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271 results for “introduced species”
Figure 3 in The conservation paradox of an introduced population of a threatened species: spadefoot toads in the coastal dunes of the Netherlands
Figure 3. Haplotype network for the common spadefoot toad (Pelobates fuscus) Haplotypes relevant to the current study are colour coded; the remainder is left grey (details in supplementary table S1). The prefix 'FUS' is not shown for the haplotype codes.
Figure 2 in The conservation paradox of an introduced population of a threatened species: spadefoot toads in the coastal dunes of the Netherlands
Figure 2. Phylogenetic tree for common spadefoot toad (Pelobates fuscus) and Pallas's spadefoot toad (P. vespertinus). Haplotypes relevant to the current study are colour coded; the remainder is left grey (details in Table S1). Haplotype abbreviations are: FUS = P. fuscus, VES = P. vespertinus, BAL = P. balcanicus, SYR = P. syriacus, CUL = P. cultripes, and VAR = P. varaldii.
FIGURE 3 in Splanchnonema-like species in Pleosporales: introducing Pseudosplanchnonema gen. nov. in Massarinaceae
FIGURE 3. Asexual morph of Pseudosplanchnonema phorcioides (MFLUCC 13-0533). A. Conidiomata on the PDA, B. Conidiogenous cells, C. Conidia, D. Upper-view (right) and the reverse view (left) of the colony on PDA. Scale bars: A= 200 μm, B= 3 μm, C= 5 μm.
FIGURE 2 in Splanchnonema-like species in Pleosporales: introducing Pseudosplanchnonema gen. nov. in Massarinaceae
FIGURE 2. Pseudosplanchnonema phorcioides (MFLUCC 13-0533). A. Pseudostroma immersed in the host tissue, B. Section of the ascoma (TS), C. Section of the peridium, D. Hyaline, pseudoparaphyses, E. Immature ascus, F–G. Mature asci, H–J. Brown ascospores, K. Ascospore with a gelatinous sheath stained in Indian ink, I. Germinating ascospore. Scale bars: A= 1 mm, B= 500 μm, C= 20 μm, D= 10 μm, E–G= 20 μm, H= 20 μm, I–L= 10 μm.
FIGURE 1 in Splanchnonema-like species in Pleosporales: introducing Pseudosplanchnonema gen. nov. in Massarinaceae
FIGURE 1. Phylogram generated from Maximum Likelihood analysis based on combined SSU and LSU gene dataset. Bootstrap support values for maximum parsimony (MP) and maximum likelihood (ML) greater than 50 % are indicated near the nodes and branches with Bayesian posterior probabilities above 0.90 are indicated in bold. The tree is rooted with Aigialus grandis (BCC 18419). The ex-types strains are in bold and the species introduced in the study are indicated in blue.
FIGURE 4 in Introducing Dictyochaeta aquatica sp. nov. and two new species of Chloridium (Chaetosphaeriaceae, Sordariomycetes) from aquatic habitats
FIGURE 4. Dictyochaeta aquatica (holotype, MFLU 15-2691). a. Colonies on substrate. b–d. Conidiophores and setae. e–h. Conidiogenous cells. i–q. Conidia with appendages. r. Germinating Conidium. s–t. Culture on PDA. Bars: b–d = 20 μm, e–h = 5 μm, i–r = 10 μm.
FIGURE 3 in Introducing Dictyochaeta aquatica sp. nov. and two new species of Chloridium (Chaetosphaeriaceae, Sordariomycetes) from aquatic habitats
FIGURE 3. Chloridium aquaticum (holotype, MFLU 11-1133). a–b. Colonies on substrate. c. Conidiophore. Note the percurrent proliferation. d–f. Conidiogenous cells. g. Colonies on PDA. h–i. Conidia. Bars: a–b = 150 μm, c = 50 μm, d–f = 30 μm, h–i = 5 μm.
FIGURE 1 in Introducing Dictyochaeta aquatica sp. nov. and two new species of Chloridium (Chaetosphaeriaceae, Sordariomycetes) from aquatic habitats
FIGURE 1. RAxML tree generated based on combined ITS and LSU sequence data of the family Chaetosphaeriaceae. Bootstrap support values for maximum likelihood (ML, red) and maximum parsimony (MP, green) equal to or greater than 50% are given above the nodes. Bayesian bootstrap value equal or higher than 90% are indicated on the branch with dot. Newly generated sequences are indicated in blue. The ex-type isolates are in bold. The tree is rooted to Jobellisia luteola (SMH 2753).
FIGURE 2 in Introducing Dictyochaeta aquatica sp. nov. and two new species of Chloridium (Chaetosphaeriaceae, Sordariomycetes) from aquatic habitats
FIGURE 2. Chloridium aseptatum (holotype, MFLU11-1051). a–b. Colonies on substrate. c. Germinating conidia d. Conidiophores from culture. e–j. Proliferating conidiophores bearing conidia. f. is from culture. k–l. Conidia. m–n. Culture on PDA. Bars: b–d = 50 μm, e = 30 μm, f = 110 μm, g = 25 μm, h = 35 μm, i = 20 μm, j = 30 μm, k–l = 15 μm.
