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Permann C, Holzinger A. Zygospore formation in Zygnematophyceae predates several land plant traits. Philos Trans R Soc Lond B Biol Sci 2024; 379:20230356. [PMID: 39343014 PMCID: PMC11449217 DOI: 10.1098/rstb.2023.0356] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Grants] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 03/05/2024] [Revised: 04/18/2024] [Accepted: 04/19/2024] [Indexed: 10/01/2024] Open
Abstract
Recent research on a special type of sexual reproduction and zygospore formation in Zygnematophyceae, the sister group of land plants, is summarized. Within this group, gamete fusion occurs by conjugation. Zygospore development in Mougeotia, Spirogyra and Zygnema is highlighted, which has recently been studied using Raman spectroscopy, allowing chemical imaging and detection of changes in starch and lipid accumulation. Three-dimensional reconstructions after serial block-face scanning electron microscopy (SBF-SEM) or focused ion beam SEM (FIB-SEM) made it possible to visualize and quantify cell wall and organelle changes during zygospore development. The zygospore walls undergo strong modifications starting from uniform thin cell walls to a multilayered structure. The mature cell wall is composed of a cellulosic endospore and exospore and a central mesospore built up by aromatic compounds. In Spirogyra, the exospore and endospore consist of thick layers of helicoidally arranged cellulose fibrils, which are otherwise only known from stone cells of land plants. While starch is degraded during maturation, providing building blocks for cell wall formation, lipid droplets accumulate and fill large parts of the ripe zygospores, similar to spores and seeds of land plants. Overall, data show similarities between streptophyte algae and embryophytes, suggesting that the genetic toolkit for many land plant traits already existed in their shared algal ancestor. This article is part of the theme issue 'The evolution of plant metabolism'.
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Affiliation(s)
- Charlotte Permann
- Department of Botany, University of Innsbruck, Sternwartestraße 15,6020 Innsbruck, Austria
| | - Andreas Holzinger
- Department of Botany, University of Innsbruck, Sternwartestraße 15,6020 Innsbruck, Austria
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2
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Li M, Zhang L, Jiang LL, Zhao ZB, Long YH, Chen DM, Bin J, Kang C, Liu YJ. Label-free Raman microspectroscopic imaging with chemometrics for cellular investigation of apple ring rot and nondestructive early recognition using near-infrared reflection spectroscopy with machine learning. Talanta 2024; 267:125212. [PMID: 37741265 DOI: 10.1016/j.talanta.2023.125212] [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] [Received: 07/07/2023] [Revised: 08/16/2023] [Accepted: 09/14/2023] [Indexed: 09/25/2023]
Abstract
Apple ring rot caused by Botryosphaeria dothidea can cause fruit decay during the growth and storage stages of apple fruit. Understanding the infection process and cellular defense response at the cellular micro-level holds immense importance in the field of prevention and control. Consequently, there is a pressing need to develop suitable chemical imaging analysis methods. Here we proposed a label-free, high-throughput imaging method for cellular investigation of apple fruit ring rot infected by Botryosphaeria dothidea, based on confocal Raman microspectroscopic imaging technology combined with multivariate curve resolution-alternating least squares algorithm (MCR-ALS). We conducted Raman measurements on every apple fruit and obtain an image cube. This cube was then unfolded into an augmented matrix in a column-wise manner. We proceeded with simultaneous MCR-ALS analysis, resolving the single-substance spectrum and concentration profile from the mixed signals. Lastly, the accurate and pure molecular imaging of low methoxyl pectin, high methoxyl pectin, cellulose, lignin, and phenols were realized by refolding the resolved concentration data to construct the composition image. Thereafter, we realized the study of the spatial-temporal changes distribution of the above substances in the cuticle and cell wall of green and red apples at different stages of infection. The imaging method proposed in this paper is expected to provide a chemical imaging strategy for studying pathogen infection process and fruit defense response at the cellular level. In addition, by utilizing a fiber-optic probe near-infrared reflection spectrometer in conjunction with machine learning, we developed a rapid and non-destructive classification method. This method allows for the timely identification of apples exhibiting early infection by Botryosphaeria dothidea. Notably, both principal component analysis-quadratic discriminant analysis and support vector machine achieved a classification accuracy of 100%.
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Affiliation(s)
- Mei Li
- School of Chemistry and Chemical Engineering, Guizhou University, Guiyang, 550025, China
| | - Lu Zhang
- Engineering and Technology Research Center of Kiwifruit, Guizhou University, Guiyang, 550025, China
| | - Ling-Li Jiang
- School of Chemistry and Chemical Engineering, Guizhou University, Guiyang, 550025, China
| | - Zhi-Bo Zhao
- Engineering and Technology Research Center of Kiwifruit, Guizhou University, Guiyang, 550025, China
| | - You-Hua Long
- Engineering and Technology Research Center of Kiwifruit, Guizhou University, Guiyang, 550025, China
| | - Dong-Mei Chen
- School of Chemistry and Chemical Engineering, Guizhou University, Guiyang, 550025, China
| | - Jun Bin
- School of Chemistry and Chemical Engineering, Guizhou University, Guiyang, 550025, China
| | - Chao Kang
- School of Chemistry and Chemical Engineering, Guizhou University, Guiyang, 550025, China.
| | - Ya-Juan Liu
- Key Laboratory of Molecular Target & Clinical Pharmacology, the NMPA & State Key Laboratory of Respiratory Disease, School of Pharmaceutical Sciences & the Fifth Affiliated Hospital, Guangzhou Medical University, Guangzhou, 511436, China.
