirus of the family Poxviridae consists of the species lumpy skin disease virus, sheeppox virus and goatpox virus that affect cattle, sheep and goats, respectively. Whereas lumpy skin disease virus (LSDV) is transmitted mainly mechanically via blood-feeding insects and possibly hard ticks, the major transmission routes of sheeppox virus (SPPV) and goatpox virus (GTPV) are via direct contact and aerosols. Affected animals develop fever and display clinical signs such as ocular and nasal discharge, lymphadenopathy and characteristic lesions of the skin. Severe clinical course, especially in combination with respiratory signs, can result in the death of the affected animals. In endemic regions, mortality of capripox virus-induced diseases is low (1-10%). However, mortalities of up to 75% have been reported for LSDV and up to 100% for SPPV and GTPV in exotic breeds and high-producing dairy or beef animals. The loss of quality of the leather, reduced weight gain and milk yield as well as complete loss of affected animals have severe impact on national and global economies. Therefore, capripox virus-induced diseases have significant impact on both the affected individual animal as well as on the existence of small-scale farmers and large agricultural enterprises. However, until now, only live attenuated vaccines are commercially available. These attenuated vaccines are not authorized in the European Union and their administration would comprise the disease-free status of the respective country. Thus, reliable diagnostic tools for the detection and characterization of capripox viruses as well as safe and efficient control measures are of high importance. The objectives of the present thesis were the development, validation and comparison of diagnostic tools, the establishment of challenge infection models and the performance of pathogenesis studies for all three capripox virus species, and the development and testing of different inactivated prototype vaccine candidates against LSDV. First, new real-time quantitative polymerase chain reaction (qPCR) assays for robust detection and differentiation of LSDV field strains, LSDV vaccine strains, SPPV and GTPV were developed and extensively validated. In the following, two single assays were combined to duplex assays, one for the differentiation between LSDV field strains and LSDV vaccine strains, and the second for discrimination of SPPV and GTPV. Finally, a diagnostic workflow based on these new duplex assays in combination with already published methods was established. This workflow enables time-saving, robust and reliable detection, species-specific identification and genetic and phylogenetic characterization of all three capripox virus species. In addition, already existing serological examination methods (serum neutralization assay and commercial enzyme-linked immunosorbent assay) were compared regarding their sensitivity and specificity. Furthermore, pathogenesis studies with different capripox virus isolates were performed in the respective target species, and the suitability of selected virus isolates as challenge viruses for future vaccine studies was analyzed. Pathogenesis studies with isolates GTPV-"V/103" and LSDV-"Macedonia2016" revealed that both are proper candidates for challenge models. Finally, three different SPPV isolates (SPPV-"V/104", SPPV-"India/2013/Surankote" and SPPV-"Egypt/2018") were tested in sheep regarding their virulence to find a suitable challenge model for SPPV, and SPPV-"India/2013/Surankote" was chosen for future vaccine studies. Once appropriate challenge models were established, different inactivated prototype vaccines against LSDV were developed, and vaccine safety as well as vaccine efficacy were tested in cattle. Eventually, a Polygen-adjuvanted inactivated LSDV-vaccine candidate was selected that is able to fully prevent cattle from any LSDV-related clinical signs after severe challenge infection. Furthermore, molecular and serological data indicate that this inactivated prototype vaccine is even able to induce a kind of "sterile immunity" against LSDV in those cattle. It has to be mentioned that a commercially available vaccine similar to this prototype vaccine would be a great advance for the control of LSDV. In the future, additional studies addressing diagnostics and optimized control of capripox viruses