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Jouhet J, Alves E, Boutté Y, Darnet S, Domergue F, Durand T, Fischer P, Fouillen L, Grube M, Joubès J, Kalnenieks U, Kargul JM, Khozin-Goldberg I, Leblanc C, Letsiou S, Lupette J, Markov GV, Medina I, Melo T, Mojzeš P, Momchilova S, Mongrand S, Moreira ASP, Neves BB, Oger C, Rey F, Santaeufemia S, Schaller H, Schleyer G, Tietel Z, Zammit G, Ziv C, Domingues R. Plant and algal lipidomes: Analysis, composition, and their societal significance. Prog Lipid Res 2024; 96:101290. [PMID: 39094698 DOI: 10.1016/j.plipres.2024.101290] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 03/18/2024] [Revised: 07/25/2024] [Accepted: 07/26/2024] [Indexed: 08/04/2024]
Abstract
Plants and algae play a crucial role in the earth's ecosystems. Through photosynthesis they convert light energy into chemical energy, capture CO2 and produce oxygen and energy-rich organic compounds. Photosynthetic organisms are primary producers and synthesize the essential omega 3 and omega 6 fatty acids. They have also unique and highly diverse complex lipids, such as glycolipids, phospholipids, triglycerides, sphingolipids and phytosterols, with nutritional and health benefits. Plant and algal lipids are useful in food, feed, nutraceutical, cosmeceutical and pharmaceutical industries but also for green chemistry and bioenergy. The analysis of plant and algal lipidomes represents a significant challenge due to the intricate and diverse nature of their composition, as well as their plasticity under changing environmental conditions. Optimization of analytical tools is crucial for an in-depth exploration of the lipidome of plants and algae. This review highlights how lipidomics analytical tools can be used to establish a complete mapping of plant and algal lipidomes. Acquiring this knowledge will pave the way for the use of plants and algae as sources of tailored lipids for both industrial and environmental applications. This aligns with the main challenges for society, upholding the natural resources of our planet and respecting their limits.
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Affiliation(s)
- Juliette Jouhet
- Laboratoire de Physiologie Cellulaire et Végétale, CNRS/INRAE/CEA/Grenoble Alpes Univ., 38000 Grenoble, France.
| | - Eliana Alves
- Mass Spectrometry Centre, LAQV-REQUIMTE, Department of Chemistry, University of Aveiro, Santiago University Campus, Aveiro 3810-193, Portugal
| | - Yohann Boutté
- Laboratoire de Biogenèse Membranaire, UMR5200 CNRS-Université de Bordeaux, CNRS, Villenave-d'Ornon, France
| | | | - Frédéric Domergue
- Laboratoire de Biogenèse Membranaire, UMR5200 CNRS-Université de Bordeaux, CNRS, Villenave-d'Ornon, France
| | - Thierry Durand
- Institut des Biomolécules Max Mousseron (IBMM), Pôle Chimie Balard Recherche, University of Montpellier, ENSCN, UMR 5247 CNRS, France
| | - Pauline Fischer
- Institut des Biomolécules Max Mousseron (IBMM), Pôle Chimie Balard Recherche, University of Montpellier, ENSCN, UMR 5247 CNRS, France
| | - Laetitia Fouillen
- Laboratoire de Biogenèse Membranaire, UMR5200 CNRS-Université de Bordeaux, CNRS, Villenave-d'Ornon, France
| | - Mara Grube
- Institute of Microbiology and Biotechnology, University of Latvia, Riga, Latvia
| | - Jérôme Joubès
- Laboratoire de Biogenèse Membranaire, UMR5200 CNRS-Université de Bordeaux, CNRS, Villenave-d'Ornon, France
| | - Uldis Kalnenieks
- Institute of Microbiology and Biotechnology, University of Latvia, Riga, Latvia
| | - Joanna M Kargul
- Solar Fuels Laboratory, Center of New Technologies, University of Warsaw, 02-097 Warsaw, Poland
| | - Inna Khozin-Goldberg
- Microalgal Biotechnology Laboratory, The French Associates Institute for Dryland Agriculture and Biotechnology, The J. Blaustein Institutes for Desert Research, Ben Gurion University, Midreshet Ben Gurion 8499000, Israel
| | - Catherine Leblanc
- Sorbonne Université, CNRS, Integrative Biology of Marine Models (LBI2M), Station Biologique de Roscoff (SBR), 29680 Roscoff, France
| | - Sophia Letsiou
- Department of Food Science and Technology, University of West Attica, Ag. Spiridonos str. Egaleo, 12243 Athens, Greece
| | - Josselin Lupette
- Laboratoire de Biogenèse Membranaire, UMR5200 CNRS-Université de Bordeaux, CNRS, Villenave-d'Ornon, France
| | - Gabriel V Markov
- Sorbonne Université, CNRS, Integrative Biology of Marine Models (LBI2M), Station Biologique de Roscoff (SBR), 29680 Roscoff, France
| | - Isabel Medina
- Instituto de Investigaciones Marinas - Consejo Superior de Investigaciones Científicas (IIM-CSIC), Eduardo Cabello 6, E-36208 Vigo, Galicia, Spain
| | - Tânia Melo
- Mass Spectrometry Centre, LAQV-REQUIMTE, Department of Chemistry, University of Aveiro, Santiago University Campus, Aveiro 3810-193, Portugal; CESAM-Centre for Environmental and Marine Studies, Department of Chemistry, University of Aveiro, Santiago University Campus, Aveiro 3810-193, Portugal
| | - Peter Mojzeš
- Institute of Physics, Faculty of Mathematics and Physics, Charles University, Ke Karlovu 5, CZ-12116 Prague 2, Czech Republic
| | - Svetlana Momchilova
- Department of Lipid Chemistry, Institute of Organic Chemistry with Centre of Phytochemistry, Bulgarian Academy of Sciences, Acad. G. Bonchev Street, bl. 9, BG-1113 Sofia, Bulgaria
| | - Sébastien Mongrand
- Laboratoire de Biogenèse Membranaire, UMR5200 CNRS-Université de Bordeaux, CNRS, Villenave-d'Ornon, France
| | - Ana S P Moreira
- Mass Spectrometry Centre, LAQV-REQUIMTE, Department of Chemistry, University of Aveiro, Santiago University Campus, Aveiro 3810-193, Portugal
| | - Bruna B Neves
- Mass Spectrometry Centre, LAQV-REQUIMTE, Department of Chemistry, University of Aveiro, Santiago University Campus, Aveiro 3810-193, Portugal; CESAM-Centre for Environmental and Marine Studies, Department of Chemistry, University of Aveiro, Santiago University Campus, Aveiro 3810-193, Portugal
| | - Camille Oger
- Institut des Biomolécules Max Mousseron (IBMM), Pôle Chimie Balard Recherche, University of Montpellier, ENSCN, UMR 5247 CNRS, France
| | - Felisa Rey
- Mass Spectrometry Centre, LAQV-REQUIMTE, Department of Chemistry, University of Aveiro, Santiago University Campus, Aveiro 3810-193, Portugal; CESAM-Centre for Environmental and Marine Studies, Department of Chemistry, University of Aveiro, Santiago University Campus, Aveiro 3810-193, Portugal
| | - Sergio Santaeufemia
- Solar Fuels Laboratory, Center of New Technologies, University of Warsaw, 02-097 Warsaw, Poland
| | - Hubert Schaller
- Institut de Biologie Moléculaire des Plantes du CNRS, Université de Strasbourg, 12 rue du Général Zimmer, F-67083 Strasbourg, France
| | - Guy Schleyer
- Department of Biomolecular Chemistry, Leibniz Institute for Natural Product Research and Infection Biology (Leibniz-HKI), 07745 Jena, Germany
| | - Zipora Tietel
- Department of Food Science, Gilat Research Center, Agricultural Research Organization, Volcani Institute, M.P. Negev 8531100, Israel
| | - Gabrielle Zammit
- Laboratory of Applied Phycology, Department of Biology, University of Malta, Msida MSD 2080, Malta
| | - Carmit Ziv
- Department of Postharvest Science, Agricultural Research Organization, Volcani Institute, Rishon LeZion 7505101, Israel
| | - Rosário Domingues
- Mass Spectrometry Centre, LAQV-REQUIMTE, Department of Chemistry, University of Aveiro, Santiago University Campus, Aveiro 3810-193, Portugal; CESAM-Centre for Environmental and Marine Studies, Department of Chemistry, University of Aveiro, Santiago University Campus, Aveiro 3810-193, Portugal.