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3
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Wang N, Wang X, Yan T, Xie H, Wang L, Ren F, Chen D, Zhang D, Zeng Q, Zhu S, Chen X. Label-free structural and functional volumetric imaging by dual-modality optical-Raman projection tomography. SCIENCE ADVANCES 2023; 9:eadf3504. [PMID: 36961894 PMCID: PMC10038343 DOI: 10.1126/sciadv.adf3504] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Abstract] [MESH Headings] [Grants] [Track Full Text] [Download PDF] [Figures] [Subscribe] [Scholar Register] [Received: 10/15/2022] [Accepted: 02/24/2023] [Indexed: 06/18/2023]
Abstract
Mesoscale volumetric imaging is of great importance for the study of bio-organisms. Among others, optical projection tomography provides unprecedented structural details of specimens, but it requires fluorescence label for chemical targeting. Raman spectroscopic imaging is able to identify chemical components in a label-free manner but lacks microstructure. Here, we present a dual-modality optical-Raman projection tomography (ORPT) technology, which enables label-free three-dimensional imaging of microstructures and components of millimeter-sized samples with a micron-level spatial resolution on the same device. We validate the feasibility of our ORPT system using images of polystyrene beads in a volume, followed by detecting biomolecules of zebrafish and Arabidopsis, demonstrating that fused three-dimensional images of the microstructure and molecular components of bio-samples could be achieved. Last, we observe the fat body of Drosophila melanogaster at different developmental stages. Our proposed technology enables bimodal label-free volumetric imaging of the structure and function of biomolecules in a large sample.
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Affiliation(s)
- Nan Wang
- Biomedical Photonics and Molecular Imaging Laboratory, School of Life Science and Technology, Xidian University, and Xi’an Key Laboratory of Intelligent Sensing and Regulation of Trans-Scale Life Information, Xi’an, Shaanxi 710126, China
- Engineering Research Center of Molecular and Neuro Imaging, Ministry of Education, Xi’an, Shaanxi 710126, China
| | - Xinyu Wang
- Biomedical Photonics and Molecular Imaging Laboratory, School of Life Science and Technology, Xidian University, and Xi’an Key Laboratory of Intelligent Sensing and Regulation of Trans-Scale Life Information, Xi’an, Shaanxi 710126, China
- Engineering Research Center of Molecular and Neuro Imaging, Ministry of Education, Xi’an, Shaanxi 710126, China
| | - Tianyu Yan
- Biomedical Photonics and Molecular Imaging Laboratory, School of Life Science and Technology, Xidian University, and Xi’an Key Laboratory of Intelligent Sensing and Regulation of Trans-Scale Life Information, Xi’an, Shaanxi 710126, China
- Engineering Research Center of Molecular and Neuro Imaging, Ministry of Education, Xi’an, Shaanxi 710126, China
| | - Hui Xie
- Biomedical Photonics and Molecular Imaging Laboratory, School of Life Science and Technology, Xidian University, and Xi’an Key Laboratory of Intelligent Sensing and Regulation of Trans-Scale Life Information, Xi’an, Shaanxi 710126, China
| | - Lin Wang
- School of Computer Science and Engineering, Xi’an University of Technology, Xi’an, Shaanxi 710048, China
| | - Feng Ren
- Biomedical Photonics and Molecular Imaging Laboratory, School of Life Science and Technology, Xidian University, and Xi’an Key Laboratory of Intelligent Sensing and Regulation of Trans-Scale Life Information, Xi’an, Shaanxi 710126, China
| | - Dan Chen
- Engineering Research Center of Molecular and Neuro Imaging, Ministry of Education, Xi’an, Shaanxi 710126, China
| | - Dongjie Zhang
- Biomedical Photonics and Molecular Imaging Laboratory, School of Life Science and Technology, Xidian University, and Xi’an Key Laboratory of Intelligent Sensing and Regulation of Trans-Scale Life Information, Xi’an, Shaanxi 710126, China
| | - Qi Zeng
- Biomedical Photonics and Molecular Imaging Laboratory, School of Life Science and Technology, Xidian University, and Xi’an Key Laboratory of Intelligent Sensing and Regulation of Trans-Scale Life Information, Xi’an, Shaanxi 710126, China
| | - Shouping Zhu
- Engineering Research Center of Molecular and Neuro Imaging, Ministry of Education, Xi’an, Shaanxi 710126, China
- International Joint Research Center for Advanced Medical Imaging and Intelligent Diagnosis and Treatment, School of Life Science and Technology, Xidian University, Xi’an, Shaanxi 710126, China
| | - Xueli Chen
- Biomedical Photonics and Molecular Imaging Laboratory, School of Life Science and Technology, Xidian University, and Xi’an Key Laboratory of Intelligent Sensing and Regulation of Trans-Scale Life Information, Xi’an, Shaanxi 710126, China
- Engineering Research Center of Molecular and Neuro Imaging, Ministry of Education, Xi’an, Shaanxi 710126, China
- International Joint Research Center for Advanced Medical Imaging and Intelligent Diagnosis and Treatment, School of Life Science and Technology, Xidian University, Xi’an, Shaanxi 710126, China
- Innovation Center for Advanced Medical Imaging and Intelligent Medicine, Guangzhou Institute of Technology, Xidian University, Guangzhou, Guangdong 51055, China
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4
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González Moreno A, Domínguez E, Mayer K, Xiao N, Bock P, Heredia A, Gierlinger N. 3D (x-y-t) Raman imaging of tomato fruit cuticle: Microchemistry during development. PLANT PHYSIOLOGY 2023; 191:219-232. [PMID: 35972400 PMCID: PMC9806558 DOI: 10.1093/plphys/kiac369] [Citation(s) in RCA: 6] [Impact Index Per Article: 6.0] [Reference Citation Analysis] [Abstract] [MESH Headings] [Grants] [Track Full Text] [Subscribe] [Scholar Register] [Received: 06/01/2022] [Accepted: 07/15/2022] [Indexed: 05/20/2023]
Abstract
The cuticle is a protective extracellular matrix that covers the above-ground epidermis of land plants. Here, we studied the cuticle of tomato (Solanum lycopersicum L.) fruits in situ using confocal Raman microscopy. Microsections from cuticles isolated at different developmental stages were scanned to visualize cuticle components with a spatial resolution of 342 nm by univariate and multivariate data analysis. Three main components, cutin, polysaccharides, and aromatics, were identified, with the latter exhibiting the strongest Raman scattering intensity. Phenolic acids and flavonoids were differentiated within the cuticle, and three schematic cuticle models were identified during development. Phenolic acids were found across the entire cuticle at the earliest stage of development, i.e. during the formation of the procuticle layer. Based on a mixture analysis with reference component spectra, the phenolic acids were identified as mainly esterified p-coumaric acid together with free p-hydroxybenzoic acid. During the cell expansion period of growth, phenolic acids accumulated in an outermost layer of the cuticle and in the middle region of the pegs. In these stages of development, cellulose and pectin were detected next to the inner cuticle region, close to the epidermal cell where flavonoid impregnation started during ripening. In the first ripening stage, chalconaringenin was observed, while methoxylated chalcones were chosen by the algorithm to fit the mature cuticle spectra. The colocation of carbohydrates, esterified p-coumaric acid, and methoxylated chalconaringenin suggests that the latter two link polysaccharide and cutin domains. Elucidating the different distribution of aromatics within the cuticle, suggests important functions: (1) overall impregnation conferring mechanical and thermal functions (2) the outermost phenolic acid layer displaying UV-B protection of the plant tissue.
