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opennotspecifiedNov 2017View details →

Distribution. Now restricted to the Channel Country of SW Queensland and the Lake Eyre Basin in NE South Australia. Descriptive notes. Head-body 95-120 mm, tail 105-160 mm, ear 23-29 mm, hindfoot 32-37 mm; weight 30-50 g. The Fawn Hopping Mouse has body form typical of hopping mice, with very long hindfeet, long tail with distal brush of longer hairs, very long ears, and large protruberant eyes. Dorsal fur is of variable color, from pale pinkish fawn to gray; ventral fur white. Unlike most other hopping mice, it has no throat pouch, but males have a glandular area of naked skin on the chest. Habitat. Occurs in low shrublands and tussock grasslands on stony ("gibber") plains and claypans. Shows marked habitat segregation from the Dusky Hopping Mouse (N. fuscus), which is closely associated with sandy substrates. Food and Feeding. The Fawn Hopping Mouse is mostly granivorous, but also eats other plant material (stems, leaves) and occasionally invertebrates. It uses succulent, salt-adapted plants around edges of claypans as a source of water. Breeding. Reproduction is probably largely opportunistic and aseasonal, with high reproductive output from near-continuous breeding after periods of high rainfall; reported littersize is 1-5, most commonly three; gestation period 38-43 days for nonlactating females. Females may mature later than other hopping mice, with reproductive maturity reached at about six months. Activity patterns. Terrestrial and nocturnal. Fawn Hopping Mice shelter during day in burrow systems that are typically simpler and shallower than those of other hopping mice. Movements, Home range and Social organization. Fawn Hopping Mice generally live singly or in small groups; typically uncommon within range, but population density may increase by an order of magnitude following periods of high rainfall. Status and Conservation. Classified as Near Threatened on The IUCN Red List. The Fawn Hopping Mouse has shown marked decline in range (estimated at greater than 50%), and presumably population size, since European settlement of Australia. This is mostlikely due to predation by the introduced house cat and Red Fox (Vulpes vulpes), and to habitat degradation associated with pastoralism. Bibliography. Brazenor (1934), Burbidge et al. (2008), Finlayson (1939), Gould (1853), Jackson & Groves (2015), Murray et al. (1999), Ogilby (1892), Thomas (1921h), Van Dyck & Strahan (2008), Waite (1898), Watts & Aslin (1981), Woinarski et al. (2014), Wood Jones (1925). in Muridae

Distribution. Now restricted to the Channel Country of SW Queensland and the Lake Eyre Basin in NE South Australia. Descriptive notes. Head-body 95-120 mm, tail 105-160 mm, ear 23-29 mm, hindfoot 32-37 mm; weight 30-50 g. The Fawn Hopping Mouse has body form typical of hopping mice, with very long hindfeet, long tail with distal brush of longer hairs, very long ears, and large protruberant eyes. Dorsal fur is of variable color, from pale pinkish fawn to gray; ventral fur white. Unlike most other hopping mice, it has no throat pouch, but males have a glandular area of naked skin on the chest. Habitat. Occurs in low shrublands and tussock grasslands on stony ("gibber") plains and claypans. Shows marked habitat segregation from the Dusky Hopping Mouse (N. fuscus), which is closely associated with sandy substrates. Food and Feeding. The Fawn Hopping Mouse is mostly granivorous, but also eats other plant material (stems, leaves) and occasionally invertebrates. It uses succulent, salt-adapted plants around edges of claypans as a source of water. Breeding. Reproduction is probably largely opportunistic and aseasonal, with high reproductive output from near-continuous breeding after periods of high rainfall; reported littersize is 1-5, most commonly three; gestation period 38-43 days for nonlactating females. Females may mature later than other hopping mice, with reproductive maturity reached at about six months. Activity patterns. Terrestrial and nocturnal. Fawn Hopping Mice shelter during day in burrow systems that are typically simpler and shallower than those of other hopping mice. Movements, Home range and Social organization. Fawn Hopping Mice generally live singly or in small groups; typically uncommon within range, but population density may increase by an order of magnitude following periods of high rainfall. Status and Conservation. Classified as Near Threatened on The IUCN Red List. The Fawn Hopping Mouse has shown marked decline in range (estimated at greater than 50%), and presumably population size, since European settlement of Australia. This is mostlikely due to predation by the introduced house cat and Red Fox (Vulpes vulpes), and to habitat degradation associated with pastoralism. Bibliography. Brazenor (1934), Burbidge et al. (2008), Finlayson (1939), Gould (1853), Jackson & Groves (2015), Murray et al. (1999), Ogilby (1892), Thomas (1921h), Van Dyck & Strahan (2008), Waite (1898), Watts & Aslin (1981), Woinarski et al. (2014), Wood Jones (1925).