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Cao X, Cong P, Song Y, Meng N, Fan X, Liu Y, Wang X, Xu J, Xue C. Comprehensive Lipidomic Analysis of Three Edible Microalgae Species Based on RPLC-Q-TOF-MS/MS. JOURNAL OF AGRICULTURAL AND FOOD CHEMISTRY 2024. [PMID: 39022817 DOI: 10.1021/acs.jafc.4c01897] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Subscribe] [Scholar Register] [Indexed: 07/20/2024]
Abstract
Microalgae, integral to marine ecosystems for their rich nutrient content, notably lipids and proteins, were investigated by using reversed-phase liquid chromatography coupled with quadrupole time-of-flight mass spectrometry (RPLC-Q-TOF-MS/MS). This study focused on lipid composition in three commonly used microalgae species (Spirulina platensis, Chlorella vulgaris, and Schizochytrium limacinum) for functional food applications. The analysis unveiled more than 700 lipid molecular species, including glycolipids (GLs), phospholipids (PLs), sphingolipids (SLs), glycerolipids, and betaine lipids (BLs). GLs (19.9-64.8%) and glycerolipids (24.1-70.4%) comprised the primary lipid. Some novel lipid content, such as acylated monogalactosyldiacylglycerols (acMGDG) and acylated digalactosyldiacylglycerols (acDGDG), ranged from 0.62 to 9.68%. The analysis revealed substantial GLs, PLs, and glycerolipid variations across microalgae species. Notably, S. platensis and C. vulgaris displayed a predominance of fatty acid (FA) 18:2 and FA 18:3 in GLs, while S. limacinum exhibited a prevalence of FA 16:0, collectively constituting over 60% of the FAs of GLs. In terms of PLs and glycerolipids, S. platensis and C. vulgaris displayed elevated levels of arachidonic acid (AA) and eicosapentaenoic acid (EPA), whereas S. limacinum exhibited a significant presence of docosahexaenoic acid (DHA). Principal component analysis (PCA) revealed MGDG (16:0/18:1), DG (16:0/22:5), Cer (d18:1/20:0), and LPC (16:1) as promising lipid markers for discriminating between these microalgae samples. This study contributes to a comprehensive understanding of lipid profiles in three microalgae species, emphasizing their distinct biochemical characteristics and potentially informing us of their high-value utilization in the food industry.
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Affiliation(s)
- Xinyu Cao
- State Key Laboratory of Marine Food Processing & Safety Control, College of Food Science and Engineering, Ocean University of China, No. 1299, Sansha Road, Qingdao, Shandong Province266003, China
| | - Peixu Cong
- State Key Laboratory of Marine Food Processing & Safety Control, College of Food Science and Engineering, Ocean University of China, No. 1299, Sansha Road, Qingdao, Shandong Province266003, China
| | - Yu Song
- State Key Laboratory of Marine Food Processing & Safety Control, College of Food Science and Engineering, Ocean University of China, No. 1299, Sansha Road, Qingdao, Shandong Province266003, China
| | - Nan Meng
- State Key Laboratory of Marine Food Processing & Safety Control, College of Food Science and Engineering, Ocean University of China, No. 1299, Sansha Road, Qingdao, Shandong Province266003, China
| | - Xiaowei Fan
- State Key Laboratory of Marine Food Processing & Safety Control, College of Food Science and Engineering, Ocean University of China, No. 1299, Sansha Road, Qingdao, Shandong Province266003, China
| | - Yanjun Liu
- State Key Laboratory of Marine Food Processing & Safety Control, College of Food Science and Engineering, Ocean University of China, No. 1299, Sansha Road, Qingdao, Shandong Province266003, China
| | - Xiaoxu Wang
- State Key Laboratory of Marine Food Processing & Safety Control, College of Food Science and Engineering, Ocean University of China, No. 1299, Sansha Road, Qingdao, Shandong Province266003, China
| | - Jie Xu
- State Key Laboratory of Marine Food Processing & Safety Control, College of Food Science and Engineering, Ocean University of China, No. 1299, Sansha Road, Qingdao, Shandong Province266003, China
| | - Changhu Xue
- State Key Laboratory of Marine Food Processing & Safety Control, College of Food Science and Engineering, Ocean University of China, No. 1299, Sansha Road, Qingdao, Shandong Province266003, China
- Qingdao Marine Science and Technology Center, Qingdao 266235, China
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Barnes AC, Myers JL, Surber SM, Liang Z, Mower JP, Schnable JC, Roston RL. Oligogalactolipid production during cold challenge is conserved in early diverging lineages. JOURNAL OF EXPERIMENTAL BOTANY 2023; 74:5405-5417. [PMID: 37357909 PMCID: PMC10848234 DOI: 10.1093/jxb/erad241] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Grants] [Track Full Text] [Subscribe] [Scholar Register] [Received: 11/14/2022] [Accepted: 06/23/2023] [Indexed: 06/27/2023]
Abstract
Severe cold, defined as a damaging cold beyond acclimation temperatures, has unique responses, but the signaling and evolution of these responses are not well understood. Production of oligogalactolipids, which is triggered by cytosolic acidification in Arabidopsis (Arabidopsis thaliana), contributes to survival in severe cold. Here, we investigated oligogalactolipid production in species from bryophytes to angiosperms. Production of oligogalactolipids differed within each clade, suggesting multiple evolutionary origins of severe cold tolerance. We also observed greater oligogalactolipid production in control samples than in temperature-challenged samples of some species. Further examination of representative species revealed a tight association between temperature, damage, and oligogalactolipid production that scaled with the cold tolerance of each species. Based on oligogalactolipid production and transcript changes, multiple angiosperm species share a signal of oligogalactolipid production initially described in Arabidopsis, namely cytosolic acidification. Together, these data suggest that oligogalactolipid production is a severe cold response that originated from an ancestral damage response that remains in many land plant lineages and that cytosolic acidification may be a common signaling mechanism for its activation.
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Affiliation(s)
- Allison C Barnes
- Department of Biochemistry, University of Nebraska-Lincoln, Lincoln, NE, USA
| | - Jennifer L Myers
- Department of Biochemistry, University of Nebraska-Lincoln, Lincoln, NE, USA
- Department of Horticulture, North Carolina State University, Raleigh, NC, USA
| | - Samantha M Surber
- Department of Biochemistry, University of Nebraska-Lincoln, Lincoln, NE, USA
| | - Zhikai Liang
- Department of Agronomy and Horticulture, University of Nebraska-Lincoln, Lincoln, NE, USA
| | - Jeffrey P Mower
- Department of Agronomy and Horticulture, University of Nebraska-Lincoln, Lincoln, NE, USA
| | - James C Schnable
- Department of Agronomy and Horticulture, University of Nebraska-Lincoln, Lincoln, NE, USA
| | - Rebecca L Roston
- Department of Biochemistry, University of Nebraska-Lincoln, Lincoln, NE, USA
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Schneider S, Hammann S, Hayen H. Determination of Polar Lipids in Wheat and Oat by a Complementary Approach of Hydrophilic Interaction Liquid Chromatography and Reversed-Phase High-Performance Liquid Chromatography Hyphenated with High-Resolution Mass Spectrometry. JOURNAL OF AGRICULTURAL AND FOOD CHEMISTRY 2023. [PMID: 37433133 DOI: 10.1021/acs.jafc.3c02073] [Citation(s) in RCA: 2] [Impact Index Per Article: 2.0] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Subscribe] [Scholar Register] [Indexed: 07/13/2023]
Abstract
Cereals contain lipids that fulfill important physiological roles and are associated with stress in the plant. However, many of the specific biological roles of lipids are yet unknown. Comprehensive analysis of these polar lipid categories in whole grain wheat and oat, cereals highly relevant also in nutrition, was performed. Hydrophilic interaction liquid chromatography (HILIC) and reversed-phase high-performance liquid chromatography (RP-HPLC) coupled with high-resolution mass spectrometry using electrospray ionization in both positive and negative ionization mode was used. Exploiting the different separation mechanisms, HILIC was used as a screening method for straightforward lipid class assignment and enabled differentiation of isomeric lipid classes, like phosphatidylethanolamine and lyso-N-acylphosphatidylethanolamine, while RP-HPLC facilitated separation of constitutional isomers. In combination with data-dependent MS/MS experiments, 67 lipid species belonging to nine polar lipid classes could be identified. Furthermore, with both ionization modes, fatty acyl chains directly connected to the lipid headgroups could be assigned. This work focused on the four lipid classes N-acylphosphatidylethanolamines, acyl-monogalactosyldiacylglycerols, digalactosyldiacylglycerols, and monogalactosyldiacylglycerols as they were less studied in detail in the past. Applying the complementary approach, the relative lipid species compositions in these lipid classes was investigated in detail.