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Affiliation(s)
| | - Eva Domínguez
- IHSM-UMA-CSIC La Mayora, Plant breeding and Biotechnology, CSIC, 29750 Algarrobo-Costa, Málaga, Spain
| | - Konrad Mayer
- Department of Nanobiotechnology, BOKU-University of Natural Resources and Life Science, Vienna, Muthgasse 11, 1190 Vienna, Austria
| | - Nannan Xiao
- Department of Nanobiotechnology, BOKU-University of Natural Resources and Life Science, Vienna, Muthgasse 11, 1190 Vienna, Austria
| | - Peter Bock
- Department of Nanobiotechnology, BOKU-University of Natural Resources and Life Science, Vienna, Muthgasse 11, 1190 Vienna, Austria
| | - Antonio Heredia
- IHSM-UMA-CSIC La Mayora, Departamento de Biología Molecular y Bioquímica, Universidad de Málaga, 29071, Málaga, Spain
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Reynoud N, Geneix N, Petit J, D’Orlando A, Fanuel M, Marion D, Rothan C, Lahaye M, Bakan B. The cutin polymer matrix undergoes a fine architectural tuning from early tomato fruit development to ripening. PLANT PHYSIOLOGY 2022; 190:1821-1840. [PMID: 36018278 PMCID: PMC9614491 DOI: 10.1093/plphys/kiac392] [Citation(s) in RCA: 2] [Impact Index Per Article: 1.0] [Reference Citation Analysis] [Abstract] [MESH Headings] [Grants] [Track Full Text] [Subscribe] [Scholar Register] [Received: 05/23/2022] [Accepted: 07/21/2022] [Indexed: 05/20/2023]
Abstract
The cuticle is a complex polymer matrix that protects all aerial organs of plants, fulfills multiple roles in plant-environment interactions, and is critical for plant development. These functions are associated with the structural features of cuticles, and the architectural modeling of cuticles during plant development is crucial for understanding their physical properties and biological functions. In this work, the in-depth architecture of the cutin polymer matrix during fruit development was investigated. Using cherry tomato fruit (Solanum lycopersicum) as a model from the beginning of the cell expansion phase to the red ripe stage, we designed an experimental scheme combining sample pretreatment, Raman mapping, multivariate data analyses, and biochemical analyses. These approaches revealed clear chemical areas with different contributions of cutin, polysaccharides, and phenolics within the cutin polymer matrix. Besides, we demonstrated that these areas are finely tuned during fruit development, including compositional and macromolecular rearrangements. The specific spatiotemporal accumulation of phenolic compounds (p-coumaric acid and flavonoids) suggests that they fulfill distinct functions during fruit development. In addition, we highlighted an unexpected dynamic remodeling of the cutin-embedded polysaccharides pectin, cellulose, and hemicellulose. Such structural tuning enables consistent adaption of the cutin-polysaccharide continuum and the functional performance of the fruit cuticle at the different developmental stages. This study provides insights into the plant cuticle architecture and in particular into the organization of the epidermal cell wall-cuticle.
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Affiliation(s)
- Nicolas Reynoud
- INRAE, Unité Biopolymères, Interactions, Assemblages, BP71627 44316, Nantes Cedex3, France
| | - Nathalie Geneix
- INRAE, Unité Biopolymères, Interactions, Assemblages, BP71627 44316, Nantes Cedex3, France
| | - Johann Petit
- INRAE, Univ. Bordeaux, UMR BFP, F-33140, Villenave d’Ornon, France
| | - Angelina D’Orlando
- INRAE, Unité Biopolymères, Interactions, Assemblages, BP71627 44316, Nantes Cedex3, France
- INRAE PROBE research infrastructure, BIBS Facility, F- 44300, Nantes, France
| | - Mathieu Fanuel
- INRAE, Unité Biopolymères, Interactions, Assemblages, BP71627 44316, Nantes Cedex3, France
- INRAE PROBE research infrastructure, BIBS Facility, F- 44300, Nantes, France
| | - Didier Marion
- INRAE, Unité Biopolymères, Interactions, Assemblages, BP71627 44316, Nantes Cedex3, France
| | | | - Marc Lahaye
- INRAE, Unité Biopolymères, Interactions, Assemblages, BP71627 44316, Nantes Cedex3, France
| | - Bénédicte Bakan
- INRAE, Unité Biopolymères, Interactions, Assemblages, BP71627 44316, Nantes Cedex3, France
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6
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Blervacq AS, Moreau M, Duputié A, De Waele I, Duponchel L, Hawkins S. Raman spectroscopy mapping of changes in the organization and relative quantities of cell wall polymers in bast fiber cell walls of flax plants exposed to gravitropic stress. FRONTIERS IN PLANT SCIENCE 2022; 13:976351. [PMID: 36072316 PMCID: PMC9442035 DOI: 10.3389/fpls.2022.976351] [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: 06/23/2022] [Accepted: 08/01/2022] [Indexed: 06/15/2023]
Abstract
Flax is an important fiber crop that is subject to lodging. In order to gain more information about the potential role of the bast fiber cell wall in the return to the vertical position, 6-week-old flax plants were subjected to a long-term (6 week) gravitropic stress by stem tilting in an experimental set-up that excluded autotropism. Stress induced significant morphometric changes (lumen surface, lumen diameter, and cell wall thickness and lumen surface/total fiber surface ratio) in pulling- and opposite-side fibers compared to control fibers. Changes in the relative amounts and spatial distribution of cell wall polymers in flax bast fibers were determined by Raman vibrational spectroscopy. Following spectra acquisition, datasets (control, pulling- and opposite sides) were analyzed by principal component analysis, PC score imaging, and Raman chemical cartography of significant chemical bonds. Our results show that gravitropic stress induces discrete but significant changes in the composition and/or spatial organization of cellulose, hemicelluloses and lignin within the cell walls of both pulling side and opposite side fibers.
