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Gempo N, Yeshi K, Crayn D, Wangchuk P. Climate-Affected Australian Tropical Montane Cloud Forest Plants: Metabolomic Profiles, Isolated Phytochemicals, and Bioactivities. PLANTS (BASEL, SWITZERLAND) 2024; 13:1024. [PMID: 38611553 PMCID: PMC11013060 DOI: 10.3390/plants13071024] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Subscribe] [Scholar Register] [Received: 03/08/2024] [Revised: 03/27/2024] [Accepted: 03/28/2024] [Indexed: 04/14/2024]
Abstract
The Australian Wet Tropics World Heritage Area (WTWHA) in northeast Queensland is home to approximately 18 percent of the nation's total vascular plant species. Over the past century, human activity and industrial development have caused global climate changes, posing a severe and irreversible danger to the entire land-based ecosystem, and the WTWHA is no exception. The current average annual temperature of WTWHA in northeast Queensland is 24 °C. However, in the coming years (by 2030), the average annual temperature increase is estimated to be between 0.5 and 1.4 °C compared to the climate observed between 1986 and 2005. Looking further ahead to 2070, the anticipated temperature rise is projected to be between 1.0 and 3.2 °C, with the exact range depending on future emissions. We identified 84 plant species, endemic to tropical montane cloud forests (TMCF) within the WTWHA, which are already experiencing climate change threats. Some of these plants are used in herbal medicines. This study comprehensively reviewed the metabolomics studies conducted on these 84 plant species until now toward understanding their physiological and metabolomics responses to global climate change. This review also discusses the following: (i) recent developments in plant metabolomics studies that can be applied to study and better understand the interactions of wet tropics plants with climatic stress, (ii) medicinal plants and isolated phytochemicals with structural diversity, and (iii) reported biological activities of crude extracts and isolated compounds.
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Affiliation(s)
- Ngawang Gempo
- Australian Institute of Tropical Health and Medicine (AITHM), James Cook University, Nguma-bada Campus, McGregor Rd., Cairns, QLD 4878, Australia; (N.G.); (P.W.)
- College of Public Health, Medical and Veterinary Services (CPHMVS), James Cook University, Nguma-bada Campus, McGregor Rd., Cairns, QLD 4878, Australia
| | - Karma Yeshi
- Australian Institute of Tropical Health and Medicine (AITHM), James Cook University, Nguma-bada Campus, McGregor Rd., Cairns, QLD 4878, Australia; (N.G.); (P.W.)
- College of Public Health, Medical and Veterinary Services (CPHMVS), James Cook University, Nguma-bada Campus, McGregor Rd., Cairns, QLD 4878, Australia
| | - Darren Crayn
- Australian Tropical Herbarium (ATH), James Cook University, Nguma-bada Campus, McGregor Rd., Cairns, QLD 4878, Australia;
| | - Phurpa Wangchuk
- Australian Institute of Tropical Health and Medicine (AITHM), James Cook University, Nguma-bada Campus, McGregor Rd., Cairns, QLD 4878, Australia; (N.G.); (P.W.)
- College of Public Health, Medical and Veterinary Services (CPHMVS), James Cook University, Nguma-bada Campus, McGregor Rd., Cairns, QLD 4878, Australia
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2
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Seidel T, Artmann PJ, Gkekas I, Illies F, Baack AL, Viefhues M. Microfluidic Single-Cell Study on Arabidopsis thaliana Protoplast Fusion-New Insights on Timescales and Reversibilities. PLANTS (BASEL, SWITZERLAND) 2024; 13:295. [PMID: 38256848 PMCID: PMC10820889 DOI: 10.3390/plants13020295] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Subscribe] [Scholar Register] [Received: 12/13/2023] [Revised: 01/16/2024] [Accepted: 01/17/2024] [Indexed: 01/24/2024]
Abstract
Plant cells are omnipotent and breeding of new varieties can be achieved by protoplast fusion. Such fusions can be achieved by treatment with poly(ethylene glycol) or by applying an electric field. Microfluidic devices allow for controlled conditions and targeted manipulation of small batches of cells down to single-cell analysis. To provide controlled conditions for protoplast fusions and achieve high reproducibility, we developed and characterized a microfluidic device to reliably trap some Arabidopsis thaliana protoplasts and induced cell fusion by controlled addition of poly(ethylene glycol) (PEG, with a molecular weight of 6000). Experiments were conducted to determine the survival rate of isolated protoplasts in our microfluidic system. Afterward, PEG-induced fusion was studied. Our results indicate that the following fusion parameters had a significant impact on the fusion efficiency and duration: PEG concentration, osmolality of solution and flow velocity. A PEG concentration below 10% led to only partial fusion. The osmolality of the PEG fusion solution was found to strongly impact the fusion process; complete fusion of two source cells sufficiently took part in slightly hyper-osmotic solutions, whereas iso-osmotic solutions led to only partial fusion at a 20% PEG concentration. We observed accelerated fusion for higher fluid velocities. Until this study, it was common sense that fusion is one-directional, i.e., once two cells are fused into one cell, they stay fused. Here, we present for the first time the reversible fusion of protoplasts. Our microfluidic device paves the way to a deeper understanding of the kinetics and processes of cell fusion.
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Affiliation(s)
- Thorsten Seidel
- Dynamic Cell Imaging, Faculty of Biology, Bielefeld University, 33615 Bielefeld, Germany
| | - Philipp Johannes Artmann
- Experimental Biophysics and Applied Nanosciences, Faculty of Physics, Bielefeld University, 33615 Bielefeld, Germany
| | - Ioannis Gkekas
- Experimental Biophysics and Applied Nanosciences, Faculty of Physics, Bielefeld University, 33615 Bielefeld, Germany
| | - Franziska Illies
- Dynamic Cell Imaging, Faculty of Biology, Bielefeld University, 33615 Bielefeld, Germany
- Experimental Biophysics and Applied Nanosciences, Faculty of Physics, Bielefeld University, 33615 Bielefeld, Germany
| | - Anna-Lena Baack
- Dynamic Cell Imaging, Faculty of Biology, Bielefeld University, 33615 Bielefeld, Germany
| | - Martina Viefhues
- Experimental Biophysics and Applied Nanosciences, Faculty of Physics, Bielefeld University, 33615 Bielefeld, Germany
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3
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Dragwidge JM, Van Damme D. Protein phase separation in plant membrane biology: more than just a compartmentalization strategy. THE PLANT CELL 2023; 35:3162-3172. [PMID: 37352127 PMCID: PMC10473209 DOI: 10.1093/plcell/koad177] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Abstract] [MESH Headings] [Grants] [Track Full Text] [Subscribe] [Scholar Register] [Received: 11/04/2022] [Revised: 06/14/2023] [Accepted: 06/20/2023] [Indexed: 06/25/2023]
Abstract
The formation of biomolecular condensates through phase separation is an important strategy to compartmentalize cellular functions. While it is now well established that condensates exist throughout eukaryotic cells, how condensates assemble and function on lipid membranes is only beginning to be understood. In this perspective, we highlight work from plant, animal, and yeast model systems showing that condensates assemble on many endomembrane surfaces to carry out diverse functions. In vesicle trafficking, condensation has reported roles in the formation of endocytic vesicles and autophagosomes and in the inactivation of secretory COPII vesicles. We briefly discuss how membranes and membrane lipids regulate the formation and function of membrane-associated condensates. This includes how membranes act as surfaces for condensate assembly, with lipids mediating the nucleation of condensates during endocytosis and other processes. Additionally, membrane-condensate interactions give rise to the biophysical property of "wetting", which has functional importance in shaping autophagosomal and vacuolar membranes. We also speculate on the existence of membrane-associated condensates during cell polarity in plants and discuss how condensation may help to establish functional plasma membrane domains. Lastly, we provide advice on relevant in vitro and in vivo approaches and techniques to study membrane-associated phase separation.
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Affiliation(s)
- Jonathan Michael Dragwidge
- Department of Plant Biotechnology and Bioinformatics, Ghent University, Technologiepark 71, 9052 Ghent, Belgium
- VIB Center for Plant Systems Biology, Technologiepark 71, 9052 Ghent, Belgium
| | - Daniël Van Damme
- Department of Plant Biotechnology and Bioinformatics, Ghent University, Technologiepark 71, 9052 Ghent, Belgium
- VIB Center for Plant Systems Biology, Technologiepark 71, 9052 Ghent, Belgium
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4
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Sharma M, Klösgen RB, Bennewitz B. Fluorescent Protein-Based Approaches for Subcellular Protein Localization in Plants. Methods Mol Biol 2023; 2564:203-211. [PMID: 36107343 DOI: 10.1007/978-1-0716-2667-2_9] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 06/15/2023]
Abstract
Fluorescent proteins (FPs) remarkably advanced the study of cellular biology of plants. The most common application is their use as reporter proteins to determine the subcellular localization of a protein of interest (POI) by endogenous expression of a suitable FP-POI fusion construct in plant cells. In this chapter we describe three approaches, namely, particle bombardment, protoplast transformation, and Agrobacterium infiltration, to transiently express such fusion constructs in plant cells of different species. These approaches are versatile and can be utilized for diverse fluorescent protein-based applications.
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Affiliation(s)
- Mayank Sharma
- Institute of Molecular Plant Biology, ETH Zürich, Zürich, Switzerland.
| | - Ralf Bernd Klösgen
- Institute of Biology-Plant Physiology, Martin Luther University Halle-Wittenberg, Halle (Saale), Germany
| | - Bationa Bennewitz
- Institute of Biology-Plant Physiology, Martin Luther University Halle-Wittenberg, Halle (Saale), Germany
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5
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Shin JM, Yuan L, Kawashima T. Live-cell imaging reveals the cellular dynamics in seed development. PLANT SCIENCE : AN INTERNATIONAL JOURNAL OF EXPERIMENTAL PLANT BIOLOGY 2022; 325:111485. [PMID: 36206961 DOI: 10.1016/j.plantsci.2022.111485] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Track Full Text] [Subscribe] [Scholar Register] [Received: 05/06/2022] [Revised: 09/28/2022] [Accepted: 09/30/2022] [Indexed: 06/16/2023]
Abstract
Seed development in flowering plants is highly complex and governed by three genetically distinct tissues: the fertilization products, the diploid embryo and triploid endosperm, as well as the seed coat that has maternal origin. There are diverse cellular dynamics such as nuclear movement in gamete cells for fertilization, cell polarity establishment for embryo development, and multinuclear endosperm formation. These tissues also coordinate and synchronize the developmental timing for proper seed formation through cell-to-cell communications. Live-cell imaging using advanced microscopy techniques enables us to decipher the dynamics of these events. Especially, the establishment of a less-invasive semi-in vivo live-cell imaging approach has allowed us to perform time-lapse analyses for long period observation of Arabidopsis thaliana intact seed development dynamics. Here we highlight the recent trends of live-cell imaging for seed development and discuss where we are heading.