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Affiliation(s)
- Svenja Schneider
- Institute of Inorganic and Analytical Chemistry, University of Münster, Corrensstraße 48, 48149 Münster, Germany
| | - Simon Hammann
- Department of Chemistry and Pharmacy, Friedrich-Alexander-Universität Erlangen-Nürnberg, Nikolaus-Fiebiger-Str. 10, 91058 Erlangen, Germany
| | - Heiko Hayen
- Institute of Inorganic and Analytical Chemistry, University of Münster, Corrensstraße 48, 48149 Münster, Germany
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Knieper M, Viehhauser A, Dietz KJ. Oxylipins and Reactive Carbonyls as Regulators of the Plant Redox and Reactive Oxygen Species Network under Stress. Antioxidants (Basel) 2023; 12:antiox12040814. [PMID: 37107189 PMCID: PMC10135161 DOI: 10.3390/antiox12040814] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Abstract] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 03/01/2023] [Revised: 03/20/2023] [Accepted: 03/22/2023] [Indexed: 03/29/2023] Open
Abstract
Reactive oxygen species (ROS), and in particular H2O2, serve as essential second messengers at low concentrations. However, excessive ROS accumulation leads to severe and irreversible cell damage. Hence, control of ROS levels is needed, especially under non-optimal growth conditions caused by abiotic or biotic stresses, which at least initially stimulate ROS synthesis. A complex network of thiol-sensitive proteins is instrumental in realizing tight ROS control; this is called the redox regulatory network. It consists of sensors, input elements, transmitters, and targets. Recent evidence revealed that the interplay of the redox network and oxylipins–molecules derived from oxygenation of polyunsaturated fatty acids, especially under high ROS levels–plays a decisive role in coupling ROS generation and subsequent stress defense signaling pathways in plants. This review aims to provide a broad overview of the current knowledge on the interaction of distinct oxylipins generated enzymatically (12-OPDA, 4-HNE, phytoprostanes) or non-enzymatically (MDA, acrolein) and components of the redox network. Further, recent findings on the contribution of oxylipins to environmental acclimatization will be discussed using flooding, herbivory, and establishment of thermotolerance as prime examples of relevant biotic and abiotic stresses.
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Pranneshraj V, Sangha MK, Djalovic I, Miladinovic J, Djanaguiraman M. Lipidomics-Assisted GWAS (lGWAS) Approach for Improving High-Temperature Stress Tolerance of Crops. Int J Mol Sci 2022; 23:ijms23169389. [PMID: 36012660 PMCID: PMC9409476 DOI: 10.3390/ijms23169389] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 07/19/2022] [Revised: 08/08/2022] [Accepted: 08/12/2022] [Indexed: 11/25/2022] Open
Abstract
High-temperature stress (HT) over crop productivity is an important environmental factor demanding more attention as recent global warming trends are alarming and pose a potential threat to crop production. According to the Sixth IPCC report, future years will have longer warm seasons and frequent heat waves. Thus, the need arises to develop HT-tolerant genotypes that can be used to breed high-yielding crops. Several physiological, biochemical, and molecular alterations are orchestrated in providing HT tolerance to a genotype. One mechanism to counter HT is overcoming high-temperature-induced membrane superfluidity and structural disorganizations. Several HT lipidomic studies on different genotypes have indicated the potential involvement of membrane lipid remodelling in providing HT tolerance. Advances in high-throughput analytical techniques such as tandem mass spectrometry have paved the way for large-scale identification and quantification of the enormously diverse lipid molecules in a single run. Physiological trait-based breeding has been employed so far to identify and select HT tolerant genotypes but has several disadvantages, such as the genotype-phenotype gap affecting the efficiency of identifying the underlying genetic association. Tolerant genotypes maintain a high photosynthetic rate, stable membranes, and membrane-associated mechanisms. In this context, studying the HT-induced membrane lipid remodelling, resultant of several up-/down-regulations of genes and post-translational modifications, will aid in identifying potential lipid biomarkers for HT tolerance/susceptibility. The identified lipid biomarkers (LIPIDOTYPE) can thus be considered an intermediate phenotype, bridging the gap between genotype–phenotype (genotype–LIPIDOTYPE–phenotype). Recent works integrating metabolomics with quantitative genetic studies such as GWAS (mGWAS) have provided close associations between genotype, metabolites, and stress-tolerant phenotypes. This review has been sculpted to provide a potential workflow that combines MS-based lipidomics and the robust GWAS (lipidomics assisted GWAS-lGWAS) to identify membrane lipid remodelling related genes and associations which can be used to develop HS tolerant genotypes with enhanced membrane thermostability (MTS) and heat stable photosynthesis (HP).
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Affiliation(s)
- Velumani Pranneshraj
- Department of Biochemistry, Punjab Agricultural University, Ludhiana 141004, India
| | - Manjeet Kaur Sangha
- Department of Biochemistry, Punjab Agricultural University, Ludhiana 141004, India
| | - Ivica Djalovic
- Institute of Field and Vegetable Crops, National Institute of the Republic of Serbia, Maxim Gorki 30, 21000 Novi Sad, Serbia
- Correspondence: (I.D.); (M.D.)
| | - Jegor Miladinovic
- Institute of Field and Vegetable Crops, National Institute of the Republic of Serbia, Maxim Gorki 30, 21000 Novi Sad, Serbia
| | - Maduraimuthu Djanaguiraman
- Department of Crop Physiology, Tamil Nadu Agricultural University, Coimbatore 641003, India
- Correspondence: (I.D.); (M.D.)
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Specific Changes in Arabidopsis thaliana Rosette Lipids during Freezing Can Be Associated with Freezing Tolerance. Metabolites 2022; 12:metabo12050385. [PMID: 35629889 PMCID: PMC9145600 DOI: 10.3390/metabo12050385] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 03/17/2022] [Revised: 04/14/2022] [Accepted: 04/19/2022] [Indexed: 01/21/2023] Open
Abstract
While the roles of a few specific lipids in plant freezing tolerance are understood, the effect of many plant lipids remains to be determined. Acclimation of plants to non-freezing cold before exposure to freezing temperatures improves the outcome of plants, compared to plants exposed to freezing without acclimation. Arabidopsis thaliana plants were subjected to one of three treatments: (1) "control", i.e., growth at 21 °C, (2) "non-acclimated", i.e., 3 days at 21 °C, 2 h at -8 °C, and 24 h recovery at 21 °C, and (3) "acclimated", i.e., 3 days at 4 °C, 2 h at -8 °C, and 24 h recovery at 21 °C. Plants were harvested at seven time points during the treatments, and lipid levels were measured by direct-infusion electrospray ionization tandem mass spectrometry. Ion leakage was measured at the same time points. To examine the function of lipid species in relation to freezing tolerance, the lipid levels in plants immediately following the freezing treatment were correlated with the outcome, i.e., ion leakage 24-h post-freezing. Based on the correlations, hypotheses about the functions of specific lipids were generated. Additionally, analysis of the lipid levels in plants with mutations in genes encoding patatin-like phospholipases, lipoxygenases, and 12-oxophytodienoic acid reductase 3 (opr3), under the same treatments as the wild-type plants, identified only the opr3-2 mutant as having major lipid compositional differences compared to wild-type plants.
