Scratching the tip of the iceberg: integrative taxonomy reveals 30 new species records of Microgastrinae (Braconidae) parasitoid wasps for Germany, including new Holarctic distributions.

Substantial parts of the European and German insect fauna still remain largely unexplored, the so-called "dark taxa". In particular, midges (Diptera) and parasitoid wasps (Hymenoptera) are abundant and species-rich throughout Europe, yet are often neglected in biodiversity research. One such dark taxon is Microgastrinae wasps (Hymenoptera: Braconidae), a group of parasitoids of lepidopteran caterpillars with 252 species reported in Germany so far. As part of the German Barcode of Life Project GBOL III: Dark Taxa, reverse DNA barcoding and integrative taxonomic approaches were used to shed some light on the German Fauna of Microgastrinae wasps. In our workflow, DNA barcoding was used for molecular clustering of our specimens in a first step, morphological examination of the voucher specimens in a second step, and host data compared in a third step. Here, 30 species are reported for the first time in Germany, adding more than 10% to the known German fauna. Information for four species is provided in a new Holarctic context, reporting them for the Nearctic or, respectively, Palaearctic region, and 26 additional country records are added from sequenced material available in the collections accessible to us. Molecular clusters that show signs of discrepancies are discussed. Results show that we are just scratching the tip of the iceberg of the unexplored Microgastrinae diversity in Germany.

A curated DNA barcode reference library for parasitoids of northern European cyclically outbreaking geometrid moths.

Large areas of forests are annually damaged or destroyed by outbreaking insect pests. Understanding the factors that trigger and terminate such population eruptions has become crucially important, as plants, plant-feeding insects, and their natural enemies may respond differentially to the ongoing changes in the global climate. In northernmost Europe, climate-driven range expansions of the geometrid moths Epirrita autumnata and Operophtera brumata have resulted in overlapping and increasingly severe outbreaks. Delayed density-dependent responses of parasitoids are a plausible explanation for the 10-year population cycles of these moth species, but the impact of parasitoids on geometrid outbreak dynamics is unclear due to a lack of knowledge on the host ranges and prevalences of parasitoids attacking the moths in nature. To overcome these problems, we reviewed the literature on parasitism in the focal geometrid species in their outbreak range and then constructed a DNA barcode reference library for all relevant parasitoid species based on reared specimens and sequences obtained from public databases. The combined recorded parasitoid community of E. autumnata and O. brumata consists of 32 hymenopteran species, all of which can be reliably identified based on their barcode sequences. The curated barcode library presented here opens up new opportunities for estimating the abundance and community composition of parasitoids across populations and ecosystems based on mass barcoding and metabarcoding approaches. Such information can be used for elucidating the role of parasitoids in moth population control, possibly also for devising methods for reducing the extent, intensity, and duration of outbreaks.

Characterisation of some species groups of Brachymeria (Hymenoptera: Chalcididae), with a review of the B. tibialis-group and description of a new species parasitizing Zygaena pupae (Lepidoptera: Zygaenidae).

The Brachymeria tibialis species group is newly recognized and diagnosed together with the Brachymeria annulata, femorata, kassiliensis and lasus species groups also newly defined. In these diagnoses a few morphological characters of the ventral part of the mesosoma, discovered in this study, are proposed to help differentiate the groups. The B. tibialis species group itself includes solely B. tibialis (Walker) and B. zygaenae Delvare Shaw n. sp., which was until now mixed with it. The biology and hosts of both species are summarized.

Larval parasitism in a specialist herbivore is explained by phenological synchrony and host plant availability.