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Affiliation(s)
- Anne-Sophie Blervacq
- Université de Lille, Sciences et Technologies, CNRS, UMR 8576 - UGSF - Unité de Glycobiologie Structurale et Fonctionnelle, Lille, France
| | - Myriam Moreau
- Université de Lille, Sciences et Technologies, CNRS, UMR 8516 - LASIRE - Laboratoire de Spectroscopie pour les Interactions, la Réactivité et l’Environnement, Plateforme FT-Raman, Lille, France
| | - Anne Duputié
- Université de Lille, Sciences et Technologies, CNRS, UMR 8198 - EEP - Evo-Eco-Paléo, Lille, France
| | - Isabelle De Waele
- Université de Lille, Sciences et Technologies, CNRS, UMR 8516 - LASIRE - Laboratoire de Spectroscopie pour les Interactions, la Réactivité et l’Environnement, Plateforme FT-Raman, Lille, France
| | - Ludovic Duponchel
- Université de Lille, Sciences et Technologies, CNRS, UMR 8516 - LASIRE – Laboratoire de Spectroscopie pour les Interactions, la Réactivité et l’Environnement, Lille, France
| | - Simon Hawkins
- Université de Lille, Sciences et Technologies, CNRS, UMR 8576 - UGSF - Unité de Glycobiologie Structurale et Fonctionnelle, Lille, France
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Raman Method in Identification of Species and Varieties, Assessment of Plant Maturity and Crop Quality—A Review. Molecules 2022; 27:molecules27144454. [PMID: 35889327 PMCID: PMC9322835 DOI: 10.3390/molecules27144454] [Citation(s) in RCA: 6] [Impact Index Per Article: 3.0] [Reference Citation Analysis] [Abstract] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 06/21/2022] [Revised: 07/08/2022] [Accepted: 07/11/2022] [Indexed: 02/05/2023] Open
Abstract
The present review covers reports discussing potential applications of the specificity of Raman techniques in the advancement of digital farming, in line with an assumption of yield maximisation with minimum environmental impact of agriculture. Raman is an optical spectroscopy method which can be used to perform immediate, label-free detection and quantification of key compounds without destroying the sample. The authors particularly focused on the reports discussing the use of Raman spectroscopy in monitoring the physiological status of plants, assessing crop maturity and quality, plant pathology and ripening, and identifying plant species and their varieties. In recent years, research reports have presented evidence confirming the effectiveness of Raman spectroscopy in identifying biotic and abiotic stresses in plants as well as in phenotyping and digital selection of plants in farming. Raman techniques used in precision agriculture can significantly improve capacities for farming management, crop quality assessment, as well as biological and chemical contaminant detection, thereby contributing to food safety as well as the productivity and profitability of agriculture. This review aims to increase the awareness of the growing potential of Raman spectroscopy in agriculture among plant breeders, geneticists, farmers and engineers.
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Kolašinac S, Pećinar I, Danojević D, Stevanović ZD. Raman spectroscopy coupled with chemometric modeling approaches for authentication of different paprika varieties at physiological maturity. Lebensm Wiss Technol 2022. [DOI: 10.1016/j.lwt.2022.113402] [Citation(s) in RCA: 1] [Impact Index Per Article: 0.5] [Reference Citation Analysis] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 10/18/2022]
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Pay ML, Kim DW, Somers DE, Kim JK, Foo M. Modelling of plant circadian clock for characterizing hypocotyl growth under different light quality conditions. IN SILICO PLANTS 2022; 4:diac001. [PMID: 35369361 PMCID: PMC8963510 DOI: 10.1093/insilicoplants/diac001] [Citation(s) in RCA: 1] [Impact Index Per Article: 0.5] [Reference Citation Analysis] [Abstract] [Key Words] [Grants] [Track Full Text] [Figures] [Subscribe] [Scholar Register] [Received: 09/30/2021] [Accepted: 01/13/2022] [Indexed: 06/14/2023]
Abstract
To meet the ever-increasing global food demand, the food production rate needs to be increased significantly in the near future. Speed breeding is considered as a promising agricultural technology solution to achieve the zero-hunger vision as specified in the United Nations Sustainable Development Goal 2. In speed breeding, the photoperiod of the artificial light has been manipulated to enhance crop productivity. In particular, regulating the photoperiod of different light qualities rather than solely white light can further improve speed breading. However, identifying the optimal light quality and the associated photoperiod simultaneously remains a challenging open problem due to complex interactions between multiple photoreceptors and proteins controlling plant growth. To tackle this, we develop a first comprehensive model describing the profound effect of multiple light qualities with different photoperiods on plant growth (i.e. hypocotyl growth). The model predicts that hypocotyls elongated more under red light compared to both red and blue light. Drawing similar findings from previous related studies, we propose that this might result from the competitive binding of red and blue light receptors, primarily Phytochrome B (phyB) and Cryptochrome 1 (cry1) for the core photomorphogenic regulator, CONSTITUTIVE PHOTOMORPHOGENIC 1 (COP1). This prediction is validated through an experimental study on Arabidopsis thaliana. Our work proposes a potential molecular mechanism underlying plant growth under different light qualities and ultimately suggests an optimal breeding protocol that takes into account light quality.