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Data from: Root inoculation with beneficial soil microbes enhances indirect plant defenses induced by insect feeding and egg deposition

Plants can respond to insect egg deposition by emitting oviposition-induced plant volatiles (OIPVs) recruiting parasitoids. The recruitment of carnivore insects in response to egg deposition is considered an indirect defense strategy that is widespread in the plant kingdom. In recent years, there has been increasing evidence showing that microbial colonization can influence the strength of plant responses to insect herbivory, yet no information is available on how beneficial microbes modulate indirect defenses induced by insect egg deposition. In this work, we evaluated the effects of inoculation with the beneficial soil fungus Trichoderma harzianum strain T22 on a tritrophic system consisting of tomato, the southern green stink bug Nezara viridula and its associated egg parasitoid Trissolcus basalis. We used Y-tube olfactometer assays to evaluate the behavioral responses of the parasitoids to OIPVs emitted by plants colonized with beneficial soil microbes. We also used gas chromatography coupled with mass spectrometry (GC-MS) to investigate how root inoculation with T. harzianum T22 affects the chemical composition of induced plant volatiles. 3. In olfactometer assays, we found that root inoculation with T. harzianum T22 enhanced the attraction of the egg parasitoid towards tomato plants induced by N. viridula feeding and oviposition activities. In particular, the egg parasitoid preferred OIPVs emitted by tomato plants previously inoculated with T. harzianum T22 over OIPVs emitted by non-inoculated plants. Furthermore, chemical analysis showed that root inoculation with T. harzianum T22 resulted in changes in the composition of OIPVs, which was consistent with the behavioral observations. Among the compounds that strongly contribute to the chemical differences between OIPVs from non-inoculated and inoculated plants, chemical analysis identified green leaf volatiles ((Z)-3-hepten-1-ol, (E,E)-2,4-hexadienal), along with terpenoids (terpinen 4-ol, α-tujene and δ-elemene). 4. Taken together our results indicate that beneficial soil microbes enhance indirect plant defenses induced by feeding and oviposition, broadening our understanding of plant responses to insect eggs. Our results underscore the importance of taking into account the role of microorganisms to fully comprehend the intricate interactions among plants, herbivore eggs and their associated egg parasitoids.

opencc-zeroMay 2024View details →

FIGURES 1–8 in New Mycodiplosis gall midge (Diptera: Cecidomyiidae) feeding on fungal rusts (Fungi: Pucciniomycetes) that are pathogenic on cultured plants

FIGURES 1–8. Mycodiplosis puccinivora. Male. (1) occipital protuberance on head dorsally, (2) 3rd flagellomere (3) mouth parts, (4) fore claw, (5) mid claw, (6) hind claw, (7) terminalia dorsally, (8) terminalia ventrally.

FIGURES 19–27 in New Mycodiplosis gall midge (Diptera: Cecidomyiidae) feeding on fungal rusts (Fungi: Pucciniomycetes) that are pathogenic on cultured plants

FIGURES 19–27. Mycodiplosis puccinivora feeding on fungal rust Maravalia pterocarpi infesting leaves of Dalbergia tonkinensis. 19–20: adult, 21: egg, 22–24: larva, 25–27: pupa. (19) female, (20) male, (21) egg on leaf surface, (22) mature larva spinning cocoon on leaf surface, (23) larvae feeding on uredinia, (24) larvae feeding on uredinia, arows indiacte larave in the distance, (25) young pupa, (26) mature pupa, (27) pupal exhiviae anchored in cocoon following emergence of adult. Fig. 24 is from Wang et al. (2017).

