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273 results for “parasitic plants”
Fig. 1 in Species Composition And Structure Of The Communities Of Plant-Parasitic And Free-Living Soil Nematodes In The Greenhouses Of Botanical Gardens Of Ukraine
Fig. 1. Dendrogram of similarity of the nematode communities in the greenhouses of botanical gardens of Ukraine (amalgamation by the method of complete linkage). Explanation of the abbreviations is given in table 2. Рис. 1. Дендрограмма сходства нематодных сообществ в оранжереях ботанических садов Украины (объединение по методу полной связи). Расшифровка сокращений дана в таблице 2.
Fig. 2 in Species Composition And Structure Of The Communities Of Plant-Parasitic And Free-Living Soil Nematodes In The Greenhouses Of Botanical Gardens Of Ukraine
Fig. 2. Dendrogram of similarity of plant-parasitic nematodes' communities in the greenhouses of botanical gardens of Ukraine (amalgamation by the method of complete linkage). Explanation of the abbreviations is given in table 2.
Figure 6 in Depth distribution of plant-parasitic nematodes on bentgrass golf greens in Missouri and Indiana
Figure 6: PCR results using Meloidogyne-specific and M. naasi and M. marylandi-specific primers. DL: DNA Ladder; 1: Meloidogyne spp. (DNA ID:9); 2: M. naasi (DNA ID:9); 3: Meloidogyne spp. (DNA ID:4); 4: M. marylandi (DNA ID:4); and 5: Meloidogyne spp.(DNA ID:4).
Figure 3 in Depth distribution of plant-parasitic nematodes on bentgrass golf greens in Missouri and Indiana
Figure 3: PCR results using Hoplolaimus-specific and H. stephanus, H. columbus and H. galeatus-specific primers. DL: DNA Ladder; 1: Hoplolaimus spp. (DNA ID:10); 2: H. stephanus (DNA ID:10); 3: H. columbus (DNA ID:10); 4 H. galeatus (DNA ID:10); 5: Hoplolaimus spp. (DNA ID:3); 6: H. stephanus (DNA ID:3); 7: H. columbus (DNA ID:3); 8 H. galeatus (DNA ID:3); 9: Hoplolaimus spp. (DNA ID:4); 10: H. stephanus (DNA ID:4); 11: H. columbus (DNA ID:4); and 12 H. galeatus (DNA ID:4).
Figure 2 in Depth distribution of plant-parasitic nematodes on bentgrass golf greens in Missouri and Indiana
Figure 2: Phylogeny of the rDNA ITS region of Hoplolaimus spp. isolated from golf putting greens. Phylogenetic trees were constructed with the neighbor-joining algorithm using the Kimura two-parameter model with Litylenchus spp. (LC383724) as the outgroup. Bootstrap values are based on 1000 resamplings of the data set. DNAID codes correlate to Table 2.
Figure 1 in Depth distribution of plant-parasitic nematodes on bentgrass golf greens in Missouri and Indiana
Figure 1: Distribution of plant-parasitic nematode species sampled from creeping bentgrass putting greens in Missouri and eastern Kansas in 2021 and Indiana in 2022 in two independent pie charts. Samples were collected during the months of April, June, August and October of 2021 and 2022, respectively. "n" indicates total PPNs represented within each chart.
Figure 3 in Plant-Parasitic Nematodes and their Effects on Ornamental Plants: A Review
Figure 3: Hot water dipping tank (A) and the interior of the tank (B) at a commercial nursery in Michigan.
Figure 4 in Depth distribution of plant-parasitic nematodes on bentgrass golf greens in Missouri and Indiana
Figure 4: Scanning-electron micrographs of a lance nematode specimen collected form Site 5. A) four lip annules; B) the presence of an epiptygma; C) 25 longitudinal striae on the basal lip annule; and D) four lateral incisures.