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Affiliation(s)
- Ji Min Shin
- Department of Plant and Soil Sciences, University of Kentucky, KY, USA; Kentucky Tobacco Research and Development Center, University of Kentucky, KY, USA
| | - Ling Yuan
- Department of Plant and Soil Sciences, University of Kentucky, KY, USA; Kentucky Tobacco Research and Development Center, University of Kentucky, KY, USA
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6
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Parmagnani AS, Maffei ME. Calcium Signaling in Plant-Insect Interactions. PLANTS (BASEL, SWITZERLAND) 2022; 11:2689. [PMID: 36297718 PMCID: PMC9609891 DOI: 10.3390/plants11202689] [Citation(s) in RCA: 1] [Impact Index Per Article: 0.5] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Figures] [Subscribe] [Scholar Register] [Received: 09/22/2022] [Revised: 10/09/2022] [Accepted: 10/11/2022] [Indexed: 06/16/2023]
Abstract
In plant-insect interactions, calcium (Ca2+) variations are among the earliest events associated with the plant perception of biotic stress. Upon herbivory, Ca2+ waves travel long distances to transmit and convert the local signal to a systemic defense program. Reactive oxygen species (ROS), Ca2+ and electrical signaling are interlinked to form a network supporting rapid signal transmission, whereas the Ca2+ message is decoded and relayed by Ca2+-binding proteins (including calmodulin, Ca2+-dependent protein kinases, annexins and calcineurin B-like proteins). Monitoring the generation of Ca2+ signals at the whole plant or cell level and their long-distance propagation during biotic interactions requires innovative imaging techniques based on sensitive sensors and using genetically encoded indicators. This review summarizes the recent advances in Ca2+ signaling upon herbivory and reviews the most recent Ca2+ imaging techniques and methods.
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7
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Hsiao AS, Huang JY. Bioimaging tools move plant physiology studies forward. FRONTIERS IN PLANT SCIENCE 2022; 13:976627. [PMID: 36204075 PMCID: PMC9530904 DOI: 10.3389/fpls.2022.976627] [Citation(s) in RCA: 2] [Impact Index Per Article: 1.0] [Reference Citation Analysis] [Key Words] [Track Full Text] [Figures] [Subscribe] [Scholar Register] [Received: 06/23/2022] [Accepted: 09/05/2022] [Indexed: 06/16/2023]
Affiliation(s)
- An-Shan Hsiao
- Biosciences, College of Life and Environmental Sciences, University of Exeter, Exeter, United Kingdom
| | - Ji-Ying Huang
- Cell Biology Core Lab, Institute of Plant and Microbial Biology, Academia Sinica, Taipei, Taiwan
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8
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Strotmann VI, Stahl Y. Visualization of in vivo protein-protein interactions in plants. JOURNAL OF EXPERIMENTAL BOTANY 2022; 73:3866-3880. [PMID: 35394544 PMCID: PMC9232200 DOI: 10.1093/jxb/erac139] [Citation(s) in RCA: 8] [Impact Index Per Article: 4.0] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Grants] [Track Full Text] [Figures] [Subscribe] [Scholar Register] [Received: 12/28/2021] [Accepted: 04/01/2022] [Indexed: 06/14/2023]
Abstract
Molecular processes depend on the concerted and dynamic interactions of proteins, either by one-on-one interactions of the same or different proteins or by the assembly of larger protein complexes consisting of many different proteins. Here, not only the protein-protein interaction (PPI) itself, but also the localization and activity of the protein of interest (POI) within the cell is essential. Therefore, in all cell biological experiments, preserving the spatio-temporal state of one POI relative to another is key to understanding the underlying complex and dynamic regulatory mechanisms in vivo. In this review, we examine some of the applicable techniques to measure PPIs in planta as well as recent combinatorial advances of PPI methods to measure the formation of higher order complexes with an emphasis on in vivo imaging techniques. We compare the different methods and discuss their benefits and potential pitfalls to facilitate the selection of appropriate techniques by providing a comprehensive overview of how to measure in vivo PPIs in plants.
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Affiliation(s)
- Vivien I Strotmann
- Institute for Developmental Genetics, Heinrich-Heine University, Universitätsstr. 1, D-40225 Düsseldorf, Germany
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9
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Fradera-Soler M, Grace OM, Jørgensen B, Mravec J. Elastic and collapsible: current understanding of cell walls in succulent plants. JOURNAL OF EXPERIMENTAL BOTANY 2022; 73:2290-2307. [PMID: 35167681 PMCID: PMC9015807 DOI: 10.1093/jxb/erac054] [Citation(s) in RCA: 11] [Impact Index Per Article: 5.5] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Grants] [Track Full Text] [Subscribe] [Scholar Register] [Received: 09/20/2021] [Accepted: 02/11/2022] [Indexed: 05/11/2023]
Abstract
Succulent plants represent a large functional group of drought-resistant plants that store water in specialized tissues. Several co-adaptive traits accompany this water-storage capacity to constitute the succulent syndrome. A widely reported anatomical adaptation of cell walls in succulent tissues allows them to fold in a regular fashion during extended drought, thus preventing irreversible damage and permitting reversible volume changes. Although ongoing research on crop and model species continuously reports the importance of cell walls and their dynamics in drought resistance, the cell walls of succulent plants have received relatively little attention to date, despite the potential of succulents as natural capital to mitigate the effects of climate change. In this review, we summarize current knowledge of cell walls in drought-avoiding succulents and their effects on tissue biomechanics, water relations, and photosynthesis. We also highlight the existing knowledge gaps and propose a hypothetical model for regulated cell wall folding in succulent tissues upon dehydration. Future perspectives of methodological development in succulent cell wall characterization, including the latest technological advances in molecular and imaging techniques, are also presented.
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Affiliation(s)
- Marc Fradera-Soler
- Department of Plant and Environmental Sciences, University of Copenhagen, Thorvaldsensvej 40, 1871 Frederiksberg, Denmark
- Royal Botanic Gardens, Kew, Richmond, Surrey, UK
- Correspondence: or
| | | | | | - Jozef Mravec
- Department of Plant and Environmental Sciences, University of Copenhagen, Thorvaldsensvej 40, 1871 Frederiksberg, Denmark
- Correspondence: or
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10
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Ovečka M, Sojka J, Tichá M, Komis G, Basheer J, Marchetti C, Šamajová O, Kuběnová L, Šamaj J. Imaging plant cells and organs with light-sheet and super-resolution microscopy. PLANT PHYSIOLOGY 2022; 188:683-702. [PMID: 35235660 PMCID: PMC8825356 DOI: 10.1093/plphys/kiab349] [Citation(s) in RCA: 7] [Impact Index Per Article: 3.5] [Reference Citation Analysis] [Abstract] [MESH Headings] [Grants] [Track Full Text] [Subscribe] [Scholar Register] [Received: 05/09/2021] [Accepted: 07/12/2021] [Indexed: 05/05/2023]
Abstract
The documentation of plant growth and development requires integrative and scalable approaches to investigate and spatiotemporally resolve various dynamic processes at different levels of plant body organization. The present update deals with vigorous developments in mesoscopy, microscopy and nanoscopy methods that have been translated to imaging of plant subcellular compartments, cells, tissues and organs over the past 3 years with the aim to report recent applications and reasonable expectations from current light-sheet fluorescence microscopy (LSFM) and super-resolution microscopy (SRM) modalities. Moreover, the shortcomings and limitations of existing LSFM and SRM are discussed, particularly for their ability to accommodate plant samples and regarding their documentation potential considering spherical aberrations or temporal restrictions prohibiting the dynamic recording of fast cellular processes at the three dimensions. For a more comprehensive description, advances in living or fixed sample preparation methods are also included, supported by an overview of developments in labeling strategies successfully applied in plants. These strategies are practically documented by current applications employing model plant Arabidopsis thaliana (L.) Heynh., but also robust crop species such as Medicago sativa L. and Hordeum vulgare L. Over the past few years, the trend towards designing of integrative microscopic modalities has become apparent and it is expected that in the near future LSFM and SRM will be bridged to achieve broader multiscale plant imaging with a single platform.
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Affiliation(s)
- Miroslav Ovečka
- Department of Cell Biology, Centre of the Region Haná for Biotechnological and Agricultural Research, Faculty of Science, Palacký University Olomouc, Šlechtitelů 27, 783 71 Olomouc, Czech Republic
| | - Jiří Sojka
- Department of Cell Biology, Centre of the Region Haná for Biotechnological and Agricultural Research, Faculty of Science, Palacký University Olomouc, Šlechtitelů 27, 783 71 Olomouc, Czech Republic
| | - Michaela Tichá
- Department of Cell Biology, Centre of the Region Haná for Biotechnological and Agricultural Research, Faculty of Science, Palacký University Olomouc, Šlechtitelů 27, 783 71 Olomouc, Czech Republic
| | - George Komis
- Department of Cell Biology, Centre of the Region Haná for Biotechnological and Agricultural Research, Faculty of Science, Palacký University Olomouc, Šlechtitelů 27, 783 71 Olomouc, Czech Republic
| | - Jasim Basheer
- Department of Cell Biology, Centre of the Region Haná for Biotechnological and Agricultural Research, Faculty of Science, Palacký University Olomouc, Šlechtitelů 27, 783 71 Olomouc, Czech Republic
| | - Cintia Marchetti
- Centre of the Region Haná for Biotechnological and Agricultural Research, Czech Advanced Technology and Research Institute, Palacký University Olomouc, Šlechtitelů 27, 783 71 Olomouc, Czech Republic
| | - Olga Šamajová
- Department of Cell Biology, Centre of the Region Haná for Biotechnological and Agricultural Research, Faculty of Science, Palacký University Olomouc, Šlechtitelů 27, 783 71 Olomouc, Czech Republic
| | - Lenka Kuběnová
- Department of Cell Biology, Centre of the Region Haná for Biotechnological and Agricultural Research, Faculty of Science, Palacký University Olomouc, Šlechtitelů 27, 783 71 Olomouc, Czech Republic
| | - Jozef Šamaj
- Department of Cell Biology, Centre of the Region Haná for Biotechnological and Agricultural Research, Faculty of Science, Palacký University Olomouc, Šlechtitelů 27, 783 71 Olomouc, Czech Republic
- Author for communication:
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11
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Colin L, Martin-Arevalillo R, Bovio S, Bauer A, Vernoux T, Caillaud MC, Landrein B, Jaillais Y. Imaging the living plant cell: From probes to quantification. THE PLANT CELL 2022; 34:247-272. [PMID: 34586412 PMCID: PMC8774089 DOI: 10.1093/plcell/koab237] [Citation(s) in RCA: 16] [Impact Index Per Article: 8.0] [Reference Citation Analysis] [Abstract] [MESH Headings] [Grants] [Track Full Text] [Subscribe] [Scholar Register] [Received: 07/16/2021] [Accepted: 09/20/2021] [Indexed: 05/20/2023]
Abstract
At the center of cell biology is our ability to image the cell and its various components, either in isolation or within an organism. Given its importance, biological imaging has emerged as a field of its own, which is inherently highly interdisciplinary. Indeed, biologists rely on physicists and engineers to build new microscopes and imaging techniques, chemists to develop better imaging probes, and mathematicians and computer scientists for image analysis and quantification. Live imaging collectively involves all the techniques aimed at imaging live samples. It is a rapidly evolving field, with countless new techniques, probes, and dyes being continuously developed. Some of these new methods or reagents are readily amenable to image plant samples, while others are not and require specific modifications for the plant field. Here, we review some recent advances in live imaging of plant cells. In particular, we discuss the solutions that plant biologists use to live image membrane-bound organelles, cytoskeleton components, hormones, and the mechanical properties of cells or tissues. We not only consider the imaging techniques per se, but also how the construction of new fluorescent probes and analysis pipelines are driving the field of plant cell biology.