FIGURE 3 in Introducing Ophiocordyceps thanathonensis, a new species of entomogenous fungi on ants, and a reference specimen for O. pseudolloydii
FIGURE 3 Ophiocordyceps pseudolloydii (MFLU 16–2914, reference specimen). a Habitat of Ophiocordyceps pseudolloydii. b Ascostroma emerging from infected ant host. c Fertile head of ascostroma. d Vertical sections showing the completely embedded obliquely aligned perithecia. e Perithecia. f Peridium. g–i Immature to mature asci. j Asci in Indian ink. k Apical cap of ascus. l, m Secondary ascospore. n, o Culture on PDA medium, obverse and reverse view. Scale Bars: b, d–f = 1000 μm, c = 200 μm, g–j = 500 μm, k = 100 μm, l = 20 μm, m = 10 μm, n, o = 20 mm.
FIGURE 2 in Introducing Ophiocordyceps thanathonensis, a new species of entomogenous fungi on ants, and a reference specimen for O. pseudolloydii
FIGURE 2 Ophiocordyceps thanathonensis (MFLU 16–2908, holotype). a Habitat of Ophiocordyceps thanathonensis. b Ascostroma emerging from infected ants. c, d Overview of host. e Fertile head of ascostroma. f Vertical section of the stroma. g, h Ascomata. i Peridium. j–l Immature to mature asci. m Apical cap of asci. n Parts of ascospores. o–q Secondary ascospore. Scale Bars: d–f = 1000 μm, g = 500 μm, h = 200 μm, i–l = 100 μm, m = 10 μm, n = 20 μm, o–q = 5 μm.
FIGURE 1 in Introducing Ophiocordyceps thanathonensis, a new species of entomogenous fungi on ants, and a reference specimen for O. pseudolloydii
FIGURE 1. Phylogenetic tree of Ophiocordyceps thanathonensis and O. pseudolloydii generated from maximum likelihood analysis of ITS, SSU, LSU, RPB1, and TEF1α sequence data. Tolypocladium inflatum and T. ophioglossoides were used as outgroup taxa. Maximum likelihood bootstrap values greater than 75% and Bayesian posterior probabilities over 0.95 are indicated above the nodes. The new species were indicated in blue.he ex-types are indicated in bold. The pathogens of ants are marked with ant drawings.
FIGURE 2 in Introducing the new Indian mangrove species, Vaginatispora microarmatispora (Lophiostomataceae) based on morphology and multigene phylogenetic analysis
FIGURE 2. Vaginatispora microarmatispora (holotype). a–b. Ascomata immersed, aggregated, erumpent on the dead wood of Aegiceras corniculatum. c–d. Longitudinal sections of ascomata e. Ostiole with periphyses. f. Section of peridium comprising inner hyaline to pale brown cells of textura angularis. g. Cellular and hyaline pseudoparaphyses. h–j, l. Immature and matured asci. k. Ascospore with an indistinct mucilaginous sheath and distinct hyaline appendages. m–p. Ascospores with large guttules. o. Ascospore stained in Indian ink. q. Germ tubes developed from terminal ends of ascospore. Scale bars: c–d = 100 μm, e, j, l = 50 μm, f–h, k, m–q = 10 μm.
FIGURE 1 in Introducing the new Indian mangrove species, Vaginatispora microarmatispora (Lophiostomataceae) based on morphology and multigene phylogenetic analysis
FIGURE 1. RAxML tree based on analysis of a combined dataset of LSU, SSU, ITS and TEF partial sequence data. Bootstrap support values for ML, MP higher than 75 % and BYPP greater than 0.95 are given above each branch respectively. The new isolate is in blue. The tree is rooted to Angustimassarina populi (Amorosiaceae).
Data from: Exclusion of introduced deer increases size and seed production success in an island-endemic plant species
The presence of extra-local invaders, such as the southern California mule deer (Odocoileus hemionus) on Santa Catalina Island, may contribute to more selective and insidious effects within the unique ecosystems that have evolved in their absence. Studies at the species level may detect effects not noticed in broader, community level vegetation monitoring or help tease apart differences in the level of effect among the various ecological components of an invaded system. In this initial study, we measured the impacts of herbivory by mule deer, a species native to analogous habitats on the adjacent mainland, on size and seed production success for Crocanthemum greenei (island rush-rose), a federally listed sub-shrub that is not present on mainland California. We found deer exclusion resulted in an overall increase in stem measurement of 18.8 cm. Exclosure populations exhibited complete seed production success, whereas control populations showed significantly reduced success and exhibited complete failure within 58% of populations. These results show that the introduced mule deer on Santa Catalina Island are negatively affecting a federally threatened plant species. This strongly implies that the current deer management strategy is insufficient, if one of its goals is biodiversity and endemic species conservation.