Figure 5 in Depth distribution of plant-parasitic nematodes on bentgrass golf greens in Missouri and Indiana
Figure 5: Phylogeny of molecularly characterized Meloidogyne spp. isolated from golf coursed based on D2/D3 28S genes. phylogenetic trees were constructed with the neighborjoining algorithm using the Kimura two-parameter model with Litylenchus spp. (LC383724) as the outgroup. Bootstrap values are based on 1000 resamplings of the data set and displayed near branch nodes. DNAID codes correlate to Table 2.
Figure 2 in Plant-Parasitic Nematodes and their Effects on Ornamental Plants: A Review
Figure 2: Light micrograph of an adult male (A) and head (B) of Aphelenchoides spp. extracted from Heliopsis spp. leaves. Angular lesions (C,D) on the leaves of two varieties of Heliopsis spp. infected with Aphelenchoides spp.
Figure 1 in Plant-Parasitic Nematodes and their Effects on Ornamental Plants: A Review
Figure 1: Light micrograph of Meloidogyne hapla second-stage juvenile (A) extracted from a daylily field at a commercial nursery in Michigan. Daylily roots were taken from the same field showing galling and stunting due to M. hapla infection (B) compared to healthy roots (C).
Figure 3 in Four new records of plant parasitic nematodes from Iran
Figure 3. Criconemoides morgensis: (A) anterior end of the body, (B) ovary, (C) body shape, (D–F) anastomoses, (G, H) variation of the tail.
Figure 4 in Four new records of plant parasitic nematodes from Iran
Figure 4. Paratylenchus vandenbrandei: (A) anterior end of the body, (B) lip region, (C) ovary, (D) body shape, (E, F) variation of the tail, (G) lateral lines with deirid.
Figure 2 in Four new records of plant parasitic nematodes from Iran
Figure 2. Geocenamus dobroticus: (A) anterior end of the body,(B) lip region, (C) ovary, (D) body shape, (E) lateral lines, (F, G) variation of the tail.
Figure 1 in Four new records of plant parasitic nematodes from Iran
Figure 1. Merlinius acuminatus: (A) anterior end of the body, (B) lip region, (C) ovary, (D) body shape, (E) lateral lines, (F, G) variation of the tail.
Linked collectors and determiners for: ARC-PPRI: National Collection of Nematodes and South African Plant-Parasitic Nematode Survey(1901-2014).
Natural history specimen data linked to collectors and determiners held within, "ARC-PPRI: National Collection of Nematodes and South African Plant-Parasitic Nematode Survey(1901-2014)". Claims or attributions were made on Bionomia by volunteer Scribes, <a href="https://bionomia.net/dataset/5edbfe13-c150-43d3-ac38-729b6aeb6147">https://bionomia.net/dataset/5edbfe13-c150-43d3-ac38-729b6aeb6147</a> using specimen data from the dataset aggregated by the Global Biodiversity Information Facility, <a href="https://gbif.org/dataset/5edbfe13-c150-43d3-ac38-729b6aeb6147">https://gbif.org/dataset/5edbfe13-c150-43d3-ac38-729b6aeb6147</a>. Formatted as a Frictionless Data package.