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Affiliation(s)
- Leia Colin
- Laboratoire Reproduction et Développement des Plantes, Université de Lyon, ENS de Lyon, CNRS, INRAE, 69342 Lyon, France
| | - Raquel Martin-Arevalillo
- Laboratoire Reproduction et Développement des Plantes, Université de Lyon, ENS de Lyon, CNRS, INRAE, 69342 Lyon, France
| | - Simone Bovio
- Laboratoire Reproduction et Développement des Plantes, Université de Lyon, ENS de Lyon, CNRS, INRAE, 69342 Lyon, France
- LYMIC-PLATIM imaging and microscopy core facility, Univ Lyon, SFR Biosciences, ENS de Lyon, Inserm US8, CNRS UMS3444, UCBL-50 Avenue Tony Garnier, 69007 Lyon, France
| | - Amélie Bauer
- Laboratoire Reproduction et Développement des Plantes, Université de Lyon, ENS de Lyon, CNRS, INRAE, 69342 Lyon, France
| | - Teva Vernoux
- Laboratoire Reproduction et Développement des Plantes, Université de Lyon, ENS de Lyon, CNRS, INRAE, 69342 Lyon, France
| | - Marie-Cecile Caillaud
- Laboratoire Reproduction et Développement des Plantes, Université de Lyon, ENS de Lyon, CNRS, INRAE, 69342 Lyon, France
| | - Benoit Landrein
- Laboratoire Reproduction et Développement des Plantes, Université de Lyon, ENS de Lyon, CNRS, INRAE, 69342 Lyon, France
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12
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Ruberti C. Mitochondrial GFP-Tagged Protein Localization Using Transient Transformations in Arabidopsis thaliana. Methods Mol Biol 2022; 2363:153-163. [PMID: 34545492 DOI: 10.1007/978-1-0716-1653-6_12] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 06/13/2023]
Abstract
Transient transformation assays for the analysis of protein localization are routinely used as rapid and convenient alternatives to stable transformation. In this chapter, we describe two transient gene expression assays (e.g., isolation and transformation of protoplasts, and agroinfiltration of leaves) optimized for Arabidopsis thaliana, and we combine them with fluorescence microscopy, with the final aim to investigate in vivo the subcellular localization of a mitochondrial protein of interest fused to a fluorescent reporter.
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Affiliation(s)
- Cristina Ruberti
- Department of Biology, University of Padua, Padua, Italy.
- Department of Biosciences, University of Milan, Milan, Italy.
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13
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Yanagisawa N, Kozgunova E, Grossmann G, Geitmann A, Higashiyama T. Microfluidics-Based Bioassays and Imaging of Plant Cells. PLANT & CELL PHYSIOLOGY 2021; 62:1239-1250. [PMID: 34027549 PMCID: PMC8579190 DOI: 10.1093/pcp/pcab067] [Citation(s) in RCA: 5] [Impact Index Per Article: 1.7] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Grants] [Track Full Text] [Subscribe] [Scholar Register] [Received: 01/05/2021] [Revised: 04/13/2021] [Accepted: 05/23/2021] [Indexed: 05/03/2023]
Abstract
Many plant processes occur in the context of and in interaction with a surrounding matrix such as soil (e.g. root growth and root-microbe interactions) or surrounding tissues (e.g. pollen tube growth through the pistil), making it difficult to study them with high-resolution optical microscopy. Over the past decade, microfabrication techniques have been developed to produce experimental systems that allow researchers to examine cell behavior in microstructured environments that mimic geometrical, physical and/or chemical aspects of the natural growth matrices and that cannot be generated using traditional agar plate assays. These microfabricated environments offer considerable design flexibility as well as the transparency required for high-resolution, light-based microscopy. In addition, microfluidic platforms have been used for various types of bioassays, including cellular force assays, chemoattraction assays and electrotropism assays. Here, we review the recent use of microfluidic devices to study plant cells and organs, including plant roots, root hairs, moss protonemata and pollen tubes. The increasing adoption of microfabrication techniques by the plant science community may transform our approaches to investigating how individual plant cells sense and respond to changes in the physical and chemical environment.
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Affiliation(s)
- Naoki Yanagisawa
- Institute of Transformative Bio-Molecules (ITbM), Nagoya University, Nagoya Furo-cho, Chikusa-ku, Nagoya, Aichi 464-8601, Japan
| | - Elena Kozgunova
- Department of Plant Biotechnology, Faculty of Biology, University of Freiburg, Freiburg, Schänzlestr. 1, Freiburg, Baden-Württemberg 79104, Germany
| | - Guido Grossmann
- Institute of Cell and Interaction Biology, Heinrich Heine University Düsseldorf, Universitätsstr. 1, Düsseldorf 40225, Germany
- Centre for Organismal Studies, Heidelberg University, Heidelberg, Baden-Württemberg 69120, Germany
| | - Anja Geitmann
- Department of Plant Science, Faculty of Agricultural and Environmental Sciences, McGill University, Québec H9X 3V9, Canada
| | - Tetsuya Higashiyama
- Institute of Transformative Bio-Molecules (ITbM), Nagoya University, Nagoya Furo-cho, Chikusa-ku, Nagoya, Aichi 464-8601, Japan
- Division of Biological Science, Graduate School of Science, Nagoya University, Furo-cho, Chikusa-ku, Nagoya, Aichi 464-8602, Japan
- Department of Biological Sciences, Graduate School of Science, The University of Tokyo, 7-3-1 Hongo, Bunkyo City, Tokyo 113-0033, Japan
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14
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Balcerowicz M, Shetty KN, Jones AM. Fluorescent biosensors illuminating plant hormone research. PLANT PHYSIOLOGY 2021; 187:590-602. [PMID: 35237816 PMCID: PMC8491072 DOI: 10.1093/plphys/kiab278] [Citation(s) in RCA: 12] [Impact Index Per Article: 4.0] [Reference Citation Analysis] [Abstract] [MESH Headings] [Grants] [Track Full Text] [Subscribe] [Scholar Register] [Received: 03/16/2021] [Accepted: 05/22/2021] [Indexed: 05/20/2023]
Abstract
Phytohormones act as key regulators of plant growth that coordinate developmental and physiological processes across cells, tissues and organs. As such, their levels and distribution are highly dynamic owing to changes in their biosynthesis, transport, modification and degradation that occur over space and time. Fluorescent biosensors represent ideal tools to track these dynamics with high spatiotemporal resolution in a minimally invasive manner. Substantial progress has been made in generating a diverse set of hormone sensors with recent FRET biosensors for visualising hormone concentrations complementing information provided by transcriptional, translational and degron-based reporters. In this review, we provide an update on fluorescent biosensor designs, examine the key properties that constitute an ideal hormone biosensor, discuss the use of these sensors in conjunction with in vivo hormone perturbations and highlight the latest discoveries made using these tools.
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Affiliation(s)
| | | | - Alexander M. Jones
- Sainsbury Laboratory, Cambridge University, Cambridge CB2 1LR, UK
- Author for communication:
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15
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Sadoine M, Ishikawa Y, Kleist TJ, Wudick MM, Nakamura M, Grossmann G, Frommer WB, Ho CH. Designs, applications, and limitations of genetically encoded fluorescent sensors to explore plant biology. PLANT PHYSIOLOGY 2021; 187:485-503. [PMID: 35237822 PMCID: PMC8491070 DOI: 10.1093/plphys/kiab353] [Citation(s) in RCA: 18] [Impact Index Per Article: 6.0] [Reference Citation Analysis] [Abstract] [MESH Headings] [Grants] [Track Full Text] [Subscribe] [Scholar Register] [Received: 06/09/2021] [Accepted: 07/12/2021] [Indexed: 05/03/2023]
Abstract
The understanding of signaling and metabolic processes in multicellular organisms requires knowledge of the spatial dynamics of small molecules and the activities of enzymes, transporters, and other proteins in vivo, as well as biophysical parameters inside cells and across tissues. The cellular distribution of receptors, ligands, and activation state must be integrated with information about the cellular distribution of metabolites in relation to metabolic fluxes and signaling dynamics in order to achieve the promise of in vivo biochemistry. Genetically encoded sensors are engineered fluorescent proteins that have been developed for a wide range of small molecules, such as ions and metabolites, or to report biophysical processes, such as transmembrane voltage or tension. First steps have been taken to monitor the activity of transporters in vivo. Advancements in imaging technologies and specimen handling and stimulation have enabled researchers in plant sciences to implement sensor technologies in intact plants. Here, we provide a brief history of the development of genetically encoded sensors and an overview of the types of sensors available for quantifying and visualizing ion and metabolite distribution and dynamics. We further discuss the pros and cons of specific sensor designs, imaging systems, and sample manipulations, provide advice on the choice of technology, and give an outlook into future developments.
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Affiliation(s)
- Mayuri Sadoine
- Molecular Physiology, Heinrich-Heine-University Düsseldorf, Düsseldorf 40225, Germany
| | - Yuuma Ishikawa
- Molecular Physiology, Heinrich-Heine-University Düsseldorf, Düsseldorf 40225, Germany
- Institute of Transformative Bio-Molecules (WPI-ITbM), Nagoya University, Chikusa, Nagoya 464-8601, Japan
| | - Thomas J. Kleist
- Molecular Physiology, Heinrich-Heine-University Düsseldorf, Düsseldorf 40225, Germany
| | - Michael M. Wudick
- Molecular Physiology, Heinrich-Heine-University Düsseldorf, Düsseldorf 40225, Germany
- Cluster of Excellence on Plant Sciences, Heinrich-Heine-University Düsseldorf, Düsseldorf 40225, Germany
| | - Masayoshi Nakamura
- Institute of Transformative Bio-Molecules (WPI-ITbM), Nagoya University, Chikusa, Nagoya 464-8601, Japan
| | - Guido Grossmann
- Cluster of Excellence on Plant Sciences, Heinrich-Heine-University Düsseldorf, Düsseldorf 40225, Germany
- Institute for Cell and Interaction Biology, Heinrich-Heine-University Düsseldorf, Düsseldorf 40225, Germany
| | - Wolf B. Frommer
- Molecular Physiology, Heinrich-Heine-University Düsseldorf, Düsseldorf 40225, Germany
- Institute of Transformative Bio-Molecules (WPI-ITbM), Nagoya University, Chikusa, Nagoya 464-8601, Japan
- Cluster of Excellence on Plant Sciences, Heinrich-Heine-University Düsseldorf, Düsseldorf 40225, Germany
| | - Cheng-Hsun Ho
- Agricultural Biotechnology Research Center, Academia Sinica, Taipei 115, Taiwan
- Author for communication:
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16
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Chaudhary A, Chen X, Leśniewska B, Boikine R, Gao J, Wolf S, Schneitz K. Cell wall damage attenuates root hair patterning and tissue morphogenesis mediated by the receptor kinase STRUBBELIG. Development 2021; 148:270854. [PMID: 34251020 DOI: 10.1242/dev.199425] [Citation(s) in RCA: 4] [Impact Index Per Article: 1.3] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 01/12/2021] [Accepted: 06/14/2021] [Indexed: 01/15/2023]
Abstract
Cell wall remodeling is essential for the control of growth and development as well as the regulation of stress responses. However, the underlying cell wall monitoring mechanisms remain poorly understood. Regulation of root hair fate and flower development in Arabidopsis thaliana requires signaling mediated by the atypical receptor kinase STRUBBELIG (SUB). Furthermore, SUB is involved in cell wall integrity signaling and regulates the cellular response to reduced levels of cellulose, a central component of the cell wall. Here, we show that continuous exposure to sub-lethal doses of the cellulose biosynthesis inhibitor isoxaben results in altered root hair patterning and floral morphogenesis. Genetically impairing cellulose biosynthesis also results in root hair patterning defects. We further show that isoxaben exerts its developmental effects through the attenuation of SUB signaling. Our evidence indicates that downregulation of SUB is a multi-step process and involves changes in SUB complex architecture at the plasma membrane, enhanced removal of SUB from the cell surface, and downregulation of SUB transcript levels. The results provide molecular insight into how the cell wall regulates cell fate and tissue morphogenesis.