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Kehelpannala C, Rupasinghe T, Hennessy T, Bradley D, Ebert B, Roessner U. The state of the art in plant lipidomics. Mol Omics 2021; 17:894-910. [PMID: 34699583 DOI: 10.1039/d1mo00196e] [Citation(s) in RCA: 4] [Impact Index Per Article: 1.3] [Reference Citation Analysis] [Abstract] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 01/08/2023]
Abstract
Lipids are a group of compounds with diverse structures that perform several important functions in plants. To unravel and better understand their in vivo functions, plant biologists have been using various lipidomic technologies including liquid-chromatography (LC)-mass spectrometry (MS). However, there are still significant challenges in LC-MS based plant lipidomics, which need to be addressed. In this review, we provide an overview of the key developments in LC-MS based lipidomic approaches to detect and identify plant lipids with emphasis on areas that can be further improved. Given that the cellular lipidome is estimated to contain hundreds of thousands of lipids,1,2 many of the lipid structures remain to be discovered. Furthermore, the plant lipidome is considered to be significantly more complex compared to that of mammals. Recent technical developments in mass spectrometry have made the detection of novel lipids possible; hence, approaches that can be used for plant lipid discovery are also discussed.
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Affiliation(s)
- Cheka Kehelpannala
- School of BioSciences, The University of Melbourne, Melbourne, VIC 3010, Australia.
| | | | - Thomas Hennessy
- Agilent Technologies Australia Pty Ltd, 679 Springvale Road, Mulgrave, VIC 3170, Australia
| | - David Bradley
- Agilent Technologies Australia Pty Ltd, 679 Springvale Road, Mulgrave, VIC 3170, Australia
| | - Berit Ebert
- School of BioSciences, The University of Melbourne, Melbourne, VIC 3010, Australia.
| | - Ute Roessner
- School of BioSciences, The University of Melbourne, Melbourne, VIC 3010, Australia.
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Ventura G, Calvano CD, Cinquepalmi V, Losito I, Cataldi TRI. Characterization of Glucuronosyl-diacyl/monoacylglycerols and Discovery of Their Acylated Derivatives in Tomato Lipid Extracts by Reversed-Phase Liquid Chromatography with Electrospray Ionization and Tandem Mass Spectrometry. JOURNAL OF THE AMERICAN SOCIETY FOR MASS SPECTROMETRY 2021; 32:2227-2240. [PMID: 34260857 DOI: 10.1021/jasms.1c00162] [Citation(s) in RCA: 1] [Impact Index Per Article: 0.3] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Track Full Text] [Subscribe] [Scholar Register] [Indexed: 06/13/2023]
Abstract
Glucuronic acid containing diacylglycerols (3-(O-α-d-glucuronopyranosyl)-1,2-diacyl-sn-glycerols, GlcA-DAG) are glycolipids of plant membranes especially formed under phosphate-depletion conditions. An analytical approach for the structural characterization of GlcA-DAG in red ripe tomato (Solanum lycopersicum L.) extracts, based on reversed-phase liquid chromatography (RPLC) coupled with electrospray ionization (ESI) and tandem mass spectrometry (MS/MS) using a linear ion trap, is described in this paper. At least 14 GlcA-DAG (R1/R2) species, including four regioisomers, containing three predominant fatty acyl chains C16:0, C18:2, and C18:3, were identified for the first time. Moreover, 29 GlcA-DAG acylated on the glucuronosyl ring (acyl-R3 GlcA-DAG) were discovered, alongside 15 acylated lyso-forms, i.e., acylated 3-(O-α-d-glucuronosyl)monoacylglycerols, abbreviated as acyl-R3 GlcA-MAG (R1/0) or (0/R2). Although many of these acylated lyso-forms were isomeric with GlcA-DAG (i.e., acyl chains with equivalent sum composition), they were successfully separated by reversed-phase liquid chromatography (RPLC) using a solid-core C18 column packed with 2.6 μm particle size. Tandem MS (and eventually MS3) data obtained from sodium adducts ([M + Na]+) and deprotonated molecules ([M - H]-) were fundamental to detect diagnostic product ions related to the glucuronosyl ring and then determine the identity of all investigated glycolipids, especially to recognize the acyl chain linked to the ring. A classification of GlcA-MAG, GlcA-DAG, and acylated GlcA-DAG and GlcA-MAG was generated by an in house-built database. The discovery of acylated derivatives emphasized the already surprising heterogeneity of glucuronic acid-containing mono- and diacylglycerols in tomato plants, stimulating interesting questions on the role played by these glycolipids.
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Yu L, Zhou C, Fan J, Shanklin J, Xu C. Mechanisms and functions of membrane lipid remodeling in plants. THE PLANT JOURNAL : FOR CELL AND MOLECULAR BIOLOGY 2021; 107:37-53. [PMID: 33853198 DOI: 10.1111/tpj.15273] [Citation(s) in RCA: 65] [Impact Index Per Article: 21.7] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Track Full Text] [Subscribe] [Scholar Register] [Received: 02/25/2021] [Revised: 04/05/2021] [Accepted: 04/08/2021] [Indexed: 05/20/2023]
Abstract
Lipid remodeling, defined herein as post-synthetic structural modifications of membrane lipids, play crucial roles in regulating the physicochemical properties of cellular membranes and hence their many functions. Processes affected by lipid remodeling include lipid metabolism, membrane repair, cellular homeostasis, fatty acid trafficking, cellular signaling and stress tolerance. Glycerolipids are the major structural components of cellular membranes and their composition can be adjusted by modifying their head groups, their acyl chain lengths and the number and position of double bonds. This review summarizes recent advances in our understanding of mechanisms of membrane lipid remodeling with emphasis on the lipases and acyltransferases involved in the modification of phosphatidylcholine and monogalactosyldiacylglycerol, the major membrane lipids of extraplastidic and photosynthetic membranes, respectively. We also discuss the role of triacylglycerol metabolism in membrane acyl chain remodeling. Finally, we discuss emerging data concerning the functional roles of glycerolipid remodeling in plant stress responses. Illustrating the molecular basis of lipid remodeling may lead to novel strategies for crop improvement and other biotechnological applications such as bioenergy production.
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Affiliation(s)
- Linhui Yu
- Biology Department, Brookhaven National Laboratory, Upton, NY, 11973, USA
| | - Chao Zhou
- Biology Department, Brookhaven National Laboratory, Upton, NY, 11973, USA
| | - Jilian Fan
- Biology Department, Brookhaven National Laboratory, Upton, NY, 11973, USA
| | - John Shanklin
- Biology Department, Brookhaven National Laboratory, Upton, NY, 11973, USA
| | - Changcheng Xu
- Biology Department, Brookhaven National Laboratory, Upton, NY, 11973, USA
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11
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Song Y, Zoong Lwe ZS, Wickramasinghe PADBV, Welti R. Head-Group Acylation of Chloroplast Membrane Lipids. Molecules 2021; 26:molecules26051273. [PMID: 33652855 PMCID: PMC7956594 DOI: 10.3390/molecules26051273] [Citation(s) in RCA: 2] [Impact Index Per Article: 0.7] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 01/30/2021] [Revised: 02/23/2021] [Accepted: 02/24/2021] [Indexed: 01/24/2023] Open
Abstract
Head group-acylated chloroplast lipids were discovered in the 1960s, but interest was renewed about 15 years ago with the discovery of Arabidopsides E and G, acylated monogalactosyldiacylglycerols with oxidized fatty acyl chains originally identified in Arabidopsis thaliana. Since then, plant biologists have applied the power of mass spectrometry to identify additional oxidized and non-oxidized chloroplast lipids and quantify their levels in response to biotic and abiotic stresses. The enzyme responsible for the head-group acylation of chloroplast lipids was identified as a cytosolic protein closely associated with the chloroplast outer membrane and christened acylated galactolipid-associated phospholipase 1 (AGAP1). Despite many advances, critical questions remain about the biological functions of AGAP1 and its head group-acylated products.