FIGURES 14–18. Mycodiplosis puccinivora. 14–17 in New Mycodiplosis gall midge (Diptera: Cecidomyiidae) feeding on fungal rusts (Fungi: Pucciniomycetes) that are pathogenic on cultured plants

FIGURES 14–18. Mycodiplosis puccinivora. 14–17: larva, 18: pupal exhuviae. (14) head in dorsal view, (15) sternal spatula with adjacent papillae, (16) terminal segment in dorsal view, (17, 18) habitus.

FIGURES 9–13 in New Mycodiplosis gall midge (Diptera: Cecidomyiidae) feeding on fungal rusts (Fungi: Pucciniomycetes) that are pathogenic on cultured plants

FIGURES 9–13. Mycodiplosis puccinivora. Female. (9) 3rd flagellomere, (10) wing, (11) hypoproct ventrally, (12) postabdomen from 7th segment to end dorsally, (13) postabdomen from 7th segment to end laterally.

Fig. 8 in What do Eumerus Meigen larvae feed on? New immature stages of three species (Diptera: Syrphidae) breeding in different plants

Fig. 8 "Bipartite" network between Eumerus species (right) and the genera of host plants (left). Length of the boxes show the number of interactions. Colors of the plant boxes: in red (dark color), genera with at least one species with economic value; in blue (light color), without economic value. Plant genera followed by plant family abbreviations as in Table 1

Fig. 4 in What do Eumerus Meigen larvae feed on? New immature stages of three species (Diptera: Syrphidae) breeding in different plants

Fig. 4 Anterior spiracles (AS) of Eumerus larvae and puparia, apicoventral view. a Eumerus alpinus, puparium; SEM. b Eumerus figurans, larva; stereo microscope. c Eumerus superbus, puparium; SEM. O spiracular opening. Scale lines: a = 50 μm; b = 200 μm; c = 100 μm

Fig. 1 in What do Eumerus Meigen larvae feed on? New immature stages of three species (Diptera: Syrphidae) breeding in different plants

Fig. 1 General shape of Eumerus puparia, dorsal view. a Eumerus alpinus. b Eumerus superbus. Scale lines: a and b = 2 mm

Fig. 3 in What do Eumerus Meigen larvae feed on? New immature stages of three species (Diptera: Syrphidae) breeding in different plants

Fig. 3 Head skeletons of Eumerus, lateral view. a Eumerus alpinus. b Eumerus figurans. c Eumerus superbus. D dorsal cornu, L mandibular lobe, M mandibular hook, P pharyngeal ridges, T accessory tooth, V ventral cornu. Scale lines = 250 μm

Fig. 7 in What do Eumerus Meigen larvae feed on? New immature stages of three species (Diptera: Syrphidae) breeding in different plants

Fig. 7 Total count of described early stages of Eumerus (triangles) and total count of known life cycles of early stages of Eumerus species (squares) by the first time a host-plant interaction was reported. X-axis shows years. Y-axis, number of Eumerus species

Fig. 6 in What do Eumerus Meigen larvae feed on? New immature stages of three species (Diptera: Syrphidae) breeding in different plants

Fig. 6 Posterior respiratory processes (PRP) of Eumerus larvae and puparia in dorsal view (left) and polar view (right). a, b Eumerus alpinus, puparium; SEM. c, d Eumerus figurans, larva; stereo microscope. e, f Eumerus superbus, puparium; SEM. α distance from the transverse ridge to the center of the spiracular plate, β width of the PRP at the transverse ridge level, C* spiracular scar, O spiracular opening, R transverse ridge, S spiracular seta. Scale lines: a and e = 500 μm; b and c = 250 μm; d = 100 μm; f = 200 μm

Fig. 5 in What do Eumerus Meigen larvae feed on? New immature stages of three species (Diptera: Syrphidae) breeding in different plants