should be performed. Firstly, probe-based real-time qPCR assays for the differentiation of SPPV and GTPV vaccine strains from their respective virulent field strains should be developed and included into the diagnostic workflow. Secondly, further tests of the inactivated prototype vaccine, e.g. determination of the minimum protective dose and the possibility of cross-protection in sheep and goats against SPPV and GTPV, respectively, should be performed. ; Die Gattung Capripoxvirus beinhaltet das Virus der Lumpy-Skin-Krankheit (LSDV), das Schafpockenvirus (SPPV) und das Ziegenpockenvirus (GTPV), die hauptsächlich Rinder bzw. Schafe und Ziegen infizieren. Während LSDV vorwiegend mechanisch über blutsaugende Vektoren und möglicherweise über Schildzecken übertragen wird, sind der direkte Kontakt sowie die Aerosoltransmission als Hauptübertragungsrouten für SPPV und GTPV beschrieben. Betroffene Tiere entwickeln Fieber und zeigen klinische Anzeichen wie z.B. okularen und nasalen Ausfluss, Lymphadenopathie und charakteristische Hautläsionen. Schwere Krankheitsverläufe, insbesondere in Verbindung mit respiratorischen Symptomen, können für die infizierten Tiere zum Tod führen. In endemischen Gebieten ist die Mortalität Capripockenvirus-induzierter Erkrankungen relativ gering (1-10%). In exotischen Rassen oder in Tieren, die auf Hochleistung (zum Beispiel Milch- oder Fleischrassen) gezüchtet wurden, kann die Mortalität von LSDV bis zu 75% und die Mortalität von SPPV und GTPV bis zu 100% betragen. Der aus den Hautläsionen resultierende Qualitätsverlust des Leders, reduzierte Gewichtszunahme und reduzierte Milchleistung sowie der Verlust betroffener Tiere führen zu Umsatzeinbußen und beeinflussen dadurch sowohl die nationale als auch die globale Wirtschaft. Dadurch haben Capripockenvirus-induzierte Erkrankungen nicht nur einen erheblichen Einfluss auf das infizierte Einzeltier, sondern auch auf kleine Familienunternehmen und landwirtschaftliche Großbetriebe. Derzeit sind zur Prophylaxe lediglich attenuierte Lebendvakzinen kommerziell erhältlich. Diese sind in der Europäischen Union jedoch nicht zugelassen, da ihr Einsatz den Verlust des Status "Capripocken-frei" für das jeweilige Land bedeutet. Aus diesen Gründen werden dringend sowohl zuverlässige und zeitsparende Diagnostikmethoden für die Detektion und Charakterisierung von Capripocken, als auch sichere und effiziente Kontrollmaßnahmen benötigt. Ziele dieser Arbeit waren die Entwicklung, Validierung und vergleichende Analyse verschiedener diagnostischer Methoden, die Durchführung von Pathogenesestudien zur Etablierung von Infektionsmodellen für alle drei Capripockenviren und die Entwicklung und Testung verschiedener inaktivierter Prototypvakzinen gegen das LSDV. Im Laufe dieser Arbeit wurden neue real-time quantitative Polymerasekettenreaktion (qPCR)-Assays für eine robuste Detektion und Differenzierung zwischen LSDV-Feldstämmen, LSDV-Vakzinestämmen, SPPV und GTPV entwickelt und umfassend validiert. Im Anschluss wurden jeweils zwei dieser Einzelassays zu sogenannten Duplex-Assays kombiniert. Der erste Duplex-Assay ist in der Lage, zwischen LSDV-Feldstämmen und LSDV-Vakzinestämmen zu unterschieden, der zweite Duplex-Assay erlaubt die Differenzierung zwischen SPPV und GTPV. Schließlich wurde ein diagnostischer Workflow basierend auf den beiden neuen Duplex-Assays in Kombination mit bereits publizierten Methoden etabliert. Dieser ermöglicht eine zeitsparende, robuste und zuverlässige Detektion, Spezies-spezifische Identifizierung und genetische sowie phylogenetische Charakterisierung der drei Capripockenvirusspezies. Zudem wurden bereits vorhandene serologische Diagnostikmethoden (der Serumneutralisationstest und ein kommerziell erhältlicher ELISA) hinsichtlich ihrer Sensitivität und ihrer Spezifität verglichen. Des Weiteren wurden Pathogenesestudien mit verschiedenen Capripockenvirusisolaten in der jeweiligen Zieltierart durchgeführt, mit dem Ziel, geeignete Infektionsmodelle für zukünftige Vakzinestudien zu etablieren. Die Pathogenesestudien mit den Isolaten GTPV-"V/103" und LSDV-"Macedonia2016" zeigten, dass beide Virusisolate gute Kandidaten für Infektionsmodelle mit GTPV und LSDV darstellen. Um ein geeignetes Infektionsmodell für SPPV zu finden, war die Testung von drei verschiedenen SPPV-Isolaten (SPPV-"V/104", SPPV-"India/2013/Surankote" und