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Affiliation(s)
- Ajeet Chaudhary
- Plant Developmental Biology, TUM School of Life Sciences, Technical University of Munich, 85354 Freising, Germany
| | - Xia Chen
- Plant Developmental Biology, TUM School of Life Sciences, Technical University of Munich, 85354 Freising, Germany
| | - Barbara Leśniewska
- Plant Developmental Biology, TUM School of Life Sciences, Technical University of Munich, 85354 Freising, Germany
| | - Rodion Boikine
- Plant Developmental Biology, TUM School of Life Sciences, Technical University of Munich, 85354 Freising, Germany
| | - Jin Gao
- Plant Developmental Biology, TUM School of Life Sciences, Technical University of Munich, 85354 Freising, Germany
| | - Sebastian Wolf
- Cell wall signaling group, Centre for Organismal Studies, University of Heidelberg, 69120 Heidelberg, Germany
| | - Kay Schneitz
- Plant Developmental Biology, TUM School of Life Sciences, Technical University of Munich, 85354 Freising, Germany
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17
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Li K, Prada J, Damineli DSC, Liese A, Romeis T, Dandekar T, Feijó JA, Hedrich R, Konrad KR. An optimized genetically encoded dual reporter for simultaneous ratio imaging of Ca 2+ and H + reveals new insights into ion signaling in plants. THE NEW PHYTOLOGIST 2021; 230:2292-2310. [PMID: 33455006 PMCID: PMC8383442 DOI: 10.1111/nph.17202] [Citation(s) in RCA: 34] [Impact Index Per Article: 11.3] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Grants] [Track Full Text] [Subscribe] [Scholar Register] [Received: 09/29/2020] [Accepted: 12/23/2020] [Indexed: 05/07/2023]
Abstract
Whereas the role of calcium ions (Ca2+ ) in plant signaling is well studied, the physiological significance of pH-changes remains largely undefined. Here we developed CapHensor, an optimized dual-reporter for simultaneous Ca2+ and pH ratio-imaging and studied signaling events in pollen tubes (PTs), guard cells (GCs), and mesophyll cells (MCs). Monitoring spatio-temporal relationships between membrane voltage, Ca2+ - and pH-dynamics revealed interconnections previously not described. In tobacco PTs, we demonstrated Ca2+ -dynamics lag behind pH-dynamics during oscillatory growth, and pH correlates more with growth than Ca2+ . In GCs, we demonstrated abscisic acid (ABA) to initiate stomatal closure via rapid cytosolic alkalization followed by Ca2+ elevation. Preventing the alkalization blocked GC ABA-responses and even opened stomata in the presence of ABA, disclosing an important pH-dependent GC signaling node. In MCs, a flg22-induced membrane depolarization preceded Ca2+ -increases and cytosolic acidification by c. 2 min, suggesting a Ca2+ /pH-independent early pathogen signaling step. Imaging Ca2+ and pH resolved similar cytosol and nuclear signals and demonstrated flg22, but not ABA and hydrogen peroxide to initiate rapid membrane voltage-, Ca2+ - and pH-responses. We propose close interrelation in Ca2+ - and pH-signaling that is cell type- and stimulus-specific and the pH having crucial roles in regulating PT growth and stomata movement.
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Affiliation(s)
- Kunkun Li
- Department of Botany I, Julius-Von-Sachs Institute for Biosciences, University of Wuerzburg, Wuerzburg 97082, Germany
| | - Juan Prada
- Department of Bioinformatics, University of Wuerzburg, Wuerzburg 97074, Germany
| | - Daniel S. C. Damineli
- Department of Cell Biology & Molecular Genetics, University of Maryland, 2136 Bioscience Research Bldg, College Park, MD 20742-5815, USA
- Department of Pediatrics, Faculdade de Medicina da Universidade de São Paulo, São Paulo, SP 01246-903, Brazil
| | - Anja Liese
- Leibniz Institute of Plant Biochemistry, Halle (Saale) 06120, Germany
| | - Tina Romeis
- Leibniz Institute of Plant Biochemistry, Halle (Saale) 06120, Germany
| | - Thomas Dandekar
- Department of Bioinformatics, University of Wuerzburg, Wuerzburg 97074, Germany
| | - José A. Feijó
- Department of Cell Biology & Molecular Genetics, University of Maryland, 2136 Bioscience Research Bldg, College Park, MD 20742-5815, USA
| | - Rainer Hedrich
- Department of Botany I, Julius-Von-Sachs Institute for Biosciences, University of Wuerzburg, Wuerzburg 97082, Germany
| | - Kai Robert Konrad
- Department of Botany I, Julius-Von-Sachs Institute for Biosciences, University of Wuerzburg, Wuerzburg 97082, Germany
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18
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Isoda R, Yoshinari A, Ishikawa Y, Sadoine M, Simon R, Frommer WB, Nakamura M. Sensors for the quantification, localization and analysis of the dynamics of plant hormones. THE PLANT JOURNAL : FOR CELL AND MOLECULAR BIOLOGY 2021; 105:542-557. [PMID: 33231903 PMCID: PMC7898640 DOI: 10.1111/tpj.15096] [Citation(s) in RCA: 14] [Impact Index Per Article: 4.7] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Grants] [Track Full Text] [Subscribe] [Scholar Register] [Received: 07/10/2020] [Accepted: 11/19/2020] [Indexed: 05/13/2023]
Abstract
Plant hormones play important roles in plant growth and development and physiology, and in acclimation to environmental changes. The hormone signaling networks are highly complex and interconnected. It is thus important to not only know where the hormones are produced, how they are transported and how and where they are perceived, but also to monitor their distribution quantitatively, ideally in a non-invasive manner. Here we summarize the diverse set of tools available for quantifying and visualizing hormone distribution and dynamics. We provide an overview over the tools that are currently available, including transcriptional reporters, degradation sensors, and luciferase and fluorescent sensors, and compare the tools and their suitability for different purposes.
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Affiliation(s)
- Reika Isoda
- Institute of Transformative Bio‐Molecules (WPI‐ITbM)Nagoya UniversityChikusaNagoya464‐8601Japan
| | - Akira Yoshinari
- Institute of Transformative Bio‐Molecules (WPI‐ITbM)Nagoya UniversityChikusaNagoya464‐8601Japan
| | - Yuuma Ishikawa
- Institute of Transformative Bio‐Molecules (WPI‐ITbM)Nagoya UniversityChikusaNagoya464‐8601Japan
- Molecular PhysiologyHeinrich‐Heine‐UniversityDüsseldorfGermany
| | - Mayuri Sadoine
- Molecular PhysiologyHeinrich‐Heine‐UniversityDüsseldorfGermany
| | - Rüdiger Simon
- Developmental GeneticsHeinrich‐Heine‐UniversityDüsseldorfGermany
| | - Wolf B. Frommer
- Institute of Transformative Bio‐Molecules (WPI‐ITbM)Nagoya UniversityChikusaNagoya464‐8601Japan
- Molecular PhysiologyHeinrich‐Heine‐UniversityDüsseldorfGermany
| | - Masayoshi Nakamura
- Institute of Transformative Bio‐Molecules (WPI‐ITbM)Nagoya UniversityChikusaNagoya464‐8601Japan
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19
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Dragwidge JM, VAN Damme D. Visualising endocytosis in plants: past, present, and future. J Microsc 2020; 280:104-110. [PMID: 32441767 DOI: 10.1111/jmi.12926] [Citation(s) in RCA: 5] [Impact Index Per Article: 1.3] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 03/09/2020] [Revised: 05/15/2020] [Accepted: 05/20/2020] [Indexed: 12/28/2022]
Abstract
Chris Hawes had a lively fascination for the immensely complex organisation of the endomembrane system, including the process of endocytosis. This is the method by which eukaryotic cells internalise membrane proteins, lipids, carbohydrates, and cell wall enzymes from the cell surface through membrane bound vesicles. Endocytosis occurs progressively, starting with early membrane deformation, scission, and finally the release of the vesicle into the cytoplasm. Next to secretion, endocytosis allows the cell to control the proteome composition of its inner and outer surface membrane and as such, its communication with the outside world. Whereas endocytosis was initially considered theoretically impossible in plants due to their high turgor pressure, it is now established as essential for plant life. Furthermore, endocytosis remains a highly active field of research, both in yeast, animal, and plant model systems. Over the past three decades, the tools and techniques used to visualise, quantify, and characterise endocytosis have resulted in an increasingly higher spatiotemporal understanding of this process. Here we provide a brief history of plant endocytosis research from the time when Chris Hawes was investigating the process, to the current state-of-the-art in the field. We will end this chapter with a discussion on some promising future developments for plant endocytosis research. LAY DESCRIPTION: Endocytosis is a key process whereby eukaryotic cells can selectively take up membrane proteins, extracellular material and lipids. As this process controls the abundance and protein composition of the plasma membrane, it also controls the communication of the cell with the outside world. Whereas endocytosis was initially considered theoretically impossible in plants due to their high turgor pressure, it is now established as essential for plant life. Today, endocytosis remains a highly active field of research, both in yeast, animal, and plant model systems. Endocytosis was one of the favourite research topics of Chris Hawes, which is why this mini-review is part of the Festschrift issue in his honour. We provide here a brief history of plant endocytosis research from the time when Chris Hawes was investigating the process, to the current state-of-the-art in the field. Over the past three decades, the tools and techniques that were developed to visualise, quantify, and characterise endocytosis have allowed to achieve an increasingly higher spatiotemporal understanding of this process. We end this chapter with a discussion on some promising future developments for plant endocytosis research.
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Affiliation(s)
- J M Dragwidge
- Department of Plant Biotechnology and Bioinformatics, Ghent University, Ghent, Belgium.,VIB Center for Plant Systems Biology, Ghent, Belgium
| | - D VAN Damme
- Department of Plant Biotechnology and Bioinformatics, Ghent University, Ghent, Belgium.,VIB Center for Plant Systems Biology, Ghent, Belgium
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20
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Rambaud-Lavigne L, Hay A. Floral organ development goes live. JOURNAL OF EXPERIMENTAL BOTANY 2020; 71:2472-2478. [PMID: 31970400 PMCID: PMC7210761 DOI: 10.1093/jxb/eraa038] [Citation(s) in RCA: 5] [Impact Index Per Article: 1.3] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Grants] [Track Full Text] [Subscribe] [Scholar Register] [Received: 10/11/2019] [Accepted: 01/20/2020] [Indexed: 05/19/2023]
Abstract
The chance to watch floral organs develop live is not to be missed! Here, we outline reasons why quantitative, live-cell imaging is an important approach to study floral morphogenesis, and provide a basic workflow of how to get started. We highlight key advances in morphodynamics of lateral organ development, and discuss recent work that uses live confocal imaging to address the regulation of floral organ number, its robustness, and patterning mechanisms that exploit stochasticity.
