A review of insect parasitoids associated with Lobesia botrana (Denis & Schiffermüller, 1775) in Italy. 1. DipteraTachinidae and HymenopteraBraconidae (Lepidoptera, Tortricidae)

Influence of Vineyard Inter-Row Management on Grapevine Leafhoppers and Their Natural Enemies

Inter-row management in vineyards can influence the abundance of grapevine pests and their natural enemies. In 2013-2015, in a vineyard in northeastern Italy, the influence of two vineyard inter-row management strategies (i.e., alternate mowing, AM, and periodical tillage, PT) on the population dynamics of grapevine leafhoppers Hebata vitis and Zygina rhamni and their natural enemies, the mymarid Anagrus atomus and spiders (Araneae), and other hymenopteran parasitoids, were studied with different survey approaches. The infestations of both leafhoppers were lower in AM than PT due to the reduced leafhopper oviposition and higher nymph mortality in AM. This occurred although leafhopper egg parasitization by A. atomus was greater in PT than AM according to a density-dependent relationship with the leafhopper egg amount. Hymenopteran parasitoids other than A. atomus were the most abundant in AM, probably due to the higher availability of nectar and pollen than in PM. The significantly higher population densities of hunting spiders in AM than PT can be associated with the higher predation of leafhopper nymphs. Therefore, the study demonstrated that the alternate mowing of vineyard inter-rows enhances the abundance of natural enemies, such as spiders and hymenopteran parasitoids, and can contribute to grapevine leafhopper pest control.

Parasitoids of Lobesia botrana (Lepidoptera: Tortricidae) in the Douro Demarcated Region vineyards and the prospects for enhancing conservation biological control

The more restrictive regulations of pesticides in Europe have led to an increase in conservation biological control (CBC) research. However, little attention has been paid to the main determinants of Lobesia botrana parasitism. The Douro Demarcated Region landscape offers scope for the use of CBC. The study was conducted between 2002 and 2015 aiming at: (i) identifying parasitoids associated with L. botrana and evaluating their impact as biological control agents in each generation of the pest, and (ii) evaluating the effect of both the proportion of ecological infrastructures (EI) near the vineyards, and the impact of management practices (chemical treatments and ground cover) on the parasitism of L. botrana. A total of 3226 larvae/pupae of L. botrana were collected (15% were parasitized and 485 parasitoids emerged). A complex of 16 taxa of parasitoids was identified, the majority belonging to Hymenoptera. The most abundant were Elachertus sp. (Eulophidae), Campoplex capitator Aubert (Ichneumonidae), and Brachymeria tibialis (Walker) (Chalcididae), which represented 62.5, 12.6, and 12.0% of the total assemblage of parasitoids which emerged, respectively. The percentage of parasitism ranged from 0.0 to 61.5% (first generation), from 0.0 to 36.8% (second generation), and from 0.0 to 12.1% (third generation). Importantly, it was found that the parasitism rate was higher in vineyards with ground cover. In addition, EI in the area surrounding the vineyards produced a significant increase in parasitism. These results suggest potential for CBC of L. botrana if EI around vineyards, and ground cover with native perennial plants within vineyards, are encouraged.

Back to the Wild: The Parasitoid Community of Lobesia botrana (Lepidoptera: Tortricidae) in a Grapevine-Free Natural Environment

Simple Summary

In a framework of sustainable agriculture, strategies aimed at preserving and enhancing pest natural enemies are crucial. However, knowledge about the parasitoid complex associated with a particular pest is often fragmentary. Herein, we investigated the parasitoids associated with the European grapevine moth, one of the main vine pests in the Mediterranean area, in a natural context, where the moth lives on Daphne gnidium, deemed as its original host plant. We observed a heterogeneous and complex community, consisting of a few predominant parasitoid species, followed by satellite species, and occasional parasitoids. Parasitic wasps, such as Campoplex capitator and Trichogramma spp., can be also found in the vineyards, thus understanding their dynamics in the wild could be useful to improve biological control strategies for managing EGVM populations.