SPPV-"Egypt/2018") notwendig. Letztendlich stellte sich das virulente SPPV-"India/2013/Surankote"-Isolat als geeignetster Kandidat heraus. Abschließend wurden verschiedene Prototypen einer inaktivierten LSDV-Vakzine entwickelt und hinsichtlich Abwehrreaktionen und Schutzwirkung im Rind getestet. Der entwickelte Vakzinekandidat induzierte einen vollständigen klinischen Schutz in Rindern und erwies sich damit als sehr vielversprechend. Molekulare und serologische Daten weisen zudem darauf hin, dass mit dieser Prototypvakzine eine sterile Immunität in den Rindern erzielt werden konnte. Eine kommerzielle Vakzine mit diesen Eigenschaften würde einen bedeutenden Fortschritt in der Kontrolle von LSDV darstellen. Weitere Studien mit dem Ziel, die Diagnostik und Kontrolle von Capripockenviren weiter zu verbessern, sind auch in Zukunft noch notwendig. Dieses betrifft beispielsweise die Entwicklung Sonden-basierter real-time qPCR-Assays zur Unterscheidung von SPPV- und GTPV-Feld- und Vakzinestämmen, die den diagnostischen Workflow komplettieren würden. Von Bedeutung sind außerdem weiterführende Tests der inaktivierten Prototypvakzine hinsichtlich der minimalen protektiven Dosis und einer möglichen Kreuzprotektion in Schafen und Ziegen gegen SPPV und GTPV.

Die Gattung Capripoxvirus beinhaltet das Virus der Lumpy-Skin-Krankheit (LSDV), das Schafpockenvirus (SPPV) und das Ziegenpockenvirus (GTPV), die hauptsächlich Rinder bzw. Schafe und Ziegen infizieren. Während LSDV vorwiegend mechanisch über blutsaugende Vektoren und möglicherweise über Schildzecken übertragen wird, sind der direkte Kontakt sowie die Aerosoltransmission als Hauptübertragungsrouten für SPPV und GTPV beschrieben. Betroffene Tiere entwickeln Fieber und zeigen klinische Anzeichen wie z.B. okularen und nasalen Ausfluss, Lymphadenopathie und charakteristische Hautläsionen. Schwere Krankheitsverläufe, insbesondere in Verbindung mit respiratorischen Symptomen, können für die infizierten Tiere zum Tod führen. In endemischen Gebieten ist die Mortalität Capripockenvirus-induzierter Erkrankungen relativ gering (1-10%). In exotischen Rassen oder in Tieren, die auf Hochleistung (zum Beispiel Milch- oder Fleischrassen) gezüchtet wurden, kann die Mortalität von LSDV bis zu 75% und die Mortalität von SPPV und GTPV bis zu 100% betragen. Der aus den Hautläsionen resultierende Qualitätsverlust des Leders, reduzierte Gewichtszunahme und reduzierte Milchleistung sowie der Verlust betroffener Tiere führen zu Umsatzeinbußen und beeinflussen dadurch sowohl die nationale als auch die globale Wirtschaft. Dadurch haben Capripockenvirus-induzierte Erkrankungen nicht nur einen erheblichen Einfluss auf das infizierte Einzeltier, sondern auch auf kleine Familienunternehmen und landwirtschaftliche Großbetriebe. Derzeit sind zur Prophylaxe lediglich attenuierte Lebendvakzinen kommerziell erhältlich. Diese sind in der Europäischen Union jedoch nicht zugelassen, da ihr Einsatz den Verlust des Status "Capripocken-frei" für das jeweilige Land bedeutet. Aus diesen Gründen werden dringend sowohl zuverlässige und zeitsparende Diagnostikmethoden für die Detektion und Charakterisierung von Capripocken, als auch sichere und effiziente Kontrollmaßnahmen benötigt. Ziele dieser Arbeit waren die Entwicklung, Validierung und vergleichende Analyse verschiedener diagnostischer Methoden, die Durchführung von Pathogenesestudien zur Etablierung von Infektionsmodellen für alle drei Capripockenviren und die Entwicklung und Testung verschiedener inaktivierter Prototypvakzinen gegen das LSDV. Im Laufe dieser Arbeit wurden neue real-time quantitative Polymerasekettenreaktion (qPCR)-Assays für eine robuste Detektion und Differenzierung zwischen LSDV-Feldstämmen, LSDV-Vakzinestämmen, SPPV und GTPV entwickelt und umfassend validiert. Im Anschluss wurden jeweils zwei dieser Einzelassays zu sogenannten Duplex-Assays kombiniert. Der erste Duplex-Assay ist in der Lage, zwischen LSDV-Feldstämmen und LSDV-Vakzinestämmen zu unterschieden, der zweite Duplex-Assay erlaubt die Differenzierung zwischen SPPV und GTPV. Schließlich wurde ein diagnostischer Workflow basierend auf den beiden neuen Duplex-Assays in Kombination mit bereits publizierten Methoden etabliert. Dieser ermöglicht eine zeitsparende, robuste und zuverlässige Detektion, Spezies-spezifische Identifizierung und genetische sowie