Climatic niche shifts in 815 introduced plant species affect their predicted distributions: Data and scripts
<p class="CxSpFirst"><u>Aim:</u> Introduced species often occupy different climates in their introduced than their native range, but to what degree do such 'climatic niche shifts' interfere with our ability to predict invasions? Answering this question is crucial if we are to understand the threat invasive species pose to human and natural systems, especially given the ever increasing use of species distribution models as tools for invasive species risk assessment and management. Here we investigated how strongly climatic niche shifts interfered with the transferability of native- and introduced-range species distribution models.</p> <p class="CxSpMiddle"><u>Location:</u> Our dataset consisted of ~14 million occurrences distributed worldwide.</p> <p class="CxSpMiddle"><u>Time Period:</u> Occurrence data were collected from online repositories dating from ca. 1600 with the vast majority being from the 20<sup>th</sup> century. Climatic data represent means between 1970–2000.</p> <p class="CxSpMiddle"><u>Major Taxa Studied:</u> Our database represented 815 terrestrial plant species.</p> <p class="CxSpMiddle"><u>Methods:</u> We used ordination to identify climatic niche shifts as species moved between continents. Next, we trained separate MAXENT models using native- or introduced-range occurrences, and projected those models into each species' introduced range. We compared the ordination and MAXENT models to determine whether niche shifts were associated with errors in MAXENT predictions.</p> <p class="CxSpMiddle"><u>Results:</u> Models trained on native-range occurrences poorly predicted introduced-range occurrences, and transferability was lowest in species with large climatic niche shifts. Directional shifts in species' predicted geographic distributions mirrored their niche dynamics. This is concerning because native-range data are often used to predict introduced-range distributions.</p> <p><u>Main Conclusions: </u>Our results highlight the importance of considering niche shifts when modeling the potential geographic distributions of introduced species, and cast doubt on the assumption that the climatic niche of a species can be transferred between native and invasive ranges.</p>
FIGURE. 10 in Spread of the introduced species Laurencia caduciramulosa (Rhodomelaceae, Rhodophyta) to the northwest Atlantic: A morphological and molecular analysis
FIGURE. 10. Phylogenetic relationships in the Laurencia complex based on Bayesian analysis of rbcL DNA sequences. MP bootstrap, ML bootstrap, and Bayesian posterior probability values are indicated at the nodes. Bold lines indicate a fully supported node. Taxa marked in bold indicate newly determined sequences.
FIGURES 3–9. Laurencia caduciramulosa. Fig. 3 in Spread of the introduced species Laurencia caduciramulosa (Rhodomelaceae, Rhodophyta) to the northwest Atlantic: A morphological and molecular analysis
FIGURES 3–9. Laurencia caduciramulosa. Fig. 3. Habit of a plant showing crown of small deciduous branchlets near apices. Note a single discoid holdfast (arrow) (200 µm). Fig. 4. Basal portion of a plant showing secondary discoid holdfast (arrow) (500 µm). Fig. 5. Upper portions of a branch with small branchlets and scars of released branchlets (arrowheads). Note lenticular thickenings throughout the branch (arrows) (100 µm). Fig. 6. Cortical cells in surface view showing one single corp en cerise per cell in living material (25 µm). Fig. 7. Cortical cells in surface view of the mid-portion of a branch showing secondary pit connections (arrow) (25 µm). Fig. 8. Transverse section of a branch showing lenticular thickenings in the wall of medullary cells (50 µm). Fig. 9. Transverse section of the upper portion of a branch showing an axial cell (a) with four pericentral cells (p). Note lenticular thickenings in detail (25 µm).
FIGURE 2 in Spread of the introduced species Laurencia caduciramulosa (Rhodomelaceae, Rhodophyta) to the northwest Atlantic: A morphological and molecular analysis
FIGURE 2. World distribution map of Laurencia caduciramulosa. Sites: 1. Ɨ Vietnam, type locality (Masuda et al. 1997) 2. Malaysia (Masuda et al. 2001). 3. Italy (Furnari et al. 2001). 4. Anambas Islands, Indonesia (Liao et al. 2004). 5. France (Klein & Verlaque 2005). 6. Greece (Tsirika & Haritonidis 2005). 7. Brazil (Cassano et al. 2006). 8. Canary Islands, Spain (Cassano et al. 2008a). 9. Cuba (Sentíes et al. 2010). 10. Brazil (Torrano-Silva & Oliveira 2013). 11. Florida, USA (this study).
Figure 1 in Introduced and cryptogenic marine and estuarine species of South Africa
Figure 1. Biogeographic regions and transition zones of South Africa. Modified after Lombard (2004).
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OpenNeuro
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