Parasitism is a key factor in the population dynamics of many herbivorous insects, although its impact on host populations varies widely, for instance, along latitudinal and altitudinal gradients. Understanding the sources of geographical variation in host-parasitoid interactions is crucial for reliably predicting the future success of the interacting species under a context of global change. Here, we examine larval parasitism in the butterfly Aglais urticae in south-west Europe, where it is a mountain specialist. Larval nests were sampled over 2 years along altitudinal gradients in three Iberian mountain ranges, including the Sierra Nevada, home to its southernmost European population. Additional data on nettle condition and adult butterflies were obtained in the study areas. These data sources were used to investigate whether or not differences in parasitism rates are related to the geographical position and phenology of the host, and to the availability of the host plants. Phenological differences in the host populations between regions were related to the severity of summer drought and the corresponding differences in host plant availability. At the trailing-edge of its distribution, the butterfly's breeding season was restricted to the end of winter and spring, while in its northern Iberian range the season was prolonged until mid-summer. Although parasitism was an important source of mortality in all regions, parasitism rates and parasitoid richness were highest in the north and lowest in the south. Moreover, within a region, there was a notable increase in parasitism rates over time, which probably led to selection against an additional late summer host generation in northern regions. Conversely, the shorter breeding season in Sierra Nevada resulted in a loss of synchrony between the host and one important late season parasitoid, Sturmia bella, which may partly explain the high density of this butterfly species at the trailing-edge of its range. Our results support the key role of host phenology in accounting for differences in parasitism rates between populations. They also provide insights into how climate through host plant availability affects host phenology and, ultimately, the impact of parasitism on host populations.

Ecology and Genetic Structure of the Parasitoid Phobocampe confusa (Hymenoptera: Ichneumonidae) in Relation to Its Hosts, Aglais Species (Lepidoptera: Nymphalidae).

The biology of parasitoids in natural ecosystems remains very poorly studied, though they are key species for their functioning. Here we focused on Phobocampe confusa, a Nymphalini specialist, responsible for high mortality rates in charismatic butterfly species in Europe (genus Aglais). We studied its ecology and genetic structure in connection with those of its host butterflies in Sweden. To this aim, we gathered data from 428 P. confusa individuals reared from 6094 butterfly larvae (of A. urticae, A. io, and in two occasions of Araschnia levana) collected over two years (2017 and 2018) and across 19 sites distributed along a 500 km latitudinal gradient. We found that P. confusa is widely distributed along the latitudinal gradient. Its distribution seems constrained over time by the phenology of its hosts. The large variation in climatic conditions between sampling years explains the decrease in phenological overlap between P. confusa and its hosts in 2018 and the 33.5% decrease in the number of butterfly larvae infected. At least in this study, P. confusa seems to favour A. urticae as host. While it parasitized nests of A. urticae and A. io equally, the proportion of larvae parasitized is significantly higher for A. urticae. At the landscape scale, P. confusa is almost exclusively found in vegetated open land and near deciduous forests, whereas artificial habitats are negatively correlated with the likelihood of a nest to be parasitized. The genetic analyses on 89 adult P. confusa and 87 adult A. urticae using CO1 and AFLP markers reveal a low genetic diversity in P. confusa and a lack of genetic structure in both species, at the scale of our sampling. Further genetic studies using high-resolution genomics tools will be required to better understand the population genetic structure of P. confusa, its biotic interactions with its hosts, and ultimately the stability and the functioning of natural ecosystems.

Revision of the western Palaearctic species of Aleiodes Wesmael (Hymenoptera, Braconidae, Rogadinae). Part 2: Revision of the A. apicalis group.