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Affiliation(s)
- Léa Rambaud-Lavigne
- Max Planck Institute for Plant Breeding Research, Carl-von-Linné-Weg, Köln, Germany
| | - Angela Hay
- Max Planck Institute for Plant Breeding Research, Carl-von-Linné-Weg, Köln, Germany
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21
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Krupinska K, Blanco NE, Oetke S, Zottini M. Genome communication in plants mediated by organelle-n-ucleus-located proteins. Philos Trans R Soc Lond B Biol Sci 2020; 375:20190397. [PMID: 32362260 PMCID: PMC7209962 DOI: 10.1098/rstb.2019.0397] [Citation(s) in RCA: 29] [Impact Index Per Article: 7.3] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 01/25/2023] Open
Abstract
An increasing number of eukaryotic proteins have been shown to have a dual localization in the DNA-containing organelles, mitochondria and plastids, and/or the nucleus. Regulation of dual targeting and relocation of proteins from organelles to the nucleus offer the most direct means for communication between organelles as well as organelles and nucleus. Most of the mitochondrial proteins of animals have functions in DNA repair and gene expression by modelling of nucleoid architecture and/or chromatin. In plants, such proteins can affect replication and early development. Most plastid proteins with a confirmed or predicted second location in the nucleus are associated with the prokaryotic core RNA polymerase and are required for chloroplast development and light responses. Few plastid–nucleus-located proteins are involved in pathogen defence and cell cycle control. For three proteins, it has been clearly shown that they are first targeted to the organelle and then relocated to the nucleus, i.e. the nucleoid-associated proteins HEMERA and Whirly1 and the stroma-located defence protein NRIP1. Relocation to the nucleus can be experimentally demonstrated by plastid transformation leading to the synthesis of proteins with a tag that enables their detection in the nucleus or by fusions with fluoroproteins in different experimental set-ups. This article is part of the theme issue ‘Retrograde signalling from endosymbiotic organelles’.
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Affiliation(s)
- Karin Krupinska
- Institute of Botany, Christian-Albrechts-University of Kiel, Olshausenstraße 40, 24098 Kiel, Germany
| | - Nicolás E Blanco
- Centre of Photosynthetic and Biochemical Studies, Faculty of Biochemical Science and Pharmacy, National University of Rosario (CEFOBI/UNR-CONICET), Rosario, Argentina
| | - Svenja Oetke
- Institute of Botany, Christian-Albrechts-University of Kiel, Olshausenstraße 40, 24098 Kiel, Germany
| | - Michela Zottini
- Department of Biology, University of Padova, Via U. Bassi 58B, 35131 Padova, Italy
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22
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Valuchova S, Mikulkova P, Pecinkova J, Klimova J, Krumnikl M, Bainar P, Heckmann S, Tomancak P, Riha K. Imaging plant germline differentiation within Arabidopsis flowers by light sheet microscopy. eLife 2020; 9:52546. [PMID: 32041682 DOI: 10.7554/elife.52546.sa2] [Citation(s) in RCA: 1] [Impact Index Per Article: 0.3] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 10/08/2019] [Accepted: 01/04/2020] [Indexed: 05/27/2023] Open
Abstract
In higher plants, germline differentiation occurs during a relatively short period within developing flowers. Understanding of the mechanisms that govern germline differentiation lags behind other plant developmental processes. This is largely because the germline is restricted to relatively few cells buried deep within floral tissues, which makes them difficult to study. To overcome this limitation, we have developed a methodology for live imaging of the germ cell lineage within floral organs of Arabidopsis using light sheet fluorescence microscopy. We have established reporter lines, cultivation conditions, and imaging protocols for high-resolution microscopy of developing flowers continuously for up to several days. We used multiview imagining to reconstruct a three-dimensional model of a flower at subcellular resolution. We demonstrate the power of this approach by capturing male and female meiosis, asymmetric pollen division, movement of meiotic chromosomes, and unusual restitution mitosis in tapetum cells. This method will enable new avenues of research into plant sexual reproduction.
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Affiliation(s)
- Sona Valuchova
- Central European Institute of Technology (CEITEC), Masaryk University, Brno, Czech Republic
| | - Pavlina Mikulkova
- Central European Institute of Technology (CEITEC), Masaryk University, Brno, Czech Republic
| | - Jana Pecinkova
- Central European Institute of Technology (CEITEC), Masaryk University, Brno, Czech Republic
| | - Jana Klimova
- IT4Innovations, VSB-Technical University of Ostrava, Ostrava, Czech Republic
| | - Michal Krumnikl
- IT4Innovations, VSB-Technical University of Ostrava, Ostrava, Czech Republic
- Department of Computer Science, FEECS VSB - Technical University of Ostrava, Ostrava, Czech Republic
| | - Petr Bainar
- IT4Innovations, VSB-Technical University of Ostrava, Ostrava, Czech Republic
| | - Stefan Heckmann
- Leibniz Institute of Plant Genetics and Crop Plant Research (IPK), Seeland, Germany
| | - Pavel Tomancak
- Max Planck Institute of Molecular Cell Biology and Genetics, Dresden, Germany
| | - Karel Riha
- Central European Institute of Technology (CEITEC), Masaryk University, Brno, Czech Republic
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23
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Valuchova S, Mikulkova P, Pecinkova J, Klimova J, Krumnikl M, Bainar P, Heckmann S, Tomancak P, Riha K. Imaging plant germline differentiation within Arabidopsis flowers by light sheet microscopy. eLife 2020; 9:e52546. [PMID: 32041682 PMCID: PMC7012603 DOI: 10.7554/elife.52546] [Citation(s) in RCA: 31] [Impact Index Per Article: 7.8] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Grants] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 10/08/2019] [Accepted: 01/04/2020] [Indexed: 12/21/2022] Open
Abstract
In higher plants, germline differentiation occurs during a relatively short period within developing flowers. Understanding of the mechanisms that govern germline differentiation lags behind other plant developmental processes. This is largely because the germline is restricted to relatively few cells buried deep within floral tissues, which makes them difficult to study. To overcome this limitation, we have developed a methodology for live imaging of the germ cell lineage within floral organs of Arabidopsis using light sheet fluorescence microscopy. We have established reporter lines, cultivation conditions, and imaging protocols for high-resolution microscopy of developing flowers continuously for up to several days. We used multiview imagining to reconstruct a three-dimensional model of a flower at subcellular resolution. We demonstrate the power of this approach by capturing male and female meiosis, asymmetric pollen division, movement of meiotic chromosomes, and unusual restitution mitosis in tapetum cells. This method will enable new avenues of research into plant sexual reproduction.
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Affiliation(s)
- Sona Valuchova
- Central European Institute of Technology (CEITEC)Masaryk UniversityBrnoCzech Republic
| | - Pavlina Mikulkova
- Central European Institute of Technology (CEITEC)Masaryk UniversityBrnoCzech Republic
| | - Jana Pecinkova
- Central European Institute of Technology (CEITEC)Masaryk UniversityBrnoCzech Republic
| | - Jana Klimova
- IT4InnovationsVSB–Technical University of OstravaOstravaCzech Republic
| | - Michal Krumnikl
- IT4InnovationsVSB–Technical University of OstravaOstravaCzech Republic
- Department of Computer ScienceFEECS VSB – Technical University of OstravaOstravaCzech Republic
| | - Petr Bainar
- IT4InnovationsVSB–Technical University of OstravaOstravaCzech Republic
| | - Stefan Heckmann
- Leibniz Institute of Plant Genetics and Crop Plant Research (IPK)SeelandGermany
| | - Pavel Tomancak
- Max Planck Institute of Molecular Cell Biology and GeneticsDresdenGermany
| | - Karel Riha
- Central European Institute of Technology (CEITEC)Masaryk UniversityBrnoCzech Republic
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24
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A Foldable Chip Array for the Continuous Investigation of Seed Germination and the Subsequent Root Development of Seedlings. MICROMACHINES 2019; 10:mi10120884. [PMID: 31861063 PMCID: PMC6953092 DOI: 10.3390/mi10120884] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Download PDF] [Figures] [Subscribe] [Scholar Register] [Received: 10/29/2019] [Revised: 12/08/2019] [Accepted: 12/13/2019] [Indexed: 11/29/2022]
Abstract
Seed germination and seedling root development are important indicators of plant development. This work designed and fabricated a foldable microfluidic chip array for conducting nondestructive and continuous evaluation of seed germination and subsequent seedling development in situ. Each plant chamber has two functional units: seed germination part and root-growth part. The root-growth parts are themselves connected to a single channel designed to provide a uniform culture medium for plant growth. The individual chips are connected into an array using elastic hinges that facilitate the folding and unfolding of the array to accommodate different viewing purposes. In the folded state, the seed germination chambers form a closely spaced array platform to facilitate the comparison of seed germination and plant development characteristics. Unfolding the array facilitates a clear examination of root development within the root-growth parts. The observation window of an individual chip facilitates either the direct examination of the developing seedling (e.g., stems and leaves) or the use of a microscope for examining microscale features (e.g., root tips and root hairs). The potential of the proposed foldable chip array as a new cultivation platform for botanic studies is demonstrated by examining the seed germination and seedling development of tobacco (Nicotiana tabacum) under different cultivation conditions.
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25
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Anjum NA, Amreen, Tantray AY, Khan NA, Ahmad A. Reactive oxygen species detection-approaches in plants: Insights into genetically encoded FRET-based sensors. J Biotechnol 2019; 308:108-117. [PMID: 31836526 DOI: 10.1016/j.jbiotec.2019.12.003] [Citation(s) in RCA: 15] [Impact Index Per Article: 3.0] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 08/07/2019] [Revised: 12/07/2019] [Accepted: 12/08/2019] [Indexed: 12/14/2022]
Abstract
The generation of reactive oxygen species (ROS) (and their reaction products) in abiotic stressed plants can be simultaneous. Hence, it is very difficult to establish individual roles of ROS (and their reaction products) in plants particularly under abiotic stress conditions. It is highly imperative to detect ROS (and their reaction products) and ascertain their role in vivo and also to point their optimal level in order to unveil exact relation of ROS (and their reaction products) with the major components of ROS-controlling systems. Förster Resonance Energy Transfer (FRET) technology enables us with high potential for monitoring and quantification of ROS and redox variations, avoiding some of the obstacles presented by small-molecule fluorescent dyes. This paper aims to: (i) introduce ROS and overview ROS-chemistry and ROS-accrued major damages to major biomolecules; (ii) highlight invasive and non-invasive approaches for the detection of ROS (and their reaction products); (iii) appraise literature available on genetically encoded ROS (and their reaction products)-sensors based on FRET technology, and (iv) enlighten so far unexplored aspects in the current context. The studies integrating the outcomes of the FRET-based ROS-detection approaches with OMICS sciences (genetics, genomics, proteomics, and metabolomics) would enlighten major insights into real-time ROS and redox dynamics, and their signaling at cellular and subcellular levels in living cells.
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Affiliation(s)
- Naser A Anjum
- Department of Botany, Aligarh Muslim University, Aligarh 202 002, U.P., India.
| | - Amreen
- Department of Botany, Aligarh Muslim University, Aligarh 202 002, U.P., India
| | - Aadil Y Tantray
- Department of Botany, Aligarh Muslim University, Aligarh 202 002, U.P., India
| | - Nafees A Khan
- Department of Botany, Aligarh Muslim University, Aligarh 202 002, U.P., India
| | - Altaf Ahmad
- Department of Botany, Aligarh Muslim University, Aligarh 202 002, U.P., India.