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Affiliation(s)
- Miao Lin Pay
- Institute for Future Transport and Cities, Coventry University, Coventry CV1 2TE, UK
| | - Dae Wook Kim
- Department of Mathematical Sciences, Korea Advanced Institute of Science and Technology, Daejeon 34141, Republic of Korea
- Biomedical Mathematics Group, Institute for Basic Science, Daejeon 34126, Republic of Korea
| | - David E Somers
- Department of Molecular Genetics, The Ohio State University, Columbus, OH 43210, USA
- Center for Applied Plant Sciences, The Ohio State University, Columbus, OH 43210, USA
| | - Jae Kyoung Kim
- Department of Mathematical Sciences, Korea Advanced Institute of Science and Technology, Daejeon 34141, Republic of Korea
- Biomedical Mathematics Group, Institute for Basic Science, Daejeon 34126, Republic of Korea
| | - Mathias Foo
- School of Engineering, University of Warwick, Coventry CV4 7AL, UK
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10
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Bilkey N, Li H, Borodinov N, Ievlev AV, Ovchinnikova OS, Dixit R, Foston M. Correlated mechanochemical maps of Arabidopsis thaliana primary cell walls using atomic force microscope infrared spectroscopy. QUANTITATIVE PLANT BIOLOGY 2022; 3:e31. [PMID: 37077971 PMCID: PMC10095902 DOI: 10.1017/qpb.2022.20] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Abstract] [Key Words] [Grants] [Track Full Text] [Figures] [Subscribe] [Scholar Register] [Received: 05/19/2022] [Revised: 09/11/2022] [Accepted: 10/07/2022] [Indexed: 05/03/2023]
Abstract
Spatial heterogeneity in composition and organisation of the primary cell wall affects the mechanics of cellular morphogenesis. However, directly correlating cell wall composition, organisation and mechanics has been challenging. To overcome this barrier, we applied atomic force microscopy coupled with infrared (AFM-IR) spectroscopy to generate spatially correlated maps of chemical and mechanical properties for paraformaldehyde-fixed, intact Arabidopsis thaliana epidermal cell walls. AFM-IR spectra were deconvoluted by non-negative matrix factorisation (NMF) into a linear combination of IR spectral factors representing sets of chemical groups comprising different cell wall components. This approach enables quantification of chemical composition from IR spectral signatures and visualisation of chemical heterogeneity at nanometer resolution. Cross-correlation analysis of the spatial distribution of NMFs and mechanical properties suggests that the carbohydrate composition of cell wall junctions correlates with increased local stiffness. Together, our work establishes new methodology to use AFM-IR for the mechanochemical analysis of intact plant primary cell walls.
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Affiliation(s)
- Natasha Bilkey
- Department of Biology, Center for Engineering Mechanobiology, Washington University in St. Louis, St. Louis, Missouri63130, USA
| | - Huiyong Li
- Department of Energy, Environmental and Chemical Engineering, Center for Engineering Mechanobiology, Washington University in St. Louis, St. Louis, Missouri63130, USA
| | - Nikolay Borodinov
- Center for Nanophase Materials Science, Oak Ridge National Laboratory, Oak Ridge, Tennessee37831, USA
| | - Anton V. Ievlev
- Center for Nanophase Materials Science, Oak Ridge National Laboratory, Oak Ridge, Tennessee37831, USA
| | - Olga S. Ovchinnikova
- Center for Nanophase Materials Science, Oak Ridge National Laboratory, Oak Ridge, Tennessee37831, USA
| | - Ram Dixit
- Department of Biology, Center for Engineering Mechanobiology, Washington University in St. Louis, St. Louis, Missouri63130, USA
| | - Marcus Foston
- Department of Energy, Environmental and Chemical Engineering, Center for Engineering Mechanobiology, Washington University in St. Louis, St. Louis, Missouri63130, USA
- Author for correspondence: M. Foston, E-mail:
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11
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Bock P, Felhofer M, Mayer K, Gierlinger N. A Guide to Elucidate the Hidden Multicomponent Layered Structure of Plant Cuticles by Raman Imaging. FRONTIERS IN PLANT SCIENCE 2021; 12:793330. [PMID: 34975980 PMCID: PMC8718554 DOI: 10.3389/fpls.2021.793330] [Citation(s) in RCA: 3] [Impact Index Per Article: 1.0] [Reference Citation Analysis] [Abstract] [Key Words] [Grants] [Track Full Text] [Subscribe] [Scholar Register] [Received: 10/12/2021] [Accepted: 11/09/2021] [Indexed: 05/29/2023]
Abstract
The cuticle covers almost all plant organs as the outermost layer and serves as a transpiration barrier, sunscreen, and first line of defense against pathogens. Waxes, fatty acids, and aromatic components build chemically and structurally diverse layers with different functionality. So far, electron microscopy has elucidated structure, while isolation, extraction, and analysis procedures have revealed chemistry. With this method paper, we close the missing link by demonstrating how Raman microscopy gives detailed information about chemistry and structure of the native cuticle on the microscale. We introduce an optimized experimental workflow, covering the whole process of sample preparation, Raman imaging experiment, data analysis, and interpretation and show the versatility of the approach on cuticles of a spruce needle, a tomato peel, and an Arabidopsis stem. We include laser polarization experiments to deduce the orientation of molecules and multivariate data analysis to separate cuticle layers and verify their molecular composition. Based on the three investigated cuticles, we discuss the chemical and structural diversity and validate our findings by comparing models based on our spectroscopic data with the current view of the cuticle. We amend the model by adding the distribution of cinnamic acids and flavonoids within the cuticle layers and their transition to the epidermal layer. Raman imaging proves as a non-destructive and fast approach to assess the chemical and structural variability in space and time. It might become a valuable tool to tackle knowledge gaps in plant cuticle research.
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Affiliation(s)
| | | | | | - Notburga Gierlinger
- Department of Nanobiotechnology, Institute of Biophysics, University of Natural Resources and Life Sciences, Vienna, Austria
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12
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Füchtner S, Piqueras S, Thygesen LG. Defensive strategies of Norway spruce and Kurile larch heartwood elucidated on the micron-level. Sci Rep 2021; 11:22235. [PMID: 34782641 PMCID: PMC8593066 DOI: 10.1038/s41598-021-01590-y] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Abstract] [Key Words] [Grants] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 07/15/2021] [Accepted: 10/28/2021] [Indexed: 11/08/2022] Open
Abstract
To decarbonize the building sector, the use of durable wood materials must be increased. Inspiration for environmentally benign wood protection systems is sought in durable tree species depositing phenolic extractives in their heartwood. Based on the hypothesis that the micro-distribution of extractives influences durability, we compared the natural impregnation patterns of non-durable, but readily available Norway spruce to more durable Kurile larch by mapping the distribution of heartwood extractives with Confocal Raman Imaging and multivariate data decomposition. Phenolics of both species were associated with hydrophobic oleoresin, likely facilitating diffusion through the tissue. They accumulated preferentially in lignin-rich sub-compartments of the cell wall. Yet, the distribution of extractives was found not to be the same. The middle lamellae contained flavonoids in larch and aromatic waxes in spruce, which was also found in rays and epithelial cells. Spruce-lignans were tentatively identified in all cell types, while larch-flavonoids were not present in resin channels, hinting at a different origin of synthesis. Larch-oleoresin without flavonoids was only found in lumina, indicating that the presence of phenolics in the mixture influences the final destination. Together our findings suggest, that spruce heartwood-defense focuses on water regulation, while the more efficient larch strategy is based on antioxidants.