phylogenetische Charakterisierung der drei Capripockenvirusspezies. Zudem wurden bereits vorhandene serologische Diagnostikmethoden (der Serumneutralisationstest und ein kommerziell erhältlicher ELISA) hinsichtlich ihrer Sensitivität und ihrer Spezifität verglichen. Des Weiteren wurden Pathogenesestudien mit verschiedenen Capripockenvirusisolaten in der jeweiligen Zieltierart durchgeführt, mit dem Ziel, geeignete Infektionsmodelle für zukünftige Vakzinestudien zu etablieren. Die Pathogenesestudien mit den Isolaten GTPV-"V/103" und LSDV-"Macedonia2016" zeigten, dass beide Virusisolate gute Kandidaten für Infektionsmodelle mit GTPV und LSDV darstellen. Um ein geeignetes Infektionsmodell für SPPV zu finden, war die Testung von drei verschiedenen SPPV-Isolaten (SPPV-"V/104", SPPV-"India/2013/Surankote" und SPPV-"Egypt/2018") notwendig. Letztendlich stellte sich das virulente SPPV-"India/2013/Surankote"-Isolat als geeignetster Kandidat heraus. Abschließend wurden verschiedene Prototypen einer inaktivierten LSDV-Vakzine entwickelt und hinsichtlich Abwehrreaktionen und Schutzwirkung im Rind getestet. Der entwickelte Vakzinekandidat induzierte einen vollständigen klinischen Schutz in Rindern und erwies sich damit als sehr vielversprechend. Molekulare und serologische Daten weisen zudem darauf hin, dass mit dieser Prototypvakzine eine sterile Immunität in den Rindern erzielt werden konnte. Eine kommerzielle Vakzine mit diesen Eigenschaften würde einen bedeutenden Fortschritt in der Kontrolle von LSDV darstellen. Weitere Studien mit dem Ziel, die Diagnostik und Kontrolle von Capripockenviren weiter zu verbessern, sind auch in Zukunft noch notwendig. Dieses betrifft beispielsweise die Entwicklung Sonden-basierter real-time qPCR-Assays zur Unterscheidung von SPPV- und GTPV-Feld- und Vakzinestämmen, die den diagnostischen Workflow komplettieren würden. Von Bedeutung sind außerdem weiterführende Tests der inaktivierten Prototypvakzine hinsichtlich der minimalen protektiven Dosis und einer möglichen Kreuzprotektion in Schafen und Ziegen gegen SPPV und GTPV. ; The genus Capripoxvirus of the family Poxviridae consists of the species lumpy skin disease virus, sheeppox virus and goatpox virus that affect cattle, sheep and goats, respectively. Whereas lumpy skin disease virus (LSDV) is transmitted mainly mechanically via blood-feeding insects and possibly hard ticks, the major transmission routes of sheeppox virus (SPPV) and goatpox virus (GTPV) are via direct contact and aerosols. Affected animals develop fever and display clinical signs such as ocular and nasal discharge, lymphadenopathy and characteristic lesions of the skin. Severe clinical course, especially in combination with respiratory signs, can result in the death of the affected animals. In endemic regions, mortality of capripox virus-induced diseases is low (1-10%). However, mortalities of up to 75% have been reported for LSDV and up to 100% for SPPV and GTPV in exotic breeds and high-producing dairy or beef animals. The loss of quality of the leather, reduced weight gain and milk yield as well as complete loss of affected animals have severe impact on national and global economies. Therefore, capripox virus-induced diseases have significant impact on both the affected individual animal as well as on the existence of small-scale farmers and large agricultural enterprises. However, until now, only live attenuated vaccines are commercially available. These attenuated vaccines are not authorized in the European Union and their administration would comprise the disease-free status of the respective country. Thus, reliable diagnostic tools for the detection and characterization of capripox viruses as well as safe and efficient control measures are of high importance. The objectives of the present thesis were the development, validation and comparison of diagnostic tools, the establishment of challenge infection models and the performance of pathogenesis studies for all three capripox virus species, and the development and testing of different inactivated prototype vaccine candidates against LSDV. First, new real-time quantitative polymerase chain reaction (qPCR) assays for robust detection and differentiation of LSDV field strains, LSDV vaccine strains, SPPV and GTPV were developed and extensively validated. In the following, two single assays were combined