Abstract

The European grapevine moth (EGVM), Lobesia botrana (Lepidoptera: Tortricidae), is one of the major concerns for vineyard managers in the Mediterranean area. It is a polyphagous moth, which develops on a wide variety of host plants, among which the spurge flax, Daphne gnidium (Thymelaeaceae), very likely represents its originary wild host plant. In this study, we investigated the parasitoid complex of L. botrana feeding on D. gnidium during a three-year sampling in a natural reserve in Tuscany, Italy, where this plant is extremely abundant while the grapevine is absent. A total of 24 species of parasitoids were obtained from eggs, larvae, and pupae of EGVM, belonging to 6 families of Hymenoptera and a family of Diptera. The ichneumonid wasp Campoplex capitator was the most abundant larval parasitoid. Four species of the genus Trichogramma were obtained from parasitized eggs during the first year of sampling, with a peak in the parasitisation during the EGVM 3rd generation. Some of the main EGVM parasitoids on spurge flax were also observed in vineyards, although a certain degree of redundancy was observed in the wild, due to several less frequent “satellite” species exploiting the same host. Overall, this research sheds light on the parasitoid community and dynamics of this important moth pest in a grapevine-free natural ecosystem, discussing the possible role of natural areas as ecological reservoirs of pest natural enemies.

Lobesia botrana: A Biological Control Approach with a Biopesticide Based on Entomopathogenic Fungi in the Winter Season in Chile

Simple Summary

Lobesia botrana, also known as the European grapevine moth, is one of the main pests that affect grapes. In Chile, this type of moth is classified as a quarantine pest, which requires fumigating the fruit with methyl bromide to prevent the immature stages of the pest from being strained and reaching the export-destination countries. In the fields, the larvae of this moth feed on grapes, which can introduce diseases such as Botrytis cinerea, thereby increasing the costs of managing the crop. One way to control this pest is to use entomopathogenic fungi on the winter pupae to reduce moth populations in the spring. In the present study, six fungi were characterized, formulated, and evaluated. The selected strains RGM 2184 and RGM 678 were evaluated in two regions of Chile during two seasons. These strains reached maximum efficiencies of 80% and 88%, respectively. Therefore, the use of entomopathogenic fungi is an environmentally friendly alternative to control L. botrana and reduce the use of chemical pesticides.

Abstract

Lobesia botrana (Denis and Shiffermüller) (Lepidoptera: Tortricidae) is one of the main pests that affect the production and export of table grapes in Chile. Because this pest has quarantine status, the fruit must be fumigated with methyl bromide, which reduces the fruit’s export competitiveness in the destination market. In the present study, to help resolve this issue, six native entomopathogenic fungi were identified through multilocus analysis, including three Beauveria pseudobassiana and three Metarhizium robertsii. These fungi were evaluated in the laboratory to control L. botrana in its pupal stage in a silk cocoon and compared against a biological control product. Formulations with additional carbon sources improved the performance of the fungi. The treatments with outstanding performance contained the fungal strains B. pseudobassiana RGM 2184 and M. robertsii RGM 678. These strains were evaluated in the field during the winter season in two different regions of the country; the strains reached maximum efficacies of 80% and 88%, respectively, at 21 days post first application. Therefore, entomopathogenic fungi can contribute to reducing pupal populations in winter, thereby decreasing the moth population in spring–summer.

Potential of in vivo- and in vitro-cultured entomopathogenic nematodes to infect Lobesia vanillana (Lepidoptera: Tortricidae) under laboratory conditions

Entomopathogenic nematodes (EPNs) have been successfully applied as biological control agents against above ground and soil stages of insect pests. However, for commercial application, it is crucial to mass culture these nematodes using in vitro liquid culture technology, as it is not attainable when using susceptible insects as hosts. Lobesia vanillana (Lepidoptera: Tortricidae) is regarded a sporadic pest of wine grapes in South Africa. The in vivo- and in vitro-cultured South African EPNs, Steinernema yirgalemense and Steinernema jeffreyense (Rhabditida: Steinernematidae), were evaluated against larvae and pupae of L. vanillana in laboratory bioassays. For larvae, high mortality was observed for all treatments: In vitro-cultured S. yirgalemense (98%) performed better than S. jeffreyense (73%), while within in vivo cultures, there was no difference between nematode species (both 83%). No significant difference was detected between in vivo- and in vitro cultures of the same nematode species. The LD50 of the in vitro-cultured S. yirgalemense, was 7.33 nematodes per larva. Mortality by infection was established by dissecting L. vanillana cadavers and confirming the presence of nematodes, which was > 90% for all treatments. Within in vitro cultures, both S. yirgalemense and S. jeffreyense were able to produce a new cohort of infective juveniles from L. vanillana larvae. Pupae, however, were found to be considerably less susceptible to EPN infection. This is the first study on the use of EPNs to control L. vanillana. The relative success of in vitro-cultured EPN species in laboratory assays, without any loss in pathogenicity, is encouraging for further research and development of this technology.