The West Palaearctic species of the Aleiodes apicalis group (Braconidae: Rogadinae) as defined by van Achterberg & Shaw (2016) are revised. Six new species of the genus Aleiodes Wesmael, 1838, are described and illustrated: A. carbonaroides van Achterberg & Shaw, sp. nov., A. coriaceus van Achterberg & Shaw, sp. nov., A. improvisus van Achterberg & Shaw, sp. nov., A. nigrifemur van Achterberg & Shaw, sp. nov., A. turcicus van Achterberg & Shaw, sp. nov., and A. zwakhalsi van Achterberg & Shaw, sp. nov. An illustrated key to 42 species is included. Hyperstemma Shestakov, 1940, is retained as subgenus to accommodate A. chloroticus (Shestakov, 1940) and similar species. Fourteen new synonyms are proposed: Rogas bicolor Lucas, 1849 (not Spinola, 1808), Rogas rufo-ater Wollaston, 1858, Rhogas bicolorinus Fahringer, 1932, Rhogas reticulator var. atripes Costa, 1884, and Rhogas similis Szépligeti, 1903, of Aleiodes apicalis (Brullé, 1832); Rogas (Rogas) vicinus Papp, 1977, of Aleiodes aterrimus (Ratzeburg, 1852); Rogas affinis Herrich-Schäffer, 1838, of Aleiodes cruentus (Nees, 1834); Bracon dimidiatus Spinola, 1808, and Rhogas (Rhogas) dimidiatus var. turkestanicus Telenga, 1941, of Aleiodes gasterator (Jurine, 1807); Rogas alpinus Thomson, 1892, of Aleiodes grassator (Thunberg, 1822); Rhogas jaroslawensis Kokujev, 1898, of Aleiodes periscelis (Reinhard, 1863); Rhogas carbonarius var. giraudi Telenga, 1941, of Aleiodes ruficornis (Herrich-Schäffer, 1838); Ichneumon ductor Thunberg, 1822, of Aleiodes unipunctator (Thunberg, 1822); Rogas heterostigma Stelfox, 1953, of Aleiodes pallidistigmus (Telenga, 1941). Neotypes are designated for Rogas affinis Herrich-Schäffer, 1838; Rogas nobilis Haliday (in Curtis), 1834; Rogas pallidicornis Herrich-Schäffer, 1838; Rogas ruficornis Herrich-Schäffer, 1838. Lectotypes are designated for Rhogas (Rhogas) dimidiatus var. turkestanicus Telenga, 1941, and Rhogas hemipterus Marshall, 1897.

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 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, Glyptapantelessubpunctatus, 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.

Braconid and ichneumonid (Hymenoptera) parasitoid wasps of Lepidoptera from the Maltese Islands.

Fourteen species of Ichneumonidae are here recorded from the Maltese Islands. Of these, all were reared from Lepidoptera hosts with the exception of Netelia (Paropheltes) inedita (Kokujev) which was collected from a malaise trap. Of these, the following species (or genera) are here reported for the first time from the Maltese Islands: Chirotica meridionalis Horstmann, Gelis carbonarius (de Stefani), G. exareolatus (FÓ§rster), G. seyrigi Ceballos, Glypta sp., Meloboris sp., Netelia (Paropheltes) inedita (Kokujev), Ophion obscuratus Fabricius and Orthizema sp. Twenty-five species of Braconidae are also here reported from Lepidoptera hosts with the exception of Homolobus (Phylacter) meridionalis van Achterberg which was collected from a malaise trap. Of these, the following species (or genera) represent new records for the Maltese Islands: Apanteles metacarpalis (Thomson), Ascogaster sp., Clinocentrus excubitor (Haliday) [previously misidentified as C. exsertor (Nees) by Papp (2015)], Cotesia vestalis (Haliday) [previously misidentified as C. ruficrus (Haliday) by Papp (2015)], Dolichogenidea britannica (Wilkinson), Homolobus (Phylacter) meridionalis van Achterberg, Iconella ? meruloides (Nixon), Lysitermus tritoma (Boucek), Lysitermus suecius (Hedqvist), Microgaster messoria Haliday, Meteorus pulchricornis (Wesmael), Pholetesor circumscriptus (Nees) [previously misidentified as P. bicolor (Nees) by Papp (2015)] and Spathius pedestris Wesmael. Thus previous records of Clinocentrus exsertor and Pholetesor bicolor from Malta were found to be based on misidentifications and are here excluded from the braconid fauna of Malta. Maltese records of Cotesia abjecta (Marshall) and Cotesia jucunda (Marshall) by Papp (2015) were found to be misidentifications and should both refer to C. glomerata (Linnaeus). Thus, both Cotesia abjecta and Cotesia jucunda are also here removed from the braconid fauna of Malta. The record of Cotesia tibialis (Curtis) by Papp (2015) was also based on a misidentification and should be attributed to C. ruficrus (Haliday). Thus, C. tibialis is also removed from the braconid fauna of Malta.