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Affiliation(s)
- Yu Song
- Department of Biochemistry and Molecular Biophysics, Kansas State University, Manhattan, KS 66506, USA; (Y.S.); (Z.S.Z.L.)
- Kansas Lipidomics Research Center, Kansas State University, Manhattan, KS 66506, USA;
| | - Zolian S. Zoong Lwe
- Department of Biochemistry and Molecular Biophysics, Kansas State University, Manhattan, KS 66506, USA; (Y.S.); (Z.S.Z.L.)
- Kansas Lipidomics Research Center, Kansas State University, Manhattan, KS 66506, USA;
| | | | - Ruth Welti
- Kansas Lipidomics Research Center, Kansas State University, Manhattan, KS 66506, USA;
- Division of Biology, Kansas State University, Manhattan, KS 66506, USA
- Correspondence:
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12
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Genva M, Andersson MX, Fauconnier ML. Simple liquid chromatography-electrospray ionization ion trap mass spectrometry method for the quantification of galacto-oxylipin arabidopsides in plant samples. Sci Rep 2020; 10:11957. [PMID: 32686714 PMCID: PMC7371884 DOI: 10.1038/s41598-020-68757-x] [Citation(s) in RCA: 3] [Impact Index Per Article: 0.8] [Reference Citation Analysis] [Abstract] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 04/02/2020] [Accepted: 06/29/2020] [Indexed: 11/13/2022] Open
Abstract
A simple and sensitive method to quantify five different arabidopsides by HPLC—ion trap mass spectrometry in complex plant samples was developed and validated. Arabidopsides are oxidized galactolipids first described in Arabidopsis thaliana but also produced by other plant species under stress conditions. External calibration was performed using arabidopsides purified from freeze-thawed Arabidopsis leaves. Lipids were extracted and pre-purified on an SPE silica column before HPLC–MS analysis. Arabidopsides were separated on a C18 column using a gradient of mQ water and acetonitrile:mQ water (85:15) supplemented with formic acid (0.2%) and ammonium formate (12 mM). The method was validated according to European commission decision 2002/657/CE. LOD, LOQ, linearity, intra-day and inter-day precision and accuracy, selectivity, matrix effects and recoveries were determined for the five metabolites. The established method is highly selective in a complex plant matrix. LOD and LOQ were, respectively, in the range 0.098–0.78 and 0.64–1.56 µM, allowing the arabidopside quantification from 25.6–62.4 nmol/g fresh weight. Calibration curve correlation coefficients were higher than 0.997. Matrix effects ranged from -2.09% to 6.10% and recoveries between 70.7% and 109%. The method was successfully applied to complex plant matrixes: Arabidopsis thaliana and Nasturtium officinale.
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Affiliation(s)
- Manon Genva
- Laboratory of Chemistry of Natural Molecules, Gembloux Agro-Bio Tech, University of Liège, Passage des Déportés 2, 5030, Gembloux, Belgium.
| | - Mats X Andersson
- Department of Biological and Environmental Sciences, University of Gothenburg, Box 461, 405 30, Göteborg, Sweden
| | - Marie-Laure Fauconnier
- Laboratory of Chemistry of Natural Molecules, Gembloux Agro-Bio Tech, University of Liège, Passage des Déportés 2, 5030, Gembloux, Belgium
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13
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Shiva S, Samarakoon T, Lowe KA, Roach C, Vu HS, Colter M, Porras H, Hwang C, Roth MR, Tamura P, Li M, Schrick K, Shah J, Wang X, Wang H, Welti R. Leaf Lipid Alterations in Response to Heat Stress of Arabidopsis thaliana. PLANTS 2020; 9:plants9070845. [PMID: 32635518 PMCID: PMC7412450 DOI: 10.3390/plants9070845] [Citation(s) in RCA: 28] [Impact Index Per Article: 7.0] [Reference Citation Analysis] [Abstract] [Key Words] [Grants] [Track Full Text] [Download PDF] [Figures] [Subscribe] [Scholar Register] [Received: 06/14/2020] [Revised: 06/30/2020] [Accepted: 07/03/2020] [Indexed: 01/19/2023]
Abstract
In response to elevated temperatures, plants alter the activities of enzymes that affect lipid composition. While it has long been known that plant leaf membrane lipids become less unsaturated in response to heat, other changes, including polygalactosylation of galactolipids, head group acylation of galactolipids, increases in phosphatidic acid and triacylglycerols, and formation of sterol glucosides and acyl sterol glucosides, have been observed more recently. In this work, by measuring lipid levels with mass spectrometry, we confirm the previously observed changes in Arabidopsis thaliana leaf lipids under three heat stress regimens. Additionally, in response to heat, increased oxidation of the fatty acyl chains of leaf galactolipids, sulfoquinovosyldiacylglycerols, and phosphatidylglycerols, and incorporation of oxidized acyl chains into acylated monogalactosyldiacylglycerols are shown. We also observed increased levels of digalactosylmonoacylglycerols and monogalactosylmonoacylglycerols. The hypothesis that a defect in sterol glycosylation would adversely affect regrowth of plants after a severe heat stress regimen was tested, but differences between wild-type and sterol glycosylation-defective plants were not detected.
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Affiliation(s)
- Sunitha Shiva
- Division of Biology, Kansas State University, Ackert Hall, Manhattan, KS 66506-4901, USA; (T.S.); (K.A.L.); (C.R.); (H.S.V.); (M.C.); (H.P.); (C.H.); (M.R.R.); (P.T.); (K.S.)
- Correspondence: (S.S.); (R.W.)
| | - Thilani Samarakoon
- Division of Biology, Kansas State University, Ackert Hall, Manhattan, KS 66506-4901, USA; (T.S.); (K.A.L.); (C.R.); (H.S.V.); (M.C.); (H.P.); (C.H.); (M.R.R.); (P.T.); (K.S.)
| | - Kaleb A. Lowe
- Division of Biology, Kansas State University, Ackert Hall, Manhattan, KS 66506-4901, USA; (T.S.); (K.A.L.); (C.R.); (H.S.V.); (M.C.); (H.P.); (C.H.); (M.R.R.); (P.T.); (K.S.)
| | - Charles Roach
- Division of Biology, Kansas State University, Ackert Hall, Manhattan, KS 66506-4901, USA; (T.S.); (K.A.L.); (C.R.); (H.S.V.); (M.C.); (H.P.); (C.H.); (M.R.R.); (P.T.); (K.S.)
| | - Hieu Sy Vu
- Division of Biology, Kansas State University, Ackert Hall, Manhattan, KS 66506-4901, USA; (T.S.); (K.A.L.); (C.R.); (H.S.V.); (M.C.); (H.P.); (C.H.); (M.R.R.); (P.T.); (K.S.)
| | - Madeline Colter
- Division of Biology, Kansas State University, Ackert Hall, Manhattan, KS 66506-4901, USA; (T.S.); (K.A.L.); (C.R.); (H.S.V.); (M.C.); (H.P.); (C.H.); (M.R.R.); (P.T.); (K.S.)
| | - Hollie Porras
- Division of Biology, Kansas State University, Ackert Hall, Manhattan, KS 66506-4901, USA; (T.S.); (K.A.L.); (C.R.); (H.S.V.); (M.C.); (H.P.); (C.H.); (M.R.R.); (P.T.); (K.S.)
| | - Caroline Hwang
- Division of Biology, Kansas State University, Ackert Hall, Manhattan, KS 66506-4901, USA; (T.S.); (K.A.L.); (C.R.); (H.S.V.); (M.C.); (H.P.); (C.H.); (M.R.R.); (P.T.); (K.S.)
| | - Mary R. Roth
- Division of Biology, Kansas State University, Ackert Hall, Manhattan, KS 66506-4901, USA; (T.S.); (K.A.L.); (C.R.); (H.S.V.); (M.C.); (H.P.); (C.H.); (M.R.R.); (P.T.); (K.S.)
| | - Pamela Tamura
- Division of Biology, Kansas State University, Ackert Hall, Manhattan, KS 66506-4901, USA; (T.S.); (K.A.L.); (C.R.); (H.S.V.); (M.C.); (H.P.); (C.H.); (M.R.R.); (P.T.); (K.S.)
| | - Maoyin Li
- Department of Biological Sciences, University of North Texas, Denton, TX 76203-5017, USA; (M.L.); (X.W.)