Tachinid (Diptera, Tachinidae) parasitoids of Lobesia botrana (Denis & Schiffermüller, 1775) (Lepidoptera, Tortricidae) and other moths

The present paper reports data on the biology of eleven species of tachinid flies collected in Italy and Spain on different host plants and emerged from different host larvae. An annotated list of the eleven species emerged from the collected lepidopterans is provided; information about distribution and biology are given as well as the description of their puparia. Two new parasitoid species of the European Grapevine Moth (EGVM) Lobesia botrana were recorded: Clemelis massilia, whose host preferences were unknown so far, and Neoplectops pomonellae. A list of lepidopteran pest species with their associated plants and tachinid parasitoids is then given in order to highlight the relationships among the three components of the biocenosis (plant, herbivore and parasitoid). Eventually, due to the great economic importance of L. botrana in viticulture, a preliminary identification key to the puparia of its tachinid parasitoids is provided.

Annotated and illustrated world checklist of Microgastrinae parasitoid wasps (Hymenoptera, Braconidae)

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 Alphomelondisputabile (Ashmead, 1900), Alphomelonnigriceps (Ashmead, 1900), Cotesiasalebrosa (Marshall, 1885), Diolcogasterxanthaspis (Ashmead, 1900), Dolichogenideaononidis (Marshall, 1889), Glyptapantelesacraeae (Wilkinson, 1932), Glyptapantelesguyanensis (Cameron, 1911), Glyptapantelesmilitaris (Walsh, 1861), and Pseudapantelesannulicornis Ashmead, 1900; 3) Three new replacement names are a) Diolcogasteraurangabadensis Fernandez-Triana, replacing Diolcogasterindicus (Rao & Chalikwar, 1970) [nec Diolcogasterindicus (Wilkinson, 1927)], b) Dolichogenideaincystatae Fernandez-Triana, replacing Dolichogenidealobesia Liu & Chen, 2019 [nec Dolichogenidealobesia Fagan-Jeffries & Austin, 2019], and c) Microplitisvitobiasi Fernandez-Triana, replacing Microplitisvariicolor Tobias, 1964 [nec Microplitisvaricolor Viereck, 1917]; 4) Three names amended are Apantelesirenecarrilloae Fernandez-Triana, 2014, Cotesiaayerzai (Brèthes, 1920), and Cotesiariverai (Porter, 1916); 5) Seven species have their status revised: Cotesiaarctica (Thomson, 1895), Cotesiaokamotoi (Watanabe, 1921), Cotesiaukrainica (Tobias, 1986), Dolichogenideaappellator (Telenga, 1949), Dolichogenideamurinanae (Capek & Zwölfer, 1957), Hypomicrogasteracarnas Nixon, 1965, and Nyererianigricoxis (Wilkinson, 1932); 6) New combinations are given for 318 species: Alloplitiscongensis, Alloplitisdetractus, Apantelesasphondyliae, Apantelesbraziliensis, Apantelessulciscutis, Choerasaper, Choerasapollion, Choerasdaphne, Choerasfomes, Choerasgerontius, Choerashelle, Choerasirates, Choeraslibanius, Choeraslongiterebrus, Choerasloretta, Choerasrecusans, Choerassordidus, Choerasstenoterga, Choerassuperbus, Choerassylleptae, Choerasvacillatrix, Choerasvacillatropsis, Choerasvenilia, Cotesiaasavari, Cotesiabactriana, Cotesiabambeytripla, Cotesiaberberidis, Cotesiabhairavi, Cotesiabiezankoi, Cotesiabifida, Cotesiacaligophagus, Cotesiacheesmanae, Cotesiacompressithorax, Cotesiadelphinensis, Cotesiaeffrena, Cotesiaeuphobetri, Cotesiaelaeodes, Cotesiaendii, Cotesiaeuthaliae, Cotesiaexelastisae, Cotesiahiberniae, Cotesiahyperion, Cotesiahypopygialis, Cotesiahypsipylae, Cotesiajujubae, Cotesialesbiae, Cotesialevigaster, Cotesializeri, Cotesiamalevola, Cotesiamalshri, Cotesiamenezesi, Cotesiamuzaffarensis, Cotesianeptisis