The changing use of the ovipositor in host shifts by ichneumonid ectoparasitoids of spiders (Hymenoptera, Ichneumonidae, Pimplinae).

Accurate egg placement into or onto a living host is an essential ability for many parasitoids, and changes in associated phenotypes, such as ovipositor morphology and behaviour, correlate with significant host shifts. Here, we report that in the ichneumonid group of koinobiont spider-ectoparasitoids ("polysphinctines"), several putatively ancestral taxa (clade I here), parasitic on ground-dwelling RTA-spiders (a group characterised by retrolateral tibial apophysis on male palpal tibiae), lay their eggs in a specific way. They tightly bend their metasoma above the spider's cephalothorax, touching the carapace with the dorsal side of the ovipositor apically ("dorsal-press"). The egg slips out from the middle part of the ventral side of the ovipositor and moves towards its apex with the parted lower valves acting as rails. Deposition occurs as the parasitoid draws the ovipositor backwards from under the egg. Oviposition upon the tough carapace of the cephalothorax, presumably less palatable than the abdomen, is conserved in these taxa, and presumed adaptive through avoiding physical damage to the developing parasitoid. This specific way of oviposition is reversed in the putatively derived clade of polysphinctines (clade II here) parasitic on Araneoidea spiders with aerial webs, which is already known. They bend their metasoma along the spider's abdomen, grasping the abdomen with their fore/mid legs, pressing the ventral tip of the metasoma and the lower valves of the ovipositor against the abdomen ("ventral-press"). The egg is expelled through an expansion of the lower valves, which is developed only in this clade and evident in most species, onto the softer and presumably more nutritious abdomen.

Checklist of British and Irish Hymenoptera - Braconidae.

BACKGROUND: The checklist of British and Irish Braconidae is revised, based in large part on the collections of the National Museums of Scotland, Edinburgh, and the Natural History Museum, London. Distribution records are provided at the country level together with extensive synonymy and bibliography. NEW INFORMATION: Of the 1,338 species regarded as valid, presumed native and certainly identified, 83 are here recorded for the first time from the British Isles. One new synonym is established (Dyscritus suffolciensis Morley, 1933 = Syntretus splendidus (Marshall, 1887) syn. nov.).

Revision of the western Palaearctic species of Aleiodes Wesmael (Hymenoptera, Braconidae, Rogadinae). Part 1: Introduction, key to species groups, outlying distinctive species, and revisionary notes on some further species.

Seven new species of the genus Aleiodes Wesmael, 1838 (Braconidae: Rogadinae) are described and illustrated: Aleiodes abraxanaesp. n., Aleiodes angustipterussp. n., Aleiodes artesiariaesp. n., Aleiodes carminatussp. n., Aleiodes diarsianaesp. n., Aleiodes leptofemursp. n., and Aleiodes ryrholmisp. n. A neotype is designated for each of Aleiodes circumscriptus (Nees, 1834) and Aleiodes pictus (Herrich-Schäffer, 1838), and both species are redescribed and illustrated. Aleiodes ochraceus Hellén, 1927 (not Aleiodes ochraceus (Curtis, 1834)) is renamed as Aleiodes curticornisnom. n. & stat. rev., and redescribed and illustrated. Aleiodes bistrigatus Roman, 1917, Aleiodes nigriceps Wesmael, 1838, and Aleiodes reticulatus (Noskiewicz, 1956), are re-instated as valid species. A lectotype is designated for Aleiodes bistrigatus Roman. An illustrated key is given to some distinctive species and the residual species groups along which further parts of an entire revision of western Palaearctic species of Aleiodes and Heterogamus will be organised. Biology, host associations and phenology are discussed for the keyed species (in addition to the above, Aleiodes albitibia (Herrich-Schäffer, 1838), Aleiodes apiculatus (Fahringer, 1932), Aleiodes arcticus (Thomson, 1892), Aleiodes cantherius (Lyle, 1919), Aleiodes esenbeckii (Hartig, 1834), Aleiodes jakowlewi (Kokujev, 1898), Aleiodes modestus (Reinhard, 1863), Aleiodes nigricornis Wesmael, 1838, Aleiodes pallidator (Thunberg, 1822), Aleiodes praetor (Reinhard, 1863), Aleiodes seriatus (Herrich- Schäffer, 1838) sensu lato, Aleiodes testaceus (Telenga, 1941), Aleiodes ungularis (Thomson, 1892), and Aleiodes varius (Herrich-Schäffer, 1838)) which are dealt with in full here (with the exception of Aleiodes seriatuss.l. which is, however, included in the key). The experimental methodology covering the revision as a whole, which involves some behavioural investigation, is outlined.