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Affiliation(s)
- Sophie Füchtner
- Institute for Geoscience and Natural Resource Management, University of Copenhagen, Rolighedsvej 23, 1955, Frederiksberg, Denmark.
| | - Sara Piqueras
- Institute for Geoscience and Natural Resource Management, University of Copenhagen, Rolighedsvej 23, 1955, Frederiksberg, Denmark
- MS-OMICS, Bygstubben 9, 2950, Vedbæk, Denmark
| | - Lisbeth Garbrecht Thygesen
- Institute for Geoscience and Natural Resource Management, University of Copenhagen, Rolighedsvej 23, 1955, Frederiksberg, Denmark
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13
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Felhofer M, Mayr K, Lütz-Meindl U, Gierlinger N. Raman imaging of Micrasterias: new insights into shape formation. PROTOPLASMA 2021; 258:1323-1334. [PMID: 34292402 PMCID: PMC8523415 DOI: 10.1007/s00709-021-01685-3] [Citation(s) in RCA: 6] [Impact Index Per Article: 2.0] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Grants] [Track Full Text] [Figures] [Subscribe] [Scholar Register] [Received: 04/06/2021] [Accepted: 06/24/2021] [Indexed: 06/13/2023]
Abstract
The algae Micrasterias with its star-shaped cell pattern is a perfect unicellular model system to study morphogenesis. How the indentations are formed in the primary cell wall at exactly defined areas puzzled scientists for decades, and they searched for chemical differences in the primary wall of the extending tips compared to the resting indents. We now tackled the question by Raman imaging and scanned in situ Micrasterias cells at different stages of development. Thousands of Raman spectra were acquired from the mother cell and the developing semicell to calculate chemical images based on an algorithm finding the most different Raman spectra. Each of those spectra had characteristic Raman bands, which were assigned to molecular vibrations of BaSO4, proteins, lipids, starch, and plant cell wall carbohydrates. Visualizing the cell wall carbohydrates revealed a cell wall thickening at the indentations of the primary cell wall of the growing semicell and uniplanar orientation of the cellulose microfibrils to the cell surface in the secondary cell wall. Crystalline cellulose dominated in the secondary cell wall spectra, while in the primary cell wall spectra, also xyloglucan and pectin were reflected. Spectral differences between the indent and tip region of the primary cell wall were scarce, but a spectral mixing approach pointed to more cellulose fibrils deposited in the indent region. Therefore, we suggest that cell wall thickening together with a denser network of cellulose microfibrils stiffens the cell wall at the indent and induces different cell wall extensibility to shape the lobes.
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Affiliation(s)
- Martin Felhofer
- Department of Nanobiotechnology, University of Natural Resources and Life Sciences Vienna (BOKU), 1190, Vienna, Austria
| | - Konrad Mayr
- Department of Nanobiotechnology, University of Natural Resources and Life Sciences Vienna (BOKU), 1190, Vienna, Austria
| | - Ursula Lütz-Meindl
- Department of Biosciences, University of Salzburg, 5020, Salzburg, Austria
| | - Notburga Gierlinger
- Department of Nanobiotechnology, University of Natural Resources and Life Sciences Vienna (BOKU), 1190, Vienna, Austria.
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14
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Permann C, Herburger K, Niedermeier M, Felhofer M, Gierlinger N, Holzinger A. Cell wall characteristics during sexual reproduction of Mougeotia sp. (Zygnematophyceae) revealed by electron microscopy, glycan microarrays and RAMAN spectroscopy. PROTOPLASMA 2021; 258:1261-1275. [PMID: 33974144 PMCID: PMC8523461 DOI: 10.1007/s00709-021-01659-5] [Citation(s) in RCA: 19] [Impact Index Per Article: 6.3] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Grants] [Track Full Text] [Subscribe] [Scholar Register] [Received: 02/11/2021] [Accepted: 04/23/2021] [Indexed: 05/22/2023]
Abstract
Mougeotia spp. collected from field samples were investigated for their conjugation morphology by light-, fluorescence-, scanning- and transmission electron microscopy. During a scalarifom conjugation, the extragametangial zygospores were initially surrounded by a thin cell wall that developed into a multi-layered zygospore wall. Maturing zygospores turned dark brown and were filled with storage compounds such as lipids and starch. While M. parvula had a smooth surface, M. disjuncta had a punctated surface structure and a prominent suture. The zygospore wall consisted of a polysaccharide rich endospore, followed by a thin layer with a lipid-like appaerance, a massive electron dense mesospore and a very thin exospore composed of polysaccharides. Glycan microarray analysis of zygospores of different developmental stages revealed the occurrence of pectins and hemicelluloses, mostly composed of homogalacturonan (HG), xyloglucans, xylans, arabino-galactan proteins and extensins. In situ localization by the probe OG7-13AF 488 labelled HG in young zygospore walls, vegetative filaments and most prominently in conjugation tubes and cross walls. Raman imaging showed the distribution of proteins, lipids, carbohydrates and aromatic components of the mature zygospore with a spatial resolution of ~ 250 nm. The carbohydrate nature of the endo- and exospore was confirmed and in-between an enrichment of lipids and aromatic components, probably algaenan or a sporopollenin-like material. Taken together, these results indicate that during zygospore formation, reorganizations of the cell walls occured, leading to a resistant and protective structure.
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Affiliation(s)
- Charlotte Permann
- Department of Botany, Functional Plant Biology, University of Innsbruck, 6020, Innsbruck, Austria
| | - Klaus Herburger
- Department of Plant and Environmental Sciences, Section for Plant Glycobiology, University of Copenhagen, 1871, Frederiksberg, Denmark
| | - Martin Niedermeier
- Department of Nanobiotechnology, University of Natural Resources and Life Sciences Vienna (BOKU), 1190, Vienna, Austria
- Department of Biomaterials, Max Planck Institute of Colloids and Interfaces, 14476, Potsdam, Germany
| | - Martin Felhofer
- Department of Nanobiotechnology, University of Natural Resources and Life Sciences Vienna (BOKU), 1190, Vienna, Austria
| | - Notburga Gierlinger
- Department of Nanobiotechnology, University of Natural Resources and Life Sciences Vienna (BOKU), 1190, Vienna, Austria
| | - Andreas Holzinger
- Department of Botany, Functional Plant Biology, University of Innsbruck, 6020, Innsbruck, Austria.