, Cotesianycteus, Cotesiaoeceticola, Cotesiaoppidicola, Cotesiaopsiphanis, Cotesiapachkuriae, Cotesiapaludicolae, Cotesiaparbhanii, Cotesiaparvicornis, Cotesiapratapae, Cotesiaprozorovi, Cotesiapterophoriphagus, Cotesiaradiarytensis, Cotesiarangii, Cotesiariverai, Cotesiaruficoxis, Cotesiasenegalensis, Cotesiaseyali, Cotesiasphenarchi, Cotesiasphingivora, Cotesiatransuta, Cotesiaturkestanica, Diolcogasterabengouroui, Diolcogasteragama, Diolcogasterambositrensis, Diolcogasteranandra, Diolcogasterannulata, Diolcogasterbambeyi, Diolcogasterbicolorina, Diolcogastercariniger, Diolcogastercincticornis, Diolcogastercingulata, Diolcogastercoronata, Diolcogastercoxalis, Diolcogasterdipika, Diolcogasterearina, Diolcogasterepectina, Diolcogasterepectinopsis, Diolcogastergrangeri, Diolcogasterheterocera, Diolcogasterhomocera, Diolcogasterindica, Diolcogasterinsularis, Diolcogasterkivuana, Diolcogastermediosulcata, Diolcogastermegaulax, Diolcogasterneglecta, Diolcogasternigromacula, Diolcogasterpalpicolor, Diolcogasterpersimilis, Diolcogasterplecopterae, Diolcogasterplutocongoensis, Diolcogasterpsilocnema, Diolcogasterrufithorax, Diolcogastersemirufa, Diolcogasterseyrigi, Diolcogastersubtorquata, Diolcogastersulcata, Diolcogastertorquatiger, Diolcogastertristiculus, Diolcogasterturneri, Diolcogastervulcana, Diolcogasterwittei, Distatrixanthedon, Distatrixcerales, Distatrixcuspidalis, Distatrixeuproctidis, Distatrixflava, Distatrixgeometrivora, Distatrixmaia, Distatrixtookei, Distatrixtermina, Distatrixsimulissima, Dolichogenideaagamedes, Dolichogenideaaluella, Dolichogenideaargiope, Dolichogenideaatreus, Dolichogenideabakeri, Dolichogenideabasiflava, Dolichogenideabersa, Dolichogenideabiplagae, Dolichogenideabisulcata, Dolichogenideacatonix, Dolichogenideachrysis, Dolichogenideacoffea, Dolichogenideacoretas, Dolichogenideacyane, Dolichogenideadiaphantus, Dolichogenideadiparopsidis, Dolichogenideadryas, Dolichogenideaearterus, Dolichogenideaensiger, Dolichogenideaeros, Dolichogenideaevadne, Dolichogenideafalcator, Dolichogenideagelechiidivoris, Dolichogenideagobica, Dolichogenideahyalinis, Dolichogenideairiarte, Dolichogenidealakhaensis, Dolichogenidealampe, Dolichogenidealaspeyresiella, Dolichogenidealatistigma, Dolichogenidealebene, Dolichogenidealucidinervis, Dolichogenideamalacosomae, Dolichogenideamaro, Dolichogenideamendosae, Dolichogenideamonticola, Dolichogenideanigra, Dolichogenideaolivierellae, Dolichogenideaparallelis, Dolichogenideapelopea, Dolichogenideapelops, Dolichogenideaphaenna, Dolichogenideapisenor, Dolichogenidearoepkei, Dolichogenideascabra, Dolichogenideastatius, Dolichogenideastenotelas, Dolichogenideastriata, Dolichogenideawittei, Exoryzaasotae, Exoryzabelippicola, Exoryzahylas, Exoryzamegagaster, Exoryzaoryzae, Glyptapantelesaggestus, Glyptapantelesagynus, Glyptapantelesaithos, Glyptapantelesamenophis, Glyptapantelesantarctiae, Glyptapantelesanubis, Glyptapantelesarginae, Glyptapantelesargus, Glyptapantelesatylana, Glyptapantelesbadgleyi, Glyptapantelesbataviensis, Glyptapantelesbistonis, Glyptapantelesborocerae, Glyptapantelescacao, Glyptapantelescadei, Glyptapantelescinyras, Glyptapanteleseryphanidis, Glyptapanteleseuproctisiphagus, Glyptapanteleseutelus, Glyptapantelesfabiae, Glyptapantelesfulvigaster, Glyptapantelesfuscinervis, Glyptapantelesgahinga, Glyptapantelesglobatus, Glyptapantelesglyphodes, Glyptapantelesguierae, Glyptapanteleshorus, Glyptapantelesintricatus, Glyptapanteleslamprosemae, Glyptapanteleslefevrei, Glyptapantelesleucotretae, Glyptapanteleslissopleurus, Glyptapantelesmadecassus, Glyptapantelesmarquesi, Glyptapantelesmelanotus, Glyptapantelesmelissus, Glyptapantelesmerope, Glyptapantelesnaromae, Glyptapantelesnepitae, Glyptapantelesnigrescens, Glyptapantelesninus, Glyptapantelesnkuli, Glyptapantelesparasundanus, Glyptapantelespenelope, Glyptapantelespenthocratus, Glyptapantelesphilippinensis, Glyptapantelesphilocampus, Glyptapantelesphoebe, Glyptapantelesphytometraduplus, Glyptapantelespropylae, Glyptapantelespuera, Glyptapantelesseydeli, Glyptapantelessiderion, Glyptapantelessimus, Glyptapantelesspeciosissimus, Glyptapantelesspilosomae, Glyptapantelessubpunctatus, Glyptapantelesthespis, Glyptapantelesthoseae, Glyptapantelesvenustus, Glyptapanteleswilkinsoni, Hypomicrogastersamarshalli, Iconellacajani, Iconelladetrectans, Iconellajason, Iconellalynceus, Iconellapyrene, Iconellatedanius, Illidopsazamgarhensis, Illidopslamprosemae, Illidopstrabea, Keylimepiestriatus, Microplitisadisurae, Microplitismexicanus, Neoclarkinellaariadne, Neoclarkinellacurvinervus, Neoclarkinellasundana, Nyereriaituriensis, Nyererianioro, Nyereriaproagynus, Nyereriataoi, Nyereriavallatae, Parapantelesaethiopicus, Parapantelesalternatus, Parapantelesaso, Parapantelesatellae, Parapantelesbagicha, Parapantelescleo, Parapantelescyclorhaphus, Parapantelesdemades, Parapantelesendymion, Parapantelesepiplemicidus, Parapantelesexpulsus, Parapantelesfallax, Parapantelesfolia, Parapantelesfurax, Parapanteleshemitheae, Parapanteleshyposidrae, Parapantelesindicus, Parapantelesjavensis, Parapantelesjhaverii, Parapantelesmaculipalpis, Parapantelesmaynei, Parapantelesneocajani, Parapantelesneohyblaeae, Parapantelesnydia, Parapantelesprosper, Parapantelesprosymna, Parapantelespunctatissimus, Parapantelesregalis, Parapantelessarpedon, Parapantelessartamus, Parapantelesscultena, Parapantelestransvaalensis, Parapantelesturri, Parapantelesxanthopholis, Pholetesoracutus, Pholetesorbrevivalvatus, Pholetesorextentus, Pholetesoringenuoides, Pholetesorkuwayamai, Promicrogasterapidanus, Promicrogasterbriareus, Promicrogasterconopiae, Promicrogasteremesa, Promicrogastergrandicula, Promicrogasterorsedice, Promicrogasterrepleta, Promicrogastertyphon, Sathonbekilyensis, Sathonflavofacialis, Sathonlaurae, Sathonmikeno, Sathonruandanus, Sathonrufotestaceus, Venanidesastydamia, Venanidesdemeter, Venanidesparmula, and Venanidessymmysta.

Updated list of the insect parasitoids (Insecta, Hymenoptera) associated with Lobesia botrana (Denis & Schiffermüller, 1775) (Lepidoptera, Tortricidae) in Italy. 2. Hymenoptera, Ichneumonidae, Anomaloninae and Campopleginae

In this second review of the parasitoids recorded on Lobesia botrana (EGVM) in Italy, an updated list and summary of the information available on 14 taxa of Ichneumonidae belonging to the subfamilies Anomaloninae and Campopleginae are provided. For each taxon, geographic distributions, host ranges, ecological role in viticulture and/or in other crops, and taxonomy are provided and discussed. For the most interesting species, tables summarizing the parasitization rates recorded in the field on EGVM or other lepidopteran pests are given. Identification mistakes and wrong synonymies that have generated great confusion and often made geographic distributions and host ranges unreliable are highlighted. A list of four Anomaloninae and 27 Campopleginae recorded on EGVM in Europe is also provided. Among the species examined, Campoplex capitator Aubert is the only potential candidate for biological control of EGVM.