In silico subcellular targeting predictions for cytosolic aminoacyl tRNA-synthetases (aaRS) in parasitic plants
<p>Eukaryotic nuclear genomes often encode distinct sets of protein translation machinery for function in the cytosol vs. organelles (mitochondria and plastids). This phenomenon raises questions about why multiple translation systems are maintained even though they are capable of comparable functions, and whether they evolve differently depending on the compartment where they operate. These questions are particularly interesting in land plants because translation machinery, including aminoacyl-tRNA synthetases (aaRS), is often dual-targeted to both the plastids and mitochondria. These two organelles have quite different metabolisms, with much higher rates of translation in plastids to supply the abundant, rapid-turnover proteins required for photosynthesis. Previous studies have indicated that plant organellar aaRS evolve more slowly compared to mitochondrial aaRS in other eukaryotes that lack plastids. Thus, we investigated the evolution of nuclear-encoded organellar and cytosolic translation machinery across a broad sampling of angiosperms, including non-photosynthetic (heterotrophic) plant species with reduced rates of plastid gene expression to test the hypothesis that translational demands associated with photosynthesis constrain the evolution of bacterial-like enzymes involved in organellar tRNA metabolism. Remarkably, heterotrophic plants exhibited wholesale loss of many organelle-targeted aaRS and other enzymes, even though translation still occurs in their mitochondria and plastids. These losses were often accompanied by apparent retargeting of cytosolic enzymes and tRNAs to the organelles, sometimes preserving aaRS-tRNA charging relationships but other times creating surprising mismatches between cytosolic aaRS and mitochondrial tRNA substrates. Our findings indicate that the presence of a photosynthetic plastid drives the retention of specialized systems for organellar tRNA metabolism.</p>
Organellar tRNAs in parasitic plant species
<p>Eukaryotic nuclear genomes often encode distinct sets of protein translation machinery for function in the cytosol vs. organelles (mitochondria and plastids). This phenomenon raises questions about why multiple translation systems are maintained even though they are capable of comparable functions, and whether they evolve differently depending on the compartment where they operate. These questions are particularly interesting in land plants because translation machinery, including aminoacyl-tRNA synthetases (aaRS), is often dual-targeted to both the plastids and mitochondria. These two organelles have quite different metabolisms, with much higher rates of translation in plastids to supply the abundant, rapid-turnover proteins required for photosynthesis. Previous studies have indicated that plant organellar aaRS evolve more slowly compared to mitochondrial aaRS in other eukaryotes that lack plastids. Thus, we investigated the evolution of nuclear-encoded organellar and cytosolic translation machinery across a broad sampling of angiosperms, including non-photosynthetic (heterotrophic) plant species with reduced rates of plastid gene expression to test the hypothesis that translational demands associated with photosynthesis constrain the evolution of bacterial-like enzymes involved in organellar tRNA metabolism. Remarkably, heterotrophic plants exhibited wholesale loss of many organelle-targeted aaRS and other enzymes, even though translation still occurs in their mitochondria and plastids. These losses were often accompanied by apparent retargeting of cytosolic enzymes and tRNAs to the organelles, sometimes preserving aaRS-tRNA charging relationships but other times creating surprising mismatches between cytosolic aaRS and mitochondrial tRNA substrates. Our findings indicate that the presence of a photosynthetic plastid drives the retention of specialized systems for organellar tRNA metabolism.</p>
Finding orthologs for aminoacyl tRNA synthetases in parasitic plants
<p>Eukaryotic nuclear genomes often encode distinct sets of protein translation machinery for function in the cytosol vs. organelles (mitochondria and plastids). This phenomenon raises questions about why multiple translation systems are maintained even though they are capable of comparable functions, and whether they evolve differently depending on the compartment where they operate. These questions are particularly interesting in land plants because translation machinery, including aminoacyl-tRNA synthetases (aaRS), is often dual-targeted to both the plastids and mitochondria. These two organelles have quite different metabolisms, with much higher rates of translation in plastids to supply the abundant, rapid-turnover proteins required for photosynthesis. Previous studies have indicated that plant organellar aaRS evolve more slowly compared to mitochondrial aaRS in other eukaryotes that lack plastids. Thus, we investigated the evolution of nuclear-encoded organellar and cytosolic translation machinery across a broad sampling of angiosperms, including non-photosynthetic (heterotrophic) plant species with reduced rates of plastid gene expression to test the hypothesis that translational demands associated with photosynthesis constrain the evolution of bacterial-like enzymes involved in organellar tRNA metabolism. Remarkably, heterotrophic plants exhibited wholesale loss of many organelle-targeted aaRS and other enzymes, even though translation still occurs in their mitochondria and plastids. These losses were often accompanied by apparent retargeting of cytosolic enzymes and tRNAs to the organelles, sometimes preserving aaRS-tRNA charging relationships but other times creating surprising mismatches between cytosolic aaRS and mitochondrial tRNA substrates. Our findings indicate that the presence of a photosynthetic plastid drives the retention of specialized systems for organellar tRNA metabolism.</p>
Finding orthologs for aminoacyl tRNA synthetases in parasitic plants
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