to duplex assays, one for the differentiation between LSDV field strains and LSDV vaccine strains, and the second for discrimination of SPPV and GTPV. Finally, a diagnostic workflow based on these new duplex assays in combination with already published methods was established. This workflow enables time-saving, robust and reliable detection, species-specific identification and genetic and phylogenetic characterization of all three capripox virus species. In addition, already existing serological examination methods (serum neutralization assay and commercial enzyme-linked immunosorbent assay) were compared regarding their sensitivity and specificity. Furthermore, pathogenesis studies with different capripox virus isolates were performed in the respective target species, and the suitability of selected virus isolates as challenge viruses for future vaccine studies was analyzed. Pathogenesis studies with isolates GTPV-"V/103" and LSDV-"Macedonia2016" revealed that both are proper candidates for challenge models. Finally, three different SPPV isolates (SPPV-"V/104", SPPV-"India/2013/Surankote" and SPPV-"Egypt/2018") were tested in sheep regarding their virulence to find a suitable challenge model for SPPV, and SPPV-"India/2013/Surankote" was chosen for future vaccine studies. Once appropriate challenge models were established, different inactivated prototype vaccines against LSDV were developed, and vaccine safety as well as vaccine efficacy were tested in cattle. Eventually, a Polygen-adjuvanted inactivated LSDV-vaccine candidate was selected that is able to fully prevent cattle from any LSDV-related clinical signs after severe challenge infection. Furthermore, molecular and serological data indicate that this inactivated prototype vaccine is even able to induce a kind of "sterile immunity" against LSDV in those cattle. It has to be mentioned that a commercially available vaccine similar to this prototype vaccine would be a great advance for the control of LSDV. In the future, additional studies addressing diagnostics and optimized control of capripox viruses should be performed. Firstly, probe-based real-time qPCR assays for the differentiation of SPPV and GTPV vaccine strains from their respective virulent field strains should be developed and included into the diagnostic workflow. Secondly, further tests of the inactivated prototype vaccine, e.g. determination of the minimum protective dose and the possibility of cross-protection in sheep and goats against SPPV and GTPV, respectively, should be performed.

[EN]: The genus Anaplasmais one of four distinct genera in the family Anaplasmataceae, which are obligate intracellular pathogens vectored by ticks and found exclusively within parasitophorous vacuoles in the host cell cytoplasm. The 2001 reclassification of the order Rickettsiales expanded the genus Anaplasma, which previously contained pathogens that were host specific for ruminants (A. marginale, A. centrale and A. bovis), by adding A. phagocytophilum, a unification of three organisms previously classified as Ehrlichia (E. equi, E. phagocytophila and the unnamed agent of human granulocytic ehrlichiosis). Also included in the genus Anaplasma were A. bovis (formerly E. bovis), A. platys (formerly E. platys) and Aegyptianella pullorum. Despite the genomic relatedness of the regrouped organisms, many aspects of their biology are diverse, including their host specificity, host cell preferences, major surface proteins (MSPs) and tick vectors. This review focuses on the two most important pathogens: A. marginale, which causes bovine anaplasmosis, and A. phagocytophilum, the aetiologic agent of tick-borne fever in sheep and human granulocytic anaplasmosis, an emerging tick-borne disease of humans. For both pathogens, strain diversity is much greater than previously recognised. While MSPs were found to be useful in phylogenetic studies and strain identification, highly conserved MSPs were found to affect the specificity of serologic tests. Comparison of these two important pathogens highlights the challenges and insight derived from reclassification and molecular analysis, both of which have implications for the development and evaluation of diagnosis and control strategies. ; [FR]: Le genre Anaplasma est l'un des quatre genres distincts de la famille des Anaplasmataceae, bactéries pathogènes