- Department of Biology, University of Missouri-St. Louis, St. Louis, MO 63121-4499, USA
| | - Kathrin Schrick
- Division of Biology, Kansas State University, Ackert Hall, Manhattan, KS 66506-4901, USA; (T.S.); (K.A.L.); (C.R.); (H.S.V.); (M.C.); (H.P.); (C.H.); (M.R.R.); (P.T.); (K.S.)
| | - Jyoti Shah
- Donald Danforth Plant Science Center, St. Louis, MO 63132, USA;
| | - Xuemin Wang
- Department of Biological Sciences, University of North Texas, Denton, TX 76203-5017, USA; (M.L.); (X.W.)
- Department of Biology, University of Missouri-St. Louis, St. Louis, MO 63121-4499, USA
| | - Haiyan Wang
- Department of Statistics, Kansas State University, Manhattan, KS 66506-0802, USA;
| | - Ruth Welti
- Division of Biology, Kansas State University, Ackert Hall, Manhattan, KS 66506-4901, USA; (T.S.); (K.A.L.); (C.R.); (H.S.V.); (M.C.); (H.P.); (C.H.); (M.R.R.); (P.T.); (K.S.)
- Correspondence: (S.S.); (R.W.)
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14
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Kytidou K, Artola M, Overkleeft HS, Aerts JMFG. Plant Glycosides and Glycosidases: A Treasure-Trove for Therapeutics. FRONTIERS IN PLANT SCIENCE 2020; 11:357. [PMID: 32318081 PMCID: PMC7154165 DOI: 10.3389/fpls.2020.00357] [Citation(s) in RCA: 50] [Impact Index Per Article: 12.5] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Subscribe] [Scholar Register] [Received: 12/23/2019] [Accepted: 03/11/2020] [Indexed: 05/10/2023]
Abstract
Plants contain numerous glycoconjugates that are metabolized by specific glucosyltransferases and hydrolyzed by specific glycosidases, some also catalyzing synthetic transglycosylation reactions. The documented value of plant-derived glycoconjugates to beneficially modulate metabolism is first addressed. Next, focus is given to glycosidases, the central theme of the review. The therapeutic value of plant glycosidases is discussed as well as the present production in plant platforms of therapeutic human glycosidases used in enzyme replacement therapies. The increasing knowledge on glycosidases, including structure and catalytic mechanism, is described. The novel insights have allowed the design of functionalized highly specific suicide inhibitors of glycosidases. These so-called activity-based probes allow unprecedented visualization of glycosidases cross-species. Here, special attention is paid on the use of such probes in plant science that promote the discovery of novel enzymes and the identification of potential therapeutic inhibitors and chaperones.
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Affiliation(s)
- Kassiani Kytidou
- Department of Medical Biochemistry, Leiden Institute of Chemistry, Leiden University, Leiden, Netherlands
| | - Marta Artola
- Department of Medical Biochemistry, Leiden Institute of Chemistry, Leiden University, Leiden, Netherlands
- Department of Bio-organic Synthesis, Leiden Institute of Chemistry, Leiden University, Leiden, Netherlands
| | - Herman S. Overkleeft
- Department of Bio-organic Synthesis, Leiden Institute of Chemistry, Leiden University, Leiden, Netherlands
| | - Johannes M. F. G. Aerts
- Department of Medical Biochemistry, Leiden Institute of Chemistry, Leiden University, Leiden, Netherlands
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15
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Lipidomic studies of membrane glycerolipids in plant leaves under heat stress. Prog Lipid Res 2019; 75:100990. [DOI: 10.1016/j.plipres.2019.100990] [Citation(s) in RCA: 55] [Impact Index Per Article: 11.0] [Reference Citation Analysis] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 03/22/2019] [Revised: 06/13/2019] [Accepted: 07/14/2019] [Indexed: 12/29/2022]
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16
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Abstract
Chloroplasts contain high amounts of monogalactosyldiacylglycerol (MGDG) and digalactosyldiacylglycerol (DGDG) and low levels of the anionic lipids sulfoquinovosyldiacylglycerol (SQDG), phosphatidylglycerol (PG), and glucuronosyldiacylglycerol (GlcADG). The mostly extraplastidial lipid phosphatidylcholine is found only in the outer envelope. Chloroplasts are the major site for fatty acid synthesis. In Arabidopsis, a certain proportion of glycerolipids is entirely synthesized in the chloroplast (prokaryotic lipids). Fatty acids are also exported to the endoplasmic reticulum and incorporated into lipids that are redistributed to the chloroplast (eukaryotic lipids). MGDG, DGDG, SQDG, and PG establish the thylakoid membranes and are integral constituents of the photosynthetic complexes. Phosphate deprivation induces phospholipid degradation accompanied by the increase in DGDG, SQDG, and GlcADG. During freezing and drought stress, envelope membranes are stabilized by the conversion of MGDG into oligogalactolipids. Senescence and chlorotic stress lead to lipid and chlorophyll degradation and the deposition of acyl and phytyl moieties as fatty acid phytyl esters.
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Affiliation(s)
- Georg Hölzl
- Institute of Molecular Physiology and Biotechnology of Plants (IMBIO), University of Bonn, 53115 Bonn, Germany;
| | - Peter Dörmann
- Institute of Molecular Physiology and Biotechnology of Plants (IMBIO), University of Bonn, 53115 Bonn, Germany;
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17
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Chechetkin IR, Blufard AS, Yarin AY, Fedina EO, Khairutdinov BI, Grechkin AN. Detection and identification of complex oxylipins in meadow buttercup (Ranunculus acris) leaves. PHYTOCHEMISTRY 2019; 157:92-102. [PMID: 30390606 DOI: 10.1016/j.phytochem.2018.10.030] [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: 05/09/2018] [Revised: 10/05/2018] [Accepted: 10/26/2018] [Indexed: 06/08/2023]
Abstract
Screening of linolipins, i.e. galactolipids containing esterified residues of divinyl ether oxylipins, in the leaves of several higher plants revealed the presence of these complex oxylipins in the meadow buttercup leaves. The rapid accumulation of linolipins occurred in the injured leaves of meadow buttercup, while intact leaves possessed no linolipins. These oxylipins were isolated from the injured leaves, separated and purified by HPLC. The structural analyses of linolipins by UV, mass-spectroscopy and NMR spectroscopy resulted in the identification of eight molecular species. Three of them were identical to linolipins B-D found earlier in the leaves of flax (Linum usitatissimum L.). Other molecular species were identified as 1-O-(ω5Z)-etherolenoyl-2-O-dinor-(ω5Z)-etherolenoyl-3-O-β-D-galactopyranosyl-sn-glycerol, 1-O-(ω5Z)-etherolenoyl-2-O-(7Z,10Z,13Z)-hexadecatrienoyl-3-O-β-D-galactopyranosyl-sn-glycerol, 1-O-(ω5Z)-etherolenoyl-2-O-(7Z,10Z)-hexadecadienoyl-3-O-β-D-galactopyranosyl-sn-glycerol, 1-O-(ω5Z)-etherolenoyl-2-O-α-linolenoyl-3-O-β-D-galactopyranosyl-sn-glycerol, and 1-O-(ω5Z)-etherolenoyl-2-O-palmitoyl-3-O-(α-galactopyranosyl-1-6-β-D-galactopyranosyl)-sn-glycerol. The trivial names "linolipins E, F, G, H and I," respectively, have been ascribed to these novel complex oxylipins.