Determinants of parasitoid communities of willow-galling sawflies: habitat overrides physiology, host plant and space.

Studies on the determinants of plant-herbivore and herbivore-parasitoid associations provide important insights into the origin and maintenance of global and local species richness. If parasitoids are specialists on herbivore niches rather than on herbivore taxa, then alternating escape of herbivores into novel niches and delayed resource tracking by parasitoids could fuel diversification at both trophic levels. We used DNA barcoding to identify parasitoids that attack larvae of seven Pontania sawfly species that induce leaf galls on eight willow species growing in subarctic and arctic-alpine habitats in three geographic locations in northern Fennoscandia, and then applied distance- and model-based multivariate analyses and phylogenetic regression methods to evaluate the hierarchical importance of location, phylogeny and different galler niche dimensions on parasitoid host use. We found statistically significant variation in parasitoid communities across geographic locations and willow host species, but the differences were mainly quantitative due to extensive sharing of enemies among gallers within habitat types. By contrast, the divide between habitats defined two qualitatively different network compartments, because many common parasitoids exhibited strong habitat preference. Galler and parasitoid phylogenies did not explain associations, because distantly related arctic-alpine gallers were attacked by a species-poor enemy community dominated by two parasitoid species that most likely have independently tracked the gallers' evolutionary shifts into the novel habitat. Our results indicate that barcode- and phylogeny-based analyses of food webs that span forested vs. tundra or grassland environments could improve our understanding of vertical diversification effects in complex plant-herbivore-parasitoid networks.

A new Australian genus and five new species of Rogadinae (Hymenoptera: Braconidae), one reared as a gregarious endoparasitoid of an unidentified limacodid (Lepidoptera) .

Teresirogas Quicke & Shaw gen. nov. (type species T. australicolorus Quicke & Shaw sp. nov.) is described and illustrated, based on a series recently reared gregariously from a cocooned mummy of an unidentified species of Limacodidae collected under loose Eucalyptus bark in New South Wales, Australia. Older reared and unreared congeneric specimens represent four additional species, T. billbrysoni Quicke & van Achterberg sp. nov., T. nolandi Quicke & Butcher sp. nov., T. prestonae Quicke & van Achterberg sp. nov., and T. williamsi Quicke & van Achterberg sp. nov., which are also described and illustrated. Three of these additional species have also been reared from Limacodidae cocoons on Eucalyptus, with one, perhaps erroneous, record suggesting a saturniid host. Molecular analysis confirms the placement of the new type species of Teresirogas in the tribe Rogadini, as inferred initially from the claws with pointed basal lobe and host relationships of some of the species, but one species has the claw character poorly developed which had made its affinities uncertain before the more recently reared and sequenceable material became available.

Biology, early stages and description of a new species of Adelognathus Holmgren (Hymenoptera: Ichneumonidae: Adelognathinae).