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26
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Wagner S, Steinbeck J, Fuchs P, Lichtenauer S, Elsässer M, Schippers JHM, Nietzel T, Ruberti C, Van Aken O, Meyer AJ, Van Dongen JT, Schmidt RR, Schwarzländer M. Multiparametric real-time sensing of cytosolic physiology links hypoxia responses to mitochondrial electron transport. THE NEW PHYTOLOGIST 2019; 224:1668-1684. [PMID: 31386759 DOI: 10.1111/nph.16093] [Citation(s) in RCA: 49] [Impact Index Per Article: 9.8] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Track Full Text] [Subscribe] [Scholar Register] [Received: 05/21/2019] [Accepted: 08/01/2019] [Indexed: 05/24/2023]
Abstract
Hypoxia regularly occurs during plant development and can be induced by the environment through, for example, flooding. To understand how plant tissue physiology responds to progressing oxygen restriction, we aimed to monitor subcellular physiology in real time and in vivo. We establish a fluorescent protein sensor-based system for multiparametric monitoring of dynamic changes in subcellular physiology of living Arabidopsis thaliana leaves and exemplify its applicability for hypoxia stress. By monitoring cytosolic dynamics of magnesium adenosine 5'-triphosphate, free calcium ion concentration, pH, NAD redox status, and glutathione redox status in parallel, linked to transcriptional and metabolic responses, we generate an integrated picture of the physiological response to progressing hypoxia. We show that the physiological changes are surprisingly robust, even when plant carbon status is modified, as achieved by sucrose feeding or extended night. Inhibition of the mitochondrial respiratory chain causes dynamics of cytosolic physiology that are remarkably similar to those under oxygen depletion, highlighting mitochondrial electron transport as a key determinant of the cellular consequences of hypoxia beyond the organelle. A broadly applicable system for parallel in vivo sensing of plant stress physiology is established to map out the physiological context under which both mitochondrial retrograde signalling and low oxygen signalling occur, indicating shared upstream stimuli.
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Affiliation(s)
- Stephan Wagner
- Institute of Plant Biology and Biotechnology (IBBP), University of Münster, Schlossplatz 8, D-48143, Münster, Germany
- Institute of Crop Science and Resource Conservation (INRES), University of Bonn, Friedrich-Ebert-Allee 144, D-53113, Bonn, Germany
- Max-Planck-Institute for Plant Breeding Research, Carl-von-Linné Weg 10, D-50829, Cologne, Germany
| | - Janina Steinbeck
- Institute of Plant Biology and Biotechnology (IBBP), University of Münster, Schlossplatz 8, D-48143, Münster, Germany
| | - Philippe Fuchs
- Institute of Plant Biology and Biotechnology (IBBP), University of Münster, Schlossplatz 8, D-48143, Münster, Germany
- Institute of Crop Science and Resource Conservation (INRES), University of Bonn, Friedrich-Ebert-Allee 144, D-53113, Bonn, Germany
| | - Sophie Lichtenauer
- Institute of Plant Biology and Biotechnology (IBBP), University of Münster, Schlossplatz 8, D-48143, Münster, Germany
| | - Marlene Elsässer
- Institute of Plant Biology and Biotechnology (IBBP), University of Münster, Schlossplatz 8, D-48143, Münster, Germany
- Institute of Crop Science and Resource Conservation (INRES), University of Bonn, Friedrich-Ebert-Allee 144, D-53113, Bonn, Germany
- Institute for Cellular and Molecular Botany (IZMB), University of Bonn, Kirschallee 1, D-53115, Bonn, Germany
| | - Jos H M Schippers
- Institute of Biology I, RWTH Aachen University, Worringerweg 1, D-52074, Aachen, Germany
- Leibniz-Institut für Pflanzengenetik und Kulturpflanzenforschung (IPK), Gatersleben, Corrensstraße 3, D-06466, Seeland, Germany
| | - Thomas Nietzel
- Institute of Plant Biology and Biotechnology (IBBP), University of Münster, Schlossplatz 8, D-48143, Münster, Germany
- Institute of Crop Science and Resource Conservation (INRES), University of Bonn, Friedrich-Ebert-Allee 144, D-53113, Bonn, Germany
| | - Cristina Ruberti
- Institute of Plant Biology and Biotechnology (IBBP), University of Münster, Schlossplatz 8, D-48143, Münster, Germany
| | - Olivier Van Aken
- Department of Biology, Lund University, Sölvegatan 35, Lund, 223 62, Sweden
| | - Andreas J Meyer
- Institute of Crop Science and Resource Conservation (INRES), University of Bonn, Friedrich-Ebert-Allee 144, D-53113, Bonn, Germany
| | - Joost T Van Dongen
- Institute of Biology I, RWTH Aachen University, Worringerweg 1, D-52074, Aachen, Germany
| | - Romy R Schmidt
- Institute of Biology I, RWTH Aachen University, Worringerweg 1, D-52074, Aachen, Germany
| | - Markus Schwarzländer
- Institute of Plant Biology and Biotechnology (IBBP), University of Münster, Schlossplatz 8, D-48143, Münster, Germany
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Dumur T, Duncan S, Graumann K, Desset S, Randall RS, Scheid OM, Prodanov D, Tatout C, Baroux C. Probing the 3D architecture of the plant nucleus with microscopy approaches: challenges and solutions. Nucleus 2019; 10:181-212. [PMID: 31362571 PMCID: PMC6682351 DOI: 10.1080/19491034.2019.1644592] [Citation(s) in RCA: 16] [Impact Index Per Article: 3.2] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 02/21/2019] [Revised: 06/24/2019] [Accepted: 07/01/2019] [Indexed: 12/18/2022] Open
Abstract
The eukaryotic cell nucleus is a central organelle whose architecture determines genome function at multiple levels. Deciphering nuclear organizing principles influencing cellular responses and identity is a timely challenge. Despite many similarities between plant and animal nuclei, plant nuclei present intriguing specificities. Complementary to molecular and biochemical approaches, 3D microscopy is indispensable for resolving nuclear architecture. However, novel solutions are required for capturing cell-specific, sub-nuclear and dynamic processes. We provide a pointer for utilising high-to-super-resolution microscopy and image processing to probe plant nuclear architecture in 3D at the best possible spatial and temporal resolution and at quantitative and cell-specific levels. High-end imaging and image-processing solutions allow the community now to transcend conventional practices and benefit from continuously improving approaches. These promise to deliver a comprehensive, 3D view of plant nuclear architecture and to capture spatial dynamics of the nuclear compartment in relation to cellular states and responses. Abbreviations: 3D and 4D: Three and Four dimensional; AI: Artificial Intelligence; ant: antipodal nuclei (ant); CLSM: Confocal Laser Scanning Microscopy; CTs: Chromosome Territories; DL: Deep Learning; DLIm: Dynamic Live Imaging; ecn: egg nucleus; FACS: Fluorescence-Activated Cell Sorting; FISH: Fluorescent In Situ Hybridization; FP: Fluorescent Proteins (GFP, RFP, CFP, YFP, mCherry); FRAP: Fluorescence Recovery After Photobleaching; GPU: Graphics Processing Unit; KEEs: KNOT Engaged Elements; INTACT: Isolation of Nuclei TAgged in specific Cell Types; LADs: Lamin-Associated Domains; ML: Machine Learning; NA: Numerical Aperture; NADs: Nucleolar Associated Domains; PALM: Photo-Activated Localization Microscopy; Pixel: Picture element; pn: polar nuclei; PSF: Point Spread Function; RHF: Relative Heterochromatin Fraction; SIM: Structured Illumination Microscopy; SLIm: Static Live Imaging; SMC: Spore Mother Cell; SNR: Signal to Noise Ratio; SRM: Super-Resolution Microscopy; STED: STimulated Emission Depletion; STORM: STochastic Optical Reconstruction Microscopy; syn: synergid nuclei; TADs: Topologically Associating Domains; Voxel: Volumetric pixel.
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Affiliation(s)
- Tao Dumur
- Gregor Mendel Institute (GMI) of Molecular Plant Biology, Austrian Academy of Sciences, Vienna Biocenter (VBC), Vienna, Austria
| | - Susan Duncan
- Norwich Research Park, Earlham Institute, Norwich, UK
| | - Katja Graumann
- Department of Biological and Medical Sciences, Oxford Brookes University, Oxford, UK
| | - Sophie Desset
- GReD, Université Clermont Auvergne, CNRS, INSERM, Clermont–Ferrand, France
| | - Ricardo S Randall
- Department of Plant and Microbial Biology, Zürich-Basel Plant Science Center, University of Zürich, Zürich, Switzerland
| | - Ortrun Mittelsten Scheid
- Gregor Mendel Institute (GMI) of Molecular Plant Biology, Austrian Academy of Sciences, Vienna Biocenter (VBC), Vienna, Austria
| | - Dimiter Prodanov
- Environment, Health and Safety, Neuroscience Research Flanders, Leuven, Belgium
| | - Christophe Tatout
- GReD, Université Clermont Auvergne, CNRS, INSERM, Clermont–Ferrand, France
| | - Célia Baroux
- Department of Plant and Microbial Biology, Zürich-Basel Plant Science Center, University of Zürich, Zürich, Switzerland
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28
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Kozgunova E, Goshima G. A versatile microfluidic device for highly inclined thin illumination microscopy in the moss Physcomitrella patens. Sci Rep 2019; 9:15182. [PMID: 31645620 PMCID: PMC6811556 DOI: 10.1038/s41598-019-51624-9] [Citation(s) in RCA: 13] [Impact Index Per Article: 2.6] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Grants] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 06/17/2019] [Accepted: 10/03/2019] [Indexed: 12/26/2022] Open
Abstract
High-resolution microscopy is a valuable tool for studying cellular processes, such as signalling, membrane trafficking, or cytoskeleton remodelling. Several techniques of inclined illumination microscopy allow imaging at a near single molecular level; however, the application of these methods to plant cells is limited, owing to thick cell walls as well as the necessity to excise a part of the tissue for sample preparation. In this study, we utilised a simple, easy-to-use microfluidic device for highly inclined and laminated optical sheet (HILO) microscopy using a model plant Physcomitrella patens. We demonstrated that the shallow microfluidic device can be used for long-term culture of living cells and enables high-resolution HILO imaging of microtubules without perturbing their dynamics. In addition, our microdevice allows the supply and robust washout of compounds during HILO microscopy imaging, for example, to perform a microtubule regrowth assay. Furthermore, we tested long-term (48 h) HILO imaging using a microdevice and visualised the developmental changes in the microtubule dynamics during tissue regeneration. These novel applications of the microfluidic device provide a valuable resource for studying molecular dynamics in living plant cells.
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Affiliation(s)
- Elena Kozgunova
- Division of Biological Science, Graduate School of Science, Nagoya University, Furo-cho, Chikusa-ku, Nagoya, Aichi, 464-8602, Japan.
| | - Gohta Goshima
- Division of Biological Science, Graduate School of Science, Nagoya University, Furo-cho, Chikusa-ku, Nagoya, Aichi, 464-8602, Japan
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29
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Goh T. Long-term live-cell imaging approaches to study lateral root formation in Arabidopsis thaliana. Microscopy (Oxf) 2019; 68:4-12. [PMID: 30476201 DOI: 10.1093/jmicro/dfy135] [Citation(s) in RCA: 4] [Impact Index Per Article: 0.8] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 09/04/2018] [Revised: 10/23/2018] [Accepted: 10/31/2018] [Indexed: 11/12/2022] Open
Abstract
Lateral roots comprise the majority of the branching root system and are important for acquiring nutrients and water from soil in addition to providing anchorage. Lateral roots develop post-embryonically from existing root parts and originate from a subset of specified pericycle cells (lateral root founder cells) located deep inside roots. Small numbers of these specified pericycle cells undergo several rounds of cell division to create a dome-shaped primordium, which eventually organizes a meristem, an essential region for plant growth with active cell division, and emerges from its parental root as a lateral root. Observing cellular and molecular processes for an extended time at various scales are crucial for understanding biological processes during organogenesis. Lateral root formation is an example of the successful application of live-cell imaging approaches to understand various aspects of developmental events in plants, including cell fate determination, cell proliferation, cell-to-cell interaction and cell wall modification. Here I review the recent progress in understanding the molecular mechanisms of lateral root formation and the contribution of live-cell imaging approaches.