intracellulaires obligatoires vectorisées par des tiques et présentes exclusivement dans les vacuoles parasitophores du cytoplasme des cellules hôtes. Suite à la reclassification de l'ordre des Rickettsiales en 2001, le genre Anaplasma, qui ne contenait précédemment que des pathogènes ayant une spécificité d'hôte pour les ruminants (A. marginale, A. centrale et A. ovis) a été reconsidéré et intègre désormais A. phagocytophilum, taxon regroupant trois microorganismes précédemment classés dans le genre Ehrlichia (E. equi, E. phagocytophila et l'agent de l'ehrlichiose granulocytaire humaine). Le genre Anaplasma contient également A. bovis (anciennement E. bovis), A. platys (anciennement E. platys) et Aegyptianella pullorum. En dépit de leur parenté génomique, les microorganismes ainsi regroupés se distinguent par de nombreux aspects de leur biologie, en particulier leur spécificité d'hôte, le tropisme des cellules hôtes, les protéines majeures de surface et la transmission par des tiques vectrices. Les auteurs examinent tout particulièrement les deux principaux agents pathogènes de ce genre, à savoir A. marginale, l'agent de l'anaplasmose bovine, et A. phagocytophilum, l'agent étiologique de fièvres transmises par les tiques chez les ovins et de l'anaplasmose granulocytaire humaine, une maladie humaine émergente transmise par les tiques. La diversité des souches de ces deux agents est bien plus importante qu'on ne l'avait estimé précédemment. Les protéines majeures de surface jouent un rôle précieux lors des études phylogénétiques et de l'identification des souches, mais il a été constaté qu'une conservation trop longue altérait la spécificité des tests sérologiques. La comparaison entre ces deux agents pathogènes majeurs souligne les défis et les éclairages nouveaux induits par la reclassification et par l'analyse moléculaire ainsi que leurs répercussions, dans chaque cas, sur la conception et la mise en œuvre dans le temps de stratégies de diagnostic et de contrôle appropriées. ; [ES]: El género Anaplasma es uno de los cuatro que componen la familia Anaplasmataceae, integrada por patógenos intracelulares obligados que se transmiten por garrapatas y residen exclusivamente en vacuolas parasitóforas dentro del citoplasma de las células del hospedador. En 2001, al reclasificar el orden Rickettsiales, se amplió el género Anaplasma, que hasta entonces contenía patógenos específicos de distintos hospedadores rumiantes (A. marginale, A. centrale y A. ovis), para dar cabida en él a A. phagocytophilum, especie resultante de la unificación de tres microorganismos anteriormente clasificados como Ehrlichia (E. equi, E. phagocytophila y el agente innominado de la erliquiosis granulocítica humana). También se incluyeron en el género Anaplasma las especies A. bovis (anteriormente E. bovis), A. platys (anteriormente E. platys) y Aegyptianella pullorum. A pesar del parentesco genómico que existe entre los microorganismos reagrupados, estos difieren en muchos aspectos de su biología, en particular su especificidad por uno u otro hospedador, su tropismo por distintos tipos celulares, sus principales proteínas de superficie (PPS), y las garrapatas que ejercen de vector. Los autores se centran en los dos patógenos más importantes: A. marginale, causante de la anaplasmosis bovina, y A. phagocytophilum, causante en los ovinos de una fiebre transmitida por garrapatas y en el hombre de anaplasmosis granulocítica, enfermedad humana emergente que también se transmite por garrapatas. En ambos patógenos, la diversidad entre cepas es mucho mayor de lo que anteriormente se había observado. Se ha descubierto que las PPS son útiles para los estudios filogenéticos y la caracterización de las cepas, y también se ha observado que las PPS muy conservadas afectan a la especificidad de las técnicas de prueba serológica. La comparación entre estos dos importantes patógenos pone de manifiesto las dificultades y los nuevos conocimientos que han traído consigo la reclasificación y el análisis molecular, que a su vez tienen repercusiones en la concepción y evaluación de estrategias de diagnóstico y control. ; The preparation of this paper was supported by Grant BFU2011-23896, the European Union FP7 ANTIGONE project, number 278976, and the Walter R. Sitlington Endowed Chair for Food Animal Research to K.M. Kocan. ; Peer Reviewed