Adelognathus leucotrochi Shaw & Wahl sp. nov. is described from Britain where it is a univoltine slightly gregarious koinobiont ectoparasitoid of late stage larvae of the tenthredinid sawfly Nematus leucotrochus Hartig feeding on Ribes uva-crispa. Defensive reactions by the host to prospecting females are described. The developmental biology of A. leucotrochi is described in detail: the host is only temporarily paralysed by the injection of a venom that has no other effect on the host, and eggs are laid on the host's dorsum without involvement of the ovipositor-that is, the egg issues direct from the genital opening. Prior to oviposition the adult female parasitoid prepares the site by spreading an adhesive substance from her ovipositor. Host-feeding by adult females occurs on haemolymph and sometimes also other tissues obtained at the site of a wound made always by the mandibles, but appears not to be obligatory. It may be concurrent or non-concurrent with oviposition; in the latter case, it may be either destructive or non-destructive. Larval development is very rapid, taking about 70 hr at 18-22ºC, and the host continues to feed for approximately the first half of this period. Five larval instars were detected, and their cephalic sclerites are described and illustrated, as are those of the final instars of a further three species of Adelognathus for comparison. The rather featureless final instar larva is also figured, as is the tough cocoon in which the winter is passed as a prepupa. The biology of some idiobiont Adelognathus species is discussed in comparison with that of A. leucotrochi, and several other instances of eggs not issuing from the ovipositor in non-aculeate ectoparasitoid Hymenoptera, whether koinobionts or idiobionts, are briefly reviewed. It is concluded that this habit seems to arise rather easily when there is direct bodily contact between the adult and the host/prey, as indeed is the case in all carnivorous aculeates that do not practice continuous provisioning. 

Wolbachia and DNA barcoding insects: patterns, potential, and problems.

Wolbachia is a genus of bacterial endosymbionts that impacts the breeding systems of their hosts. Wolbachia can confuse the patterns of mitochondrial variation, including DNA barcodes, because it influences the pathways through which mitochondria are inherited. We examined the extent to which these endosymbionts are detected in routine DNA barcoding, assessed their impact upon the insect sequence divergence and identification accuracy, and considered the variation present in Wolbachia COI. Using both standard PCR assays (Wolbachia surface coding protein--wsp), and bacterial COI fragments we found evidence of Wolbachia in insect total genomic extracts created for DNA barcoding library construction. When >2 million insect COI trace files were examined on the Barcode of Life Datasystem (BOLD) Wolbachia COI was present in 0.16% of the cases. It is possible to generate Wolbachia COI using standard insect primers; however, that amplicon was never confused with the COI of the host. Wolbachia alleles recovered were predominantly Supergroup A and were broadly distributed geographically and phylogenetically. We conclude that the presence of the Wolbachia DNA in total genomic extracts made from insects is unlikely to compromise the accuracy of the DNA barcode library; in fact, the ability to query this DNA library (the database and the extracts) for endosymbionts is one of the ancillary benefits of such a large scale endeavor--which we provide several examples. It is our conclusion that regular assays for Wolbachia presence and type can, and should, be adopted by large scale insect barcoding initiatives. While COI is one of the five multi-locus sequence typing (MLST) genes used for categorizing Wolbachia, there is limited overlap with the eukaryotic DNA barcode region.

Utility of the DNA barcoding gene fragment for parasitic wasp phylogeny (Hymenoptera: Ichneumonoidea): data release and new measure of taxonomic congruence.

The enormous cytochrome oxidase subunit I (COI) sequence database being assembled from the various DNA barcoding projects as well as from independent phylogenetic studies constitutes an almost unprecedented amount of data for molecular systematics, in addition to its role in species identification and discovery. As part of a study of the potential of this gene fragment to improve the accuracy of phylogenetic reconstructions, and in particular, exploring the effects of dense taxon sampling, we have assembled a data set for the hyperdiverse, cosmopolitan parasitic wasp superfamily Ichneumonoidea, including the release of 1793 unpublished sequences. Of approximately 84 currently recognized Ichneumonoidea subfamilies, 2500 genera and 41,000 described species, barcoding 5'-COI data were assembled for 4168 putative species-level terminals (many undescribed), representing 671 genera and all but ten of the currently recognized subfamilies. After the removal of identical and near-identical sequences, the 4174 initial sequences were reduced to 3278. We show that when subjected to phylogenetic analysis using both maximum likelihood and parsimony, there is a broad correlation between taxonomic congruence and number of included sequences. We additionally present a new measure of taxonomic congruence based upon the Simpson diversity index, the Simpson dominance index, which gives greater weight to morphologically recognized taxonomic groups (subfamilies) recovered with most representatives in one or a few contiguous groups or subclusters.