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15
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He Q, Yang J, Zabotina OA, Yu C. Surface-enhanced Raman spectroscopic chemical imaging reveals distribution of pectin and its co-localization with xyloglucan inside onion epidermal cell wall. PLoS One 2021; 16:e0250650. [PMID: 33951055 PMCID: PMC8099099 DOI: 10.1371/journal.pone.0250650] [Citation(s) in RCA: 1] [Impact Index Per Article: 0.3] [Reference Citation Analysis] [Abstract] [MESH Headings] [Grants] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 12/30/2020] [Accepted: 04/12/2021] [Indexed: 12/01/2022] Open
Abstract
The primary plant cell wall is a complex matrix composed of interconnected polysaccharides including cellulose, hemicellulose, and pectin. Changes of this dynamic polysaccharide system play a critical role during plant cell development and differentiation. A better understanding of cell wall architectures can provide insight into the plant cell development. In this study, a Raman spectroscopic imaging approach was developed to visualize the distribution of plant cell wall polysaccharides. In this approach, Surface-enhanced Raman scattering (SERS through self-assembled silver nanoparticles) was combined with Raman labels (4-Aminothiophenol. 4ATP) and targeted enzymatic hydrolysis to improve the sensitivity, specificity, and throughput of the Raman imaging technique, and to reveal the distribution of pectin and its co-localization with xyloglucan inside onion epidermal cell (OEC) wall. This technique significantly decreased the required spectral acquisition time. The resulted Raman spectra showed a high Raman signal. The resulted Raman images successfully revealed and characterized the pectin distribution and its co-localization pattern with xyloglucan in OEC wall.
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Affiliation(s)
- Qing He
- Department of Agricultural and Biosystems Engineering, Iowa State University, Ames, IA, United States of America
| | - Jingyi Yang
- Department of Agricultural and Biosystems Engineering, Iowa State University, Ames, IA, United States of America
| | - Olga A. Zabotina
- Department of Molecular Biology, Biochemistry and Biophysics, Iowa State University, Ames, IA, United States of America
| | - Chenxu Yu
- Department of Agricultural and Biosystems Engineering, Iowa State University, Ames, IA, United States of America
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Saletnik A, Saletnik B, Puchalski C. Overview of Popular Techniques of Raman Spectroscopy and Their Potential in the Study of Plant Tissues. Molecules 2021; 26:1537. [PMID: 33799702 PMCID: PMC7999012 DOI: 10.3390/molecules26061537] [Citation(s) in RCA: 31] [Impact Index Per Article: 10.3] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 02/17/2021] [Revised: 03/05/2021] [Accepted: 03/09/2021] [Indexed: 01/15/2023] Open
Abstract
Raman spectroscopy is one of the main analytical techniques used in optical metrology. It is a vibration, marker-free technique that provides insight into the structure and composition of tissues and cells at the molecular level. Raman spectroscopy is an outstanding material identification technique. It provides spatial information of vibrations from complex biological samples which renders it a very accurate tool for the analysis of highly complex plant tissues. Raman spectra can be used as a fingerprint tool for a very wide range of compounds. Raman spectroscopy enables all the polymers that build the cell walls of plants to be tracked simultaneously; it facilitates the analysis of both the molecular composition and the molecular structure of cell walls. Due to its high sensitivity to even minute structural changes, this method is used for comparative tests. The introduction of new and improved Raman techniques by scientists as well as the constant technological development of the apparatus has resulted in an increased importance of Raman spectroscopy in the discovery and defining of tissues and the processes taking place in them.
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Affiliation(s)
| | - Bogdan Saletnik
- Department of Bioenergetics, Food Analysis and Microbiology, Institute of Food Technology and Nutrition, College of Natural Sciences, University of Rzeszów, Ćwiklińskiej 2D, 35-601 Rzeszów, Poland; (A.S.); (C.P.)
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17
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Pećinar I, Krstić D, Caruso G, Popović-Djordjević JB. Rapid characterization of hypanthium and seed in wild and cultivated rosehip: application of Raman microscopy combined with multivariate analysis. ROYAL SOCIETY OPEN SCIENCE 2021; 8:202064. [PMID: 33959359 PMCID: PMC8074960 DOI: 10.1098/rsos.202064] [Citation(s) in RCA: 4] [Impact Index Per Article: 1.3] [Reference Citation Analysis] [Abstract] [Key Words] [Grants] [Track Full Text] [Subscribe] [Scholar Register] [Indexed: 05/11/2023]
Abstract
Rosehip (pseudo-fruit) of dog rose (Rosa canina L.) is highly valued, and owing to nutritional and sensory properties it has a significant place in the food industry. This work represents an innovative report focusing on the evaluation of the phytochemical composition of rosehips (hypanthium and seed) grown in different locations in Serbia, using Raman microspectroscopy combined with multivariate data analysis. Some significant differences arose between the analysed rosehip samples with regard to the chemical profile of both hypanthium parenchyma cells and seed, although no evident discrimination was recorded between the samples of wild and cultivated rosehip. The differences between the hypanthium samples compared were mainly determined by the content of carotenoids, phenolic compounds and polysaccharides, whereas phenolics, polysaccharides (pectin, cellulose and hemicellulose) and lipids (to a lower extent) contributed to the seed sample discrimination. The differences observed between the rosehip samples may be attributed to abiotic factors (growing, ripening and storage conditions), which had a significant impact on the carotenoid and polyphenols biosynthesis.