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Affiliation(s)
- Ivan R Chechetkin
- Kazan Institute of Biochemistry and Biophysics, FRC Kazan Scientific Center of RAS, P.O. Box 30, 420111, Kazan, Russia.
| | - Alexander S Blufard
- Kazan Institute of Biochemistry and Biophysics, FRC Kazan Scientific Center of RAS, P.O. Box 30, 420111, Kazan, Russia
| | - Andrey Y Yarin
- Kazan Institute of Biochemistry and Biophysics, FRC Kazan Scientific Center of RAS, P.O. Box 30, 420111, Kazan, Russia
| | - Evgenia O Fedina
- Kazan Institute of Biochemistry and Biophysics, FRC Kazan Scientific Center of RAS, P.O. Box 30, 420111, Kazan, Russia
| | - Bulat I Khairutdinov
- Kazan Institute of Biochemistry and Biophysics, FRC Kazan Scientific Center of RAS, P.O. Box 30, 420111, Kazan, Russia
| | - Alexander N Grechkin
- Kazan Institute of Biochemistry and Biophysics, FRC Kazan Scientific Center of RAS, P.O. Box 30, 420111, Kazan, Russia
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18
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Kenchanmane Raju SK, Barnes AC, Schnable JC, Roston RL. Low-temperature tolerance in land plants: Are transcript and membrane responses conserved? PLANT SCIENCE : AN INTERNATIONAL JOURNAL OF EXPERIMENTAL PLANT BIOLOGY 2018; 276:73-86. [PMID: 30348330 DOI: 10.1016/j.plantsci.2018.08.002] [Citation(s) in RCA: 49] [Impact Index Per Article: 8.2] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Track Full Text] [Subscribe] [Scholar Register] [Received: 04/23/2018] [Revised: 08/01/2018] [Accepted: 08/02/2018] [Indexed: 05/20/2023]
Abstract
Plants' tolerance of low temperatures is an economically and ecologically important limitation on geographic distributions and growing seasons. Tolerance for low temperatures varies significantly across different plant species, and different mechanisms likely act in different species. In order to survive low-temperature stress, plant membranes must maintain their fluidity in increasingly cold and oxidative cellular environments. The responses of different species to low-temperature stress include changes to the types and desaturation levels of membrane lipids, though the precise lipids affected tend to vary by species. Regulation of membrane dynamics and other low-temperature tolerance factors are controlled by both transcriptional and post-transcriptional mechanisms. Here, we review low-temperature induced changes in both membrane lipid composition and gene transcription across multiple related plant species with differing degrees of low-temperature tolerance. We attempt to define a core set of changes for transcripts and lipids across species and treatment variations. Some responses appear to be consistent across all species for which data are available, while many others appear likely to be species or family-specific. Potential rationales are presented, including variance in testing, reporting and the importance of considering the level of stress perceived by the plant.
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Affiliation(s)
- Sunil Kumar Kenchanmane Raju
- Center for Plant Science Innovation, University of Nebraska-Lincoln, Lincoln, Nebraska, 68588, USA; Department of Agronomy and Horticulture, University of Nebraska-Lincoln, Lincoln, Nebraska, 68588, USA
| | - Allison C Barnes
- Center for Plant Science Innovation, University of Nebraska-Lincoln, Lincoln, Nebraska, 68588, USA; Department of Biochemistry, University of Nebraska-Lincoln, Lincoln, Nebraska, 68588, USA
| | - James C Schnable
- Center for Plant Science Innovation, University of Nebraska-Lincoln, Lincoln, Nebraska, 68588, USA; Department of Agronomy and Horticulture, University of Nebraska-Lincoln, Lincoln, Nebraska, 68588, USA
| | - Rebecca L Roston
- Center for Plant Science Innovation, University of Nebraska-Lincoln, Lincoln, Nebraska, 68588, USA; Department of Biochemistry, University of Nebraska-Lincoln, Lincoln, Nebraska, 68588, USA.
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Wasternack C, Strnad M. Jasmonates: News on Occurrence, Biosynthesis, Metabolism and Action of an Ancient Group of Signaling Compounds. Int J Mol Sci 2018; 19:E2539. [PMID: 30150593 PMCID: PMC6164985 DOI: 10.3390/ijms19092539] [Citation(s) in RCA: 118] [Impact Index Per Article: 19.7] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 07/26/2018] [Revised: 08/22/2018] [Accepted: 08/22/2018] [Indexed: 02/07/2023] Open
Abstract
: Jasmonic acid (JA) and its related derivatives are ubiquitously occurring compounds of land plants acting in numerous stress responses and development. Recent studies on evolution of JA and other oxylipins indicated conserved biosynthesis. JA formation is initiated by oxygenation of α-linolenic acid (α-LeA, 18:3) or 16:3 fatty acid of chloroplast membranes leading to 12-oxo-phytodienoic acid (OPDA) as intermediate compound, but in Marchantiapolymorpha and Physcomitrellapatens, OPDA and some of its derivatives are final products active in a conserved signaling pathway. JA formation and its metabolic conversion take place in chloroplasts, peroxisomes and cytosol, respectively. Metabolites of JA are formed in 12 different pathways leading to active, inactive and partially active compounds. The isoleucine conjugate of JA (JA-Ile) is the ligand of the receptor component COI1 in vascular plants, whereas in the bryophyte M. polymorpha COI1 perceives an OPDA derivative indicating its functionally conserved activity. JA-induced gene expressions in the numerous biotic and abiotic stress responses and development are initiated in a well-studied complex regulation by homeostasis of transcription factors functioning as repressors and activators.
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Affiliation(s)
- Claus Wasternack
- Department of Molecular Signal Processing, Leibniz Institute of Plant Biochemistry, Weinberg 3, D-06120 Halle (Saale), Germany.
- Laboratory of Growth Regulators, Institute of Experimental Botany AS CR & Palacký University, Šlechtitelů 11, CZ-78371 Olomouc, Czech Republic.
| | - Miroslav Strnad
- Laboratory of Growth Regulators, Institute of Experimental Botany AS CR & Palacký University, Šlechtitelů 11, CZ-78371 Olomouc, Czech Republic.
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20
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Li HM, Yu CW. Chloroplast Galactolipids: The Link Between Photosynthesis, Chloroplast Shape, Jasmonates, Phosphate Starvation and Freezing Tolerance. PLANT & CELL PHYSIOLOGY 2018; 59:1128-1134. [PMID: 29727004 DOI: 10.1093/pcp/pcy088] [Citation(s) in RCA: 32] [Impact Index Per Article: 5.3] [Reference Citation Analysis] [Abstract] [MESH Headings] [Track Full Text] [Subscribe] [Scholar Register] [Received: 02/22/2018] [Accepted: 04/26/2018] [Indexed: 05/23/2023]
Abstract
Monogalactosyldiacylglycerol (MGDG) and digalactosyldiacylglycerol (DGDG) together constitute approximately 80% of chloroplast lipids. Apart from facilitating the photosynthesis light reaction in the thylakoid membrane, these two lipids are important for maintaining chloroplast morphology and for plant survival under abiotic stresses such as phosphate starvation and freezing. Recently it was shown that severe growth retardation phenotypes of the DGDG-deficient mutant dgd1 were due to jasmonate overproduction, linking MGDG and DGDG homeostasis with phytohormone production and suggesting MGDG as a major substrate for jasmonate biosynthesis. Induction of jasmonate synthesis and jasmonic acid (JA) signaling was also observed under conditions of phosphate starvation. We hypothesize that when DGDG is recruited to substitute for phospholipids in extraplastidic membranes during phosphate deficiency, the altered MGDG to DGDG ratio in the chloroplast envelope triggers the conversion of galactolipids into jasmonates. The conversion may contribute to rebalancing the MGDG to DGDG ratio rapidly to maintain chloroplast shape, and jasmonate production can reduce the growth rate and enhance predator deterrence. We also hypothesize that other conditions, such as suppression of dgd1 phenotypes by trigalactosyldiacylglycerol (tgd) mutations, may all be linked to altered jasmonate production, indicating that caution should be exercised when interpreting phenotypes caused by conditions that may alter the MGDG to DGDG ratio at the chloroplast envelope.