Evolution of the parasitic wasp subfamily Rogadinae (Braconidae): phylogeny and evolution of lepidopteran host ranges and mummy characteristics.

BACKGROUND: The braconid subfamily Rogadinae is a large, cosmopolitan group of endoparasitoid wasps characterised by 'mummifying' their lepidopteran host larvae, from which the adult subsequently emerges. Rogadines attack a variety of both macro- and microlepidopteran taxa, although the speciose genus Aleiodes almost exclusively attacks macrolepidopterans. Here, we investigate the phylogenetic history of the Rogadinae, revise their higher-level classification and assess the evolution of their host ranges and mummy types. We also assess the divergence times within the subfamily and discuss the reasons for the extraordinary evolutionary diversification of Aleiodes. RESULTS: Our Bayesian analyses weakly support the monophyly of the subfamily. A clade comprising all Aleiodes species and some other taxa is not nested within the tribe Rogadini as previously supposed, but instead is recovered as sister to the Yeliconini, with the remaining Rogadini genera being recovered as sister to the Stiropiini. The Rogadinae is estimated to have originated during the mid to late Eocene, 36.1-51.62 MYA. Molecular dating gives a more recent origin for the Aleiodes clade (17.98-41.76 MYA) compared to the origins proposed for two of its principal lepidopteran host groups (Noctuidae: 60.7-113.4 MYA; Geometridae 48-62 MYA). The Bayesian ancestral reconstruction of the emergence habits from the mummified hosts weakly recovered an anterior emergence as the ancestral condition for the subfamily. Producing a hard mummy has evolved at various times independently, though most of the species with this biology belong to the Aleiodes clade. CONCLUSION: Based on our results, we erect the tribe Aleiodini nov. to include Aleiodes and Heterogamus stat. rev. Cordylorhogas, Pholichora and Hemigyroneuron are synonymised with Aleiodes. The molecular dating of clades and the ancestral reconstruction of host ranges support the hypothesis that radiation within Aleiodes s. s. was due to host recruitment leading to host range expansion followed by speciation, and not to parasitoid-host coevolution. Within the Rogadinae, variation in the site of emergence from the mummified host probably evolved as a consequence of the mummy's site and mode of formation, and the extent of mummy tanning/hardness to the degree of protection needed in relation to the cost of providing it.

Molecular phylogeny of Cotesia Cameron, 1891 (Insecta: Hymenoptera: Braconidae: Microgastrinae) parasitoids associated with Melitaeini butterflies (Insecta: Lepidoptera: Nymphalidae: Melitaeini).

Phylogenetic relationships among Cotesia Cameron (Braconidae) species parasitising Melitaeini butterflies were examined using DNA sequence data (mitochondrial cytochrome oxidase subunit I and NADH1 dehydrogenase genes, nuclear ribosomal DNA internal transcribed spacer region) as well as 12 microsatellite loci. Molecular data were available from ostensibly six species of Cotesia from 16 host butterfly species in Europe, Asia, and North America. Analysis of the combined sequence data using both maximum parsimony and maximum likelihood revealed two distinct Cotesia clades. In one clade (C. acuminata (Reinhard); C. bignellii (Marshall)) host ranges are apparently narrow and, although Euphydryas (s. lato) is well-utilised, permeation of Melitaea (s. lato) has been slight. In the other clade (C. melitaearum (Wilkinson); C. lycophron (Nixon); C. cynthiae (Nixon)) host utilization across the Melitaeini as a whole is more extensive and the data are consistent with more recent, or active, speciation processes. Neighbour-joining trees calculated separately for the two main clades based on chord distance (DCE) of microsatellite allele frequencies were consistent with phylogenetic trees obtained from the sequence data. Our analysis strongly suggests the presence of several additional, previously unrecognised, Cotesia species parasitising this group of butterflies.