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Affiliation(s)
- Tatsuaki Goh
- Graduate School of Science and Technology, Nara Institute of Science and Technology, 8916-5 Takayama, Ikoma, Japan
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Fernández-Fernández ÁD, Van der Hoorn RAL, Gevaert K, Van Breusegem F, Stael S. Caught green-handed: methods for in vivo detection and visualization of protease activity. JOURNAL OF EXPERIMENTAL BOTANY 2019; 70:2125-2141. [PMID: 30805604 DOI: 10.1093/jxb/erz076] [Citation(s) in RCA: 2] [Impact Index Per Article: 0.4] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Track Full Text] [Subscribe] [Scholar Register] [Received: 11/11/2018] [Revised: 01/25/2019] [Accepted: 01/29/2019] [Indexed: 06/09/2023]
Abstract
Proteases are enzymes that cleave peptide bonds of other proteins. Their omnipresence and diverse activities make them important players in protein homeostasis and turnover of the total cell proteome as well as in signal transduction in plant stress responses and development. To understand protease function, it is of paramount importance to assess when and where a specific protease is active. Here, we review the existing methods to detect in vivo protease activity by means of imaging chemical activity-based probes and genetically encoded sensors. We focus on the diverse fluorescent and luminescent sensors at the researcher's disposal and evaluate the potential of imaging techniques to deliver in vivo spatiotemporal detail of protease activity. We predict that in the coming years, revised techniques will help to elucidate plant protease activity and functions and hence expand the current status of the field.
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Affiliation(s)
- Álvaro Daniel Fernández-Fernández
- Department of Plant Biotechnology and Bioinformatics, Ghent University, Ghent, Belgium
- VIB Center for Plant Systems Biology, Ghent, Belgium
| | | | - Kris Gevaert
- Department of Biomolecular Medicine, Ghent University, Ghent, Belgium
- VIB Center for Medical Biotechnology, Ghent, Belgium
| | - Frank Van Breusegem
- Department of Plant Biotechnology and Bioinformatics, Ghent University, Ghent, Belgium
- VIB Center for Plant Systems Biology, Ghent, Belgium
| | - Simon Stael
- Department of Plant Biotechnology and Bioinformatics, Ghent University, Ghent, Belgium
- VIB Center for Plant Systems Biology, Ghent, Belgium
- Department of Biomolecular Medicine, Ghent University, Ghent, Belgium
- VIB Center for Medical Biotechnology, Ghent, Belgium
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31
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Zaman N, Seitz K, Kabir M, George-Schreder LS, Shepstone I, Liu Y, Zhang S, Krysan PJ. A Förster resonance energy transfer sensor for live-cell imaging of mitogen-activated protein kinase activity in Arabidopsis. THE PLANT JOURNAL : FOR CELL AND MOLECULAR BIOLOGY 2019; 97:970-983. [PMID: 30444549 PMCID: PMC6750906 DOI: 10.1111/tpj.14164] [Citation(s) in RCA: 17] [Impact Index Per Article: 3.4] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Grants] [Track Full Text] [Subscribe] [Scholar Register] [Received: 07/05/2018] [Revised: 10/23/2018] [Accepted: 10/30/2018] [Indexed: 05/08/2023]
Abstract
The catalytic activity of mitogen-activated protein kinases (MAPKs) is dynamically modified in plants. Since MAPKs have been shown to play important roles in a wide range of signaling pathways, the ability to monitor MAPK activity in living plant cells would be valuable. Here, we report the development of a genetically encoded MAPK activity sensor for use in Arabidopsis thaliana. The sensor is composed of yellow and blue fluorescent proteins, a phosphopeptide binding domain, a MAPK substrate domain and a flexible linker. Using in vitro testing, we demonstrated that phosphorylation causes an increase in the Förster resonance energy transfer (FRET) efficiency of the sensor. The FRET efficiency can therefore serve as a readout of kinase activity. We also produced transgenic Arabidopsis lines expressing this sensor of MAPK activity (SOMA) and performed live-cell imaging experiments using detached cotyledons. Treatment with NaCl, the synthetic flagellin peptide flg22 and chitin all led to rapid gains in FRET efficiency. Control lines expressing a version of SOMA in which the phosphosite was mutated to an alanine did not show any substantial changes in FRET. We also expressed the sensor in a conditional loss-of-function double-mutant line for the Arabidopsis MAPK genes MPK3 and MPK6. These experiments demonstrated that MPK3/6 are necessary for the NaCl-induced FRET gain of the sensor, while other MAPKs are probably contributing to the chitin and flg22-induced increases in FRET. Taken together, our results suggest that SOMA is able to dynamically report MAPK activity in living plant cells.
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Affiliation(s)
- Najia Zaman
- Horticulture Department, University of Wisconsin-Madison, Madison, WI, USA
| | - Kati Seitz
- Laboratory of Genetics, University of Wisconsin-Madison, Madison, WI, USA
| | - Mohiuddin Kabir
- Horticulture Department, University of Wisconsin-Madison, Madison, WI, USA
| | | | - Ian Shepstone
- Horticulture Department, University of Wisconsin-Madison, Madison, WI, USA
| | - Yidong Liu
- Division of Biochemistry, Interdisciplinary Plant Group, Bond Life Sciences Center, University of Missouri, Columbia, MO, USA
| | - Shuqun Zhang
- Division of Biochemistry, Interdisciplinary Plant Group, Bond Life Sciences Center, University of Missouri, Columbia, MO, USA
| | - Patrick J. Krysan
- Horticulture Department, University of Wisconsin-Madison, Madison, WI, USA
- Genome Center of Wisconsin, University of Wisconsin-Madison, Madison, WI, USA
- For correspondence ()
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Shahid M, Khan MS, Kumar M. Kitazin-pea interaction: understanding the fungicide induced nodule alteration, cytotoxicity, oxidative damage and toxicity alleviation byRhizobium leguminosarum. RSC Adv 2019; 9:16929-16947. [PMID: 35519857 PMCID: PMC9064474 DOI: 10.1039/c9ra01253b] [Citation(s) in RCA: 16] [Impact Index Per Article: 3.2] [Reference Citation Analysis] [Abstract] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 02/18/2019] [Accepted: 05/08/2019] [Indexed: 12/19/2022] Open
Abstract
Realizing the severity of fungicidal toxicity to legumes and importance of fungicide tolerant rhizobia in legume production, kitazin tolerant (2400 μg mL−1) strain RP1 was recovered from pea nodules and was identified as Rhizobium leguminosarum (accession no. KY940047). R. leguminosarum produced indole acetic acid (80.5 ± 2.5 mL−1), siderophores: salicylic acid (54 ± 7.3 μg mL−1) and 2,3-dihydoxybenzoic acid (31.9 ± 2.7 μg mL−1), α-ketobutyrate (51 ± 3.2 per mg per protein per hour), solubilized insoluble phosphate (29.5 ± 1.8 μg mL−1) and secreted 29.5 + 2.6 μg mL−1 exopolysaccharides, which, however, decreased consistently with gradually increasing kitazin concentrations. Beyond the tolerance level, kitazin caused structural damage and altered membrane integrity of RP1, as revealed under scanning (SEM) and confocal (CLSM) electron microscopy. Phytotoxicity of kitazin to peas was obvious under both in vitro and in vivo conditions. A significant reduction of 23, 68, 57 and 50% in germination, seedling vigor index, plumule length and radicle length was found at 2× kitazin compared to the control. Cellular damage and cytotoxicity induced by kitazin in membrane altered root cells was detected with acridine orange/propidium iodide (AO/PI) and Evans blue dye. A maximum increase of 1.72, 5.2, 9.3 and 1.72, 5.2, 9.3-fold in red and blue fluorescence was quantified at 1×, 2×, and 3× doses of kitazin, respectively. In contrast, application of R. leguminosarum RP1 alleviated toxicity and enhanced the length of plant organs, dry biomass, symbiotic attributes, photosynthetic pigments, nutrient uptake and grain features of peas comparatively uninoculated and fungicide-treated plants. Additionally, strain RP1 expressively reduced the antioxidant enzymes peroxidase, ascorbate peroxidase, guaiacol peroxidase, catalase and malondialdehyde contents by 10, 2.2, 11, 20 and 4% compared to stressed plants raised at 192 μg kg−1 soil. Moreover, a decline of 19, 21 and 20% in proline content extracted from roots, shoots and grains, respectively was recorded for R. leguminosarum inoculated pea plants grown with 96 μg kg−1 kitazin. Also, the SEM and CLSM of roots revealed the bacterial colonization. In conclusion, R. leguminosarum tolerated a higher level of kitazin, secreted plant growth promoting (PGP) bioactive molecules even under fungicide stress and significantly increased the performance of peas while reducing the levels of proline and antioxidant enzymes. So, it can safely be suggested to legume growers that RP1 strain could inexpensively be explored as an efficient biofertilizer for enhancing the production of legumes especially peas while growing even under fungicide (kitazin) enriched soils. Realizing the severity of fungicidal toxicity to legumes and the importance of fungicide tolerant rhizobia in legume production, kitazin tolerant strain RP1 was recovered from pea nodules and was identified as Rhizobium leguminosarum.![]()
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Affiliation(s)
- Mohammad Shahid
- Department of Agricultural Microbiology
- Faculty of Agricultural Sciences
- Aligarh Muslim University
- Aligarh-202002
- India
| | - Mohammad Saghir Khan
- Department of Agricultural Microbiology
- Faculty of Agricultural Sciences
- Aligarh Muslim University
- Aligarh-202002
- India
| | - Murugan Kumar
- Genomics-II
- ICAR-NBAIM (National Bureau of Agriculturally Important Microorganisms)
- Mau-275103
- India
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Matzke AJ, Lin WD, Matzke M. Evidence That Ion-Based Signaling Initiating at the Cell Surface Can Potentially Influence Chromatin Dynamics and Chromatin-Bound Proteins in the Nucleus. FRONTIERS IN PLANT SCIENCE 2019; 10:1267. [PMID: 31681370 PMCID: PMC6811650 DOI: 10.3389/fpls.2019.01267] [Citation(s) in RCA: 5] [Impact Index Per Article: 1.0] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Subscribe] [Scholar Register] [Received: 04/01/2019] [Accepted: 09/11/2019] [Indexed: 05/18/2023]
Abstract
We have developed tools and performed pilot experiments to test the hypothesis that an intracellular ion-based signaling pathway, provoked by an extracellular stimulus acting at the cell surface, can influence interphase chromosome dynamics and chromatin-bound proteins in the nucleus. The experimental system employs chromosome-specific fluorescent tags and the genome-encoded fluorescent pH sensor SEpHluorinA227D, which has been targeted to various intracellular membranes and soluble compartments in root cells of Arabidopsis thaliana. We are using this system and three-dimensional live cell imaging to visualize whether fluorescent-tagged interphase chromosome sites undergo changes in constrained motion concurrently with reductions in membrane-associated pH elicited by extracellular ATP, which is known to trigger a cascade of events in plant cells including changes in calcium ion concentrations, pH, and membrane potential. To examine possible effects of the proposed ion-based signaling pathway directly at the chromatin level, we generated a pH-sensitive fluorescent DNA-binding protein that allows pH changes to be monitored at specific genomic sites. Results obtained using these tools support the existence of a rapid, ion-based signaling pathway that initiates at the cell surface and reaches the nucleus to induce alterations in interphase chromatin mobility and the surrounding pH of chromatin-bound proteins. Such a pathway could conceivably act under natural circumstances to allow external stimuli to swiftly influence gene expression by affecting interphase chromosome movement and the structures and/or activities of chromatin-associated proteins.