Fig. 5 Pupal spiracles (PS) of Eumerus puparia (left) and details of the tubercles bearing spiracular openings (right). a, b Eumerus alpinus. c, d Eumerus superbus. O spiracular opening. Scale lines: a = 100 μm; b and d = 50 μm; c = 250 μm

Fig. 9 in What do Eumerus Meigen larvae feed on? New immature stages of three species (Diptera: Syrphidae) breeding in different plants

Fig. 9 Feeding network between larvae of Eumerus species (left, in gray) and plant tissues they feed on (right, colored) based on the interactions historically reported in bibliography for different genera of plants. Links between sides indicate relationships. Scales on each segment show the number of interactions established with the counter side. Plant tissue color palette as follows: tuber (yellow), swollen root (orange), rhizome (brown), processed material (black), fruits (red), stem (light green), corm (purple), cone (pink), and bulb (blue). Picture made using "circlize" package for R software

opencc-by-4.0Sep 2024View details →

Effects of a plant-based diet from first feeding on the intestinal expression of nutrient sensors in rainbow trout

Raw data corresponding to results included in the above mentioned publication

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Data from: Match and mismatch between dietary switches and microbial partners in plant sap-feeding insects

Some animal groups associate with the same vertically-transmitted microbial symbionts over extended periods of evolutionary time, punctuated by occasional symbiont switches to different microbial taxa. Here we test the oft-repeated suggestion that symbiont switches are linked with host diet changes, focusing on hemipteran insects of the suborder Auchenorrhyncha. These insects include the only animals that feed on plant xylem sap through the life cycle, as well as taxa that feed on phloem sap and plant parenchyma cells. Ancestral state reconstruction provides strong statistical support for a xylem-feeding auchenorrhynchan ancestor bearing the dual symbiosis with the primary symbiont Sulcia (Bacteroidetes) and companion symbiont "β-Sym" (β-proteobacteria). We identified 7 dietary transitions from xylem-feeding (six to phloem-feeding, one to parenchyma-feeding), but no reversions to xylem-feeding; five evolutionary losses of Sulcia, including replacements by yeast symbionts, exclusively in phloem/parenchyma-feeding lineages; and 14-15 losses of β-Sym, including 9 transitions to a different bacterial companion symbiont. Our analysis indicates that, although companion symbiont switching is not associated with shifts in host diet, Sulcia is likely required for xylem-feeding. Furthermore, the ancestral auchenorrhynchan bearing Sulcia and β-Sym likely represents the sole evolutionary origin of xylem feeding in the animal kingdom.

opencc-zeroDec 2018View details →

opencc-by-4.0Sep 2021View details →

Datasets from Benhamou et al.: Cytotype conditions capability to feed and oviposit of the whitefly Bemisia tabaci (Hemiptera: Aleyrodidae) MED species on an unfavorable host plant

This excel file contains all datasets generated analyzed in this study.

opennotspecifiedSep 2021View details →

FIGURES 70–73 in Most trumpet moths don't feed on plants of the nettle family but Paratischeria does: the first discovery of Tischeriidae (Lepidoptera) on Urticaceae in Asia

FIGURES 70–73. Female genitalia of Paratischeria grossa Diškus & Stonis, sp. nov., paratype, genitalia slide no. AD1059 (ZIN).

opennotspecifiedSep 2021View details →

FIGURES 62–69 in Most trumpet moths don't feed on plants of the nettle family but Paratischeria does: the first discovery of Tischeriidae (Lepidoptera) on Urticaceae in Asia

FIGURES 62–69. Male genitalia of Paratischeria grossa Diškus & Stonis, sp. nov., dissected genitalia capsules of paratypes. 62–64, tegumen and uncus, genitalia slide no. AD1067 (NRC); 65, socii, genitalia slide no. AD1037 (GNU); 66, 67, details of genitalia, slide no. AD1067 (NRC); 68, genitalia slide no. AD1037, uncus, tegumen, and dorsal sclerite (GNU); 69, same, val- vae, anellus, and vinculum (GNU)