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Affiliation(s)
- Hsou-Min Li
- Institute of Molecular Biology, Academia Sinica, Nankang, Taipei 11529, Taiwan
| | - Chun-Wei Yu
- Institute of Molecular Biology, Academia Sinica, Nankang, Taipei 11529, Taiwan
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21
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Abstract
Lipids are primary metabolites used for energy storage, signal transduction, and pigmentation, besides being common membrane components. Considering the importance of comprehensive lipid analysis (lipidomics) for a detailed understanding of cellular metabolic states, this chapter introduces liquid chromatography-quadrupole time-of-flight mass spectrometry as a powerful untargeted plant lipidomics technique.
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Affiliation(s)
- Yozo Okazaki
- Metabolomics Research Group, RIKEN Center for Sustainable Resource Science, Yokohama, Japan. .,Graduate School of Bioresources, Mie University, Tsu, Mie, Japan.
| | - Kazuki Saito
- Metabolomics Research Group, RIKEN Center for Sustainable Resource Science, Yokohama, Japan.,Graduate School of Pharmaceutical Sciences, Chiba University, Chiba, Japan
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22
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Wasternack C, Song S. Jasmonates: biosynthesis, metabolism, and signaling by proteins activating and repressing transcription. JOURNAL OF EXPERIMENTAL BOTANY 2017; 68:1303-1321. [PMID: 27940470 DOI: 10.1093/jxb/erw443] [Citation(s) in RCA: 149] [Impact Index Per Article: 21.3] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Track Full Text] [Subscribe] [Scholar Register] [Received: 09/02/2016] [Accepted: 11/07/2016] [Indexed: 05/21/2023]
Abstract
The lipid-derived phytohormone jasmonate (JA) regulates plant growth, development, secondary metabolism, defense against insect attack and pathogen infection, and tolerance to abiotic stresses such as wounding, UV light, salt, and drought. JA was first identified in 1962, and since the 1980s many studies have analyzed the physiological functions, biosynthesis, distribution, metabolism, perception, signaling, and crosstalk of JA, greatly expanding our knowledge of the hormone's action. In response to fluctuating environmental cues and transient endogenous signals, the occurrence of multilayered organization of biosynthesis and inactivation of JA, and activation and repression of the COI1-JAZ-based perception and signaling contributes to the fine-tuning of JA responses. This review describes the JA biosynthetic enzymes in terms of gene families, enzymatic activity, location and regulation, substrate specificity and products, the metabolic pathways in converting JA to activate or inactivate compounds, JA signaling in perception, and the co-existence of signaling activators and repressors.
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Affiliation(s)
- Claus Wasternack
- Laboratory of Growth Regulators, Centre of the Region Haná for Biotechnological and Agricultural Research, Palacký University, Institute of Experimental Botany AS CR, Šlechtitelu 11, CZ 78371 Olomouc, Czech Republic
| | - Susheng Song
- Beijing Key Laboratory of Plant Gene Resources and Biotechnology for Carbon Reduction and Environmental Improvement, College of Life Sciences, Capital Normal University, Beijing 100048, China
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23
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Nilsson AK, Fahlberg P, Johansson ON, Hamberg M, Andersson MX, Ellerström M. The activity of HYDROPEROXIDE LYASE 1 regulates accumulation of galactolipids containing 12-oxo-phytodienoic acid in Arabidopsis. JOURNAL OF EXPERIMENTAL BOTANY 2016; 67:5133-44. [PMID: 27422994 PMCID: PMC5014160 DOI: 10.1093/jxb/erw278] [Citation(s) in RCA: 5] [Impact Index Per Article: 0.6] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Track Full Text] [Subscribe] [Scholar Register] [Indexed: 05/06/2023]
Abstract
Arabidopsis produces galactolipids containing esters of 12-oxo-phytodienoic acid (OPDA) and dinor-12-oxo-phytodienoic acid (dnOPDA). These lipids are referred to as arabidopsides and accumulate in response to abiotic and biotic stress. We explored the natural genetic variation found in 14 different Arabidopsis accessions to identify genes involved in the formation of arabidopsides. The accession C24 was identified as a poor accumulator of arabidopsides whereas the commonly used accession Col-0 was found to accumulate comparably large amounts of arabidopsides in response to tissue damage. A quantitative trait loci analysis of an F2 population created from a cross between C24 and Col-0 located a region on chromosome four strongly linked to the capacity to form arabidopsides. Expression analysis of HYDROPEROXIDE LYASE 1 (HPL1) showed large differences in transcript abundance between accessions. Transformation of Col-0 plants with the C24 HPL1 allele under transcriptional regulation of the 35S promoter revealed a strong negative correlation between HPL1 expression and arabidopside accumulation after tissue damage, thereby strengthening the view that HPL1 competes with ALLENE OXIDE SYNTHASE (AOS) for lipid-bound hydroperoxide fatty acids. We further show that the last step in the synthesis of galactolipid-bound OPDA and dnOPDA from unstable allene oxides is exclusively enzyme-catalyzed and not the result of spontaneous cyclization. Thus, the results presented here together with previous studies suggest that all steps in arabidopside biosynthesis are enzyme-dependent and apparently all reactions can take place with substrates being esterified to galactolipids.
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Affiliation(s)
- Anders K Nilsson
- Department of Biological and Environmental Sciences, University of Gothenburg, Box 461, SE-405 30 Göteborg, Sweden
| | - Per Fahlberg
- Department of Biological and Environmental Sciences, University of Gothenburg, Box 461, SE-405 30 Göteborg, Sweden
| | - Oskar N Johansson
- Department of Biological and Environmental Sciences, University of Gothenburg, Box 461, SE-405 30 Göteborg, Sweden
| | - Mats Hamberg
- Division of Chemistry II, Department of Medical Biochemistry and Biophysics, Karolinska Institutet, SE-17 177 Stockholm, Sweden
| | - Mats X Andersson
- Department of Biological and Environmental Sciences, University of Gothenburg, Box 461, SE-405 30 Göteborg, Sweden
| | - Mats Ellerström
- Department of Biological and Environmental Sciences, University of Gothenburg, Box 461, SE-405 30 Göteborg, Sweden
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24
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Kelly AA, Feussner I. Oil is on the agenda: Lipid turnover in higher plants. Biochim Biophys Acta Mol Cell Biol Lipids 2016; 1861:1253-1268. [PMID: 27155216 DOI: 10.1016/j.bbalip.2016.04.021] [Citation(s) in RCA: 22] [Impact Index Per Article: 2.8] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 02/02/2016] [Revised: 04/23/2016] [Accepted: 04/25/2016] [Indexed: 12/13/2022]
Abstract
Lipases hydrolyze ester bonds within lipids. This process is called lipolysis. They are key players in lipid turnover and involved in numerous metabolic pathways, many of which are shared between organisms like the mobilization of neutral or storage lipids or lipase-mediated membrane lipid homeostasis. Some reactions though are predominantly present in certain organisms, such as the production of signaling molecules (endocannabinoids) by diacylglycerol (DAG) and monoacylglycerol (MAG) lipases in mammals and plants or the jasmonate production in flowering plants. This review aims at giving an overview of the different functional classes of lipases and respective well-known activities, with a focus on the most recent findings in plant biology for selected classes. Here we will put an emphasis on the physiological role and contribution of lipases to the turnover of neutral lipids found in seed oil and other vegetative tissue as candidates for increasing the economical values of crop plants. This article is part of a Special Issue entitled: Plant Lipid Biology edited by Kent D. Chapman and Ivo Feussner.
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Affiliation(s)
- Amélie A Kelly
- Georg-August-University, Albrecht-von-Haller-Institute for Plant Sciences, Justus-von-Liebig Weg 11, 37077 Göttingen, Germany
| | - Ivo Feussner
- Georg-August-University, Albrecht-von-Haller-Institute for Plant Sciences, Justus-von-Liebig Weg 11, 37077 Göttingen, Germany; Georg-August-University, Göttingen Center for Molecular Biosciences (GZMB), Justus-von-Liebig Weg 11, 37077 Göttingen, Germany; Georg-August-University, International Center for Advanced Studies of Energy Conversion (ICASEC), Justus-von-Liebig Weg 11, 37077 Göttingen, Germany
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