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Affiliation(s)
| | | | - Marjori Matzke
- *Correspondence: Antonius J.M. Matzke, ; Marjori Matzke,
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Tofanelli R, Vijayan A, Scholz S, Schneitz K. Protocol for rapid clearing and staining of fixed Arabidopsis ovules for improved imaging by confocal laser scanning microscopy. PLANT METHODS 2019; 15:120. [PMID: 31673277 PMCID: PMC6814113 DOI: 10.1186/s13007-019-0505-x] [Citation(s) in RCA: 19] [Impact Index Per Article: 3.8] [Reference Citation Analysis] [Abstract] [Key Words] [Grants] [Track Full Text] [Subscribe] [Scholar Register] [Received: 06/07/2019] [Accepted: 10/17/2019] [Indexed: 05/15/2023]
Abstract
BACKGROUND A salient topic in developmental biology relates to the molecular and genetic mechanisms that underlie tissue morphogenesis. Modern quantitative approaches to this central question frequently involve digital cellular models of the organ or tissue under study. The ovules of the model species Arabidopsis thaliana have long been established as a model system for the study of organogenesis in plants. While ovule development in Arabidopsis can be followed by a variety of different imaging techniques, no experimental strategy presently exists that enables an easy and straightforward investigation of the morphology of internal tissues of the ovule with cellular resolution. RESULTS We developed a protocol for rapid and robust confocal microscopy of fixed Arabidopsis ovules of all stages. The method combines clearing of fixed ovules in ClearSee solution with marking the cell outline using the cell wall stain SCRI Renaissance 2200 and the nuclei with the stain TO-PRO-3 iodide. We further improved the microscopy by employing a homogenous immersion system aimed at minimizing refractive index differences. The method allows complete inspection of the cellular architecture even deep within the ovule. Using the new protocol we were able to generate digital three-dimensional models of ovules of various stages. CONCLUSIONS The protocol enables the quick and reproducible imaging of fixed Arabidopsis ovules of all developmental stages. From the imaging data three-dimensional digital ovule models with cellular resolution can be rapidly generated using image analysis software, for example MorphographX. Such digital models will provide the foundation for a future quantitative analysis of ovule morphogenesis in a model species.
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Affiliation(s)
- Rachele Tofanelli
- Entwicklungsbiologie der Pflanzen, Wissenschaftszentrum Weihenstephan, Technische Universität München, Emil-Ramann-Str. 4, 85354 Freising, Germany
| | - Athul Vijayan
- Entwicklungsbiologie der Pflanzen, Wissenschaftszentrum Weihenstephan, Technische Universität München, Emil-Ramann-Str. 4, 85354 Freising, Germany
| | - Sebastian Scholz
- Entwicklungsbiologie der Pflanzen, Wissenschaftszentrum Weihenstephan, Technische Universität München, Emil-Ramann-Str. 4, 85354 Freising, Germany
- Present Address: EU Research Lab, Technische Hochschule Wildau, 15745 Wildau, Germany
| | - Kay Schneitz
- Entwicklungsbiologie der Pflanzen, Wissenschaftszentrum Weihenstephan, Technische Universität München, Emil-Ramann-Str. 4, 85354 Freising, Germany
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35
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Kinoshita N, Sugita A, Lustig B, Betsuyaku S, Fujikawa T, Morishita T. Automating measurements of fluorescent signals in freely moving plant leaf specimens. PLANT BIOTECHNOLOGY (TOKYO, JAPAN) 2019; 36:7-11. [PMID: 31275043 PMCID: PMC6566008 DOI: 10.5511/plantbiotechnology.18.1002a] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Subscribe] [Scholar Register] [Received: 09/12/2018] [Accepted: 10/02/2018] [Indexed: 06/09/2023]
Abstract
Existing methods to quantify fluorescent signals are primarily limited to non-moving objects or tracking a limited number of cells. These techniques, however, are unsuitable for measuring fluorescent signals in time-lapse experiments using plant specimens that move naturally during a course of imaging. We developed an automated method to measure fluorescent signal intensities in transgenic Arabidopsis plants using a stereomicroscope with standard microscopy software. The features of our technique include: 1) recognizing the shape of plant specimens using autofluorescent signals; 2) merging targeted fluorescent signals to specimen outlines; 3) extracting signals within the shape of specimens from their background signals. Our method facilitates the measurement of fluorescent signals on freely moving plant leaves that are physically unrestrained. The method we developed addresses the challenge of recognizing plant shapes without relying on: a) manual definition which is prone to subjectivity and human error; b) introducing stable fluorescent markers to define plant shapes; c) recognizing plant shapes from bright field images which include a wide range of colors and background noise; d) unnecessarily stressing plants by immobilizing them; e) the use of multiple software packages or software development expertise.
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Affiliation(s)
- Natsuko Kinoshita
- Faculty of Life and Environmental Sciences, University of Tsukuba, 1-1-1 Tennodai, Tsukuba, Ibaraki 305-8572, Japan
| | - Aki Sugita
- Faculty of Life and Environmental Sciences, University of Tsukuba, 1-1-1 Tennodai, Tsukuba, Ibaraki 305-8572, Japan
- Department of Evolutionary Studies of Biosystems, School of Advanced Sciences, SOKENDAI (The Graduate University for Advanced Studies), Shonan Village, Hayama, Kanagawa 240-0193, Japan
| | - Barry Lustig
- Cormorant Group, Pittsburgh, Pennsylvania 15243, USA
| | - Shigeyuki Betsuyaku
- Faculty of Life and Environmental Sciences, University of Tsukuba, 1-1-1 Tennodai, Tsukuba, Ibaraki 305-8572, Japan
| | | | - Tatsuji Morishita
- Leica Microsystems, 1-29-9 Takatanobaba, Shinjuku, Tokyo 169-0075, Japan
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36
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Geisler M. Seeing is better than believing: visualization of membrane transport in plants. CURRENT OPINION IN PLANT BIOLOGY 2018; 46:104-112. [PMID: 30253307 DOI: 10.1016/j.pbi.2018.09.005] [Citation(s) in RCA: 4] [Impact Index Per Article: 0.7] [Reference Citation Analysis] [Abstract] [MESH Headings] [Track Full Text] [Subscribe] [Scholar Register] [Received: 04/25/2018] [Revised: 08/30/2018] [Accepted: 09/03/2018] [Indexed: 05/27/2023]
Abstract
Recently, the plant transport field has shifted their research focus toward a more integrative investigation of transport networks thought to provide the basis for long-range transport routes. Substantial progress was provided by of a series of elegant techniques that allow for a visualization or prediction of substrate movements in plant tissues in contrast to established quantitative methods offering low spatial resolution. These methods are critically evaluated in respect to their spatio-temporal resolution, invasiveness, dynamics and overall quality. Current limitations of transport route predictions-based on transporter locations and transport modeling are addressed. Finally, the potential of new tools that have not yet been fully implemented into plant research is indicated.
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Affiliation(s)
- Markus Geisler
- University of Fribourg, Department of Biology, Chemin du Musée 10, CH-1700 Fribourg, Switzerland.
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37
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A simple microfluidic device for live cell imaging of Arabidopsis cotyledons, leaves, and seedlings. Biotechniques 2018; 64:255-261. [PMID: 29939090 PMCID: PMC8592504 DOI: 10.2144/btn-2018-0044] [Citation(s) in RCA: 5] [Impact Index Per Article: 0.8] [Reference Citation Analysis] [Abstract] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 11/23/2022] Open
Abstract
One of the challenges of performing live-cell imaging in plants is establishing a system for securing the sample during imaging that allows for the rapid addition of treatments. Here we report how a commercially available device called a HybriWell™ can be repurposed to create an imaging chamber suitable for Arabidopsis seedlings, cotyledons and leaves. Liquid in the imaging chamber can be rapidly exchanged to introduce chemical treatments via microfluidic passive pumping. When used in conjunction with fluorescent biosensors, this system can facilitate live-cell imaging studies of signal transduction pathways triggered by different treatments. As a demonstration, we show how the HybriWell can be used to monitor flg22-induced calcium transients using the R-GECO1 calcium indicator in detached Arabidopsis leaves.
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38
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Shahid M, Ahmed B, Zaidi A, Khan MS. Toxicity of fungicides toPisum sativum: a study of oxidative damage, growth suppression, cellular death and morpho-anatomical changes. RSC Adv 2018; 8:38483-38498. [PMID: 35559088 PMCID: PMC9090578 DOI: 10.1039/c8ra03923b] [Citation(s) in RCA: 28] [Impact Index Per Article: 4.7] [Reference Citation Analysis] [Abstract] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 05/08/2018] [Accepted: 11/01/2018] [Indexed: 11/21/2022] Open
Abstract
Considering the fungicidal threat to the sustainable agro-environment, the toxicological impacts of three fungicides, namely kitazin, hexaconazole and carbendazim, on the biological, chemical and morpho-anatomical changes of peas were assessed. Fungicide applications in general caused a slow but gradual reduction in growth, symbiosis and yields of peas, which, however, varied appreciably among species and concentrations of the three fungicides. Of the three fungicides, carbendazim had the most lethal effect, in which it delayed seed germination and also diminished the overall pea growth. Carbendazim at 3000 μg kg−1 maximally reduced the germination, SVI, size of roots and shoots and total dry matter accumulation in roots, shoots and whole plants distinctly by 40%, 84%, 72%, 73%, 68%, 75% and 73% (p ≤ 0.05), respectively. Hexaconazole at 120 μg kg−1 significantly (p ≤ 0.05) declined total chlorophyll, carotenoids, grain yields, grain protein, root P and shoot N by 19%, 28%, 46%, 69%, 48% and 51%, respectively, over the control. The synthesis of stress biomarkers and oxidative stress were increased with increasing dosage rates of fungicides. Proline content in roots, shoots, leaves and grains, MDA, electrolyte leakage and H2O2 of plants grown in soil treated with 288 μg kg−1 kitazin were increased significantly (p ≤ 0.05) by 73%, 52%, 41%, 24%, 59%, 40% and 27%, respectively, relative to the control. Antioxidant defence enzymes were greater in pea foliage. The SEM and CLSM images revealed an obvious alteration in root tips, enhanced cellular damage and cell death when plants were raised under fungicide stress. Also, morpho-anatomical variations in fungicide-treated foliage were visible in the SEM images. Overall, the present study suggests that a careful and secure strategy should be adopted before fungicides are chosen for enhancing pulse production in different agro-climatic regions. Considering the fungicidal threat to the sustainable agro-environment, the toxicological impacts of three fungicides, namely kitazin, hexaconazole and carbendazim, on the biological, chemical and morpho-anatomical changes of peas were assessed.![]()
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Affiliation(s)
- Mohammad Shahid
- Department of Agricultural Microbiology
- Faculty of Agricultural Sciences
- Aligarh Muslim University
- Aligarh-202002
- India
| | - Bilal Ahmed
- Department of Agricultural Microbiology
- Faculty of Agricultural Sciences
- Aligarh Muslim University
- Aligarh-202002
- India
| | - Almas Zaidi
- Department of Agricultural Microbiology
- Faculty of Agricultural Sciences
- Aligarh Muslim University
- Aligarh-202002
- India
| | - Mohd Saghir Khan
- Department of Agricultural Microbiology
- Faculty of Agricultural Sciences
- Aligarh Muslim University
- Aligarh-202002
- India
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