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Affiliation(s)
- Ilinka Pećinar
- Faculty of Agriculture, Department for Agrobotany, University of Belgrade, Nemanjina 6, 11080 Belgrade, Serbia
| | - Djurdja Krstić
- Faculty of Chemistry, University of Belgrade, Studentski trg 12-16, 11158 Belgrade, Serbia
| | - Gianluca Caruso
- Department of Agricultural Sciences, University of Naples Federico II, Portici (Naples), Italy
| | - Jelena B. Popović-Djordjević
- Faculty of Agriculture, Department for Chemistry and Biochemistry, University of Belgrade, Nemanjina 6, 11080 Belgrade, Serbia
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18
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Sasani N, Bock P, Felhofer M, Gierlinger N. Raman imaging reveals in-situ microchemistry of cuticle and epidermis of spruce needles. PLANT METHODS 2021; 17:17. [PMID: 33557869 PMCID: PMC7871409 DOI: 10.1186/s13007-021-00717-6] [Citation(s) in RCA: 19] [Impact Index Per Article: 6.3] [Reference Citation Analysis] [Abstract] [Key Words] [Grants] [Track Full Text] [Subscribe] [Scholar Register] [Received: 12/07/2020] [Accepted: 01/28/2021] [Indexed: 05/26/2023]
Abstract
BACKGROUND The cuticle is a protective layer playing an important role in plant defense against biotic and abiotic stresses. So far cuticle structure and chemistry was mainly studied by electron microscopy and chemical extraction. Thus, analysing composition involved sample destruction and the link between chemistry and microstructure remained unclear. In the last decade, Raman imaging showed high potential to link plant anatomical structure with microchemistry and to give insights into orientation of molecules. In this study, we use Raman imaging and polarization experiments to study the native cuticle and epidermal layer of needles of Norway spruce, one of the economically most important trees in Europe. The acquired hyperspectral dataset is the basis to image the chemical heterogeneity using univariate (band integration) as well as multivariate data analysis (cluster analysis and non-negative matrix factorization). RESULTS Confocal Raman microscopy probes the cuticle together with the underlying epidermis in the native state and tracks aromatics, lipids, carbohydrates and minerals with a spatial resolution of 300 nm. All three data analysis approaches distinguish a waxy, crystalline layer on top, in which aliphatic chains and coumaric acid are aligned perpendicular to the surface. Also in the lipidic amorphous cuticle beneath, strong signals of coumaric acid and flavonoids are detected. Even the unmixing algorithm results in mixed endmember spectra and confirms that lipids co-locate with aromatics. The underlying epidermal cell walls are devoid of lipids but show strong aromatic Raman bands. Especially the upper periclinal thicker cell wall is impregnated with aromatics. At the interface between epidermis and cuticle Calcium oxalate crystals are detected in a layer-like fashion. Non-negative matrix factorization gives the purest component spectra, thus the best match with reference spectra and by this promotes band assignments and interpretation of the visualized chemical heterogeneity. CONCLUSIONS Results sharpen our view about the cuticle as the outermost layer of plants and highlight the aromatic impregnation throughout. In the future, developmental studies tracking lipid and aromatic pathways might give new insights into cuticle formation and comparative studies might deepen our understanding why some trees and their needle and leaf surfaces are more resistant to biotic and abiotic stresses than others.
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Affiliation(s)
- Nadia Sasani
- Department of Nanobiotechnology (DNBT), Institute for Biophysics, University of Natural Resources and Life Sciences (BOKU), Muthgasse 11-II, 1190, Vienna, Austria
| | - Peter Bock
- Department of Nanobiotechnology (DNBT), Institute for Biophysics, University of Natural Resources and Life Sciences (BOKU), Muthgasse 11-II, 1190, Vienna, Austria
| | - Martin Felhofer
- Department of Nanobiotechnology (DNBT), Institute for Biophysics, University of Natural Resources and Life Sciences (BOKU), Muthgasse 11-II, 1190, Vienna, Austria
| | - Notburga Gierlinger
- Department of Nanobiotechnology (DNBT), Institute for Biophysics, University of Natural Resources and Life Sciences (BOKU), Muthgasse 11-II, 1190, Vienna, Austria.
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19
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Kahle EM, Zarnkow M, Jacob F. Beer Turbidity Part 2: A Review of Raman Spectroscopy and Possible Future Use for Beer Turbidity Analysis. JOURNAL OF THE AMERICAN SOCIETY OF BREWING CHEMISTS 2020. [DOI: 10.1080/03610470.2020.1800345] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Track Full Text] [Subscribe] [Scholar Register] [Indexed: 10/23/2022]
Affiliation(s)
- Eva-Maria Kahle
- Forschungszentrum Weihenstephan für Brau- und Lebensmittelqualität, Technische Universität München, Alte Akademie 3, 85354 Freising-Weihenstephan, Germany
| | - Martin Zarnkow
- Forschungszentrum Weihenstephan für Brau- und Lebensmittelqualität, Technische Universität München, Alte Akademie 3, 85354 Freising-Weihenstephan, Germany
| | - Fritz Jacob
- Forschungszentrum Weihenstephan für Brau- und Lebensmittelqualität, Technische Universität München, Alte Akademie 3, 85354 Freising-Weihenstephan, Germany
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20
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Abstract
Raman imaging is a microspectroscopic approach revealing the chemistry and structure of plant cell walls in situ on the micro- and nanoscale. The method is based on the Raman effect (inelastic scattering) that takes place when monochromatic laser light interacts with matter. The scattered light conveys a change in energy that is inherent of the involved molecule vibrations. The Raman spectra are thus characteristic for the chemical structure of the molecules and can be recorded spatially ordered with a lateral resolution of about 300 nm. Based on thousands of acquired Raman spectra, images can be assessed using univariate as well as multivariate data analysis approaches. One advantage compared to staining or labeling techniques is that not only one image is obtained as a result but different components and characteristics can be displayed in several images. Furthermore, as every pixel corresponds to a Raman spectrum, which is a kind of "molecular fingerprint," the imaging results should always be evaluated and further details revealed by analysis (e.g., band assignment) of extracted spectra. In this chapter, the basic theoretical background of the technique and instrumentation are described together with sample preparation requirements and tips for high-quality plant tissue sections and successful Raman measurements. Typical Raman spectra of the different plant cell wall components are shown as well as an exemplified analysis of Raman data acquired on the model plant Arabidopsis. Important preprocessing methods of the spectra are included as well as single component image generation (univariate) and spectral unmixing by means of multivariate approaches (e.g., vertex component analysis).
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Affiliation(s)
- Batirtze Prats Mateu
- Department of Nanobiotechnology, Institute of Biophysics, BOKU-University of Natural Resources and Life Sciences, Vienna, Austria
| | - Peter Bock
- Department of Nanobiotechnology, Institute of Biophysics, BOKU-University of Natural Resources and Life Sciences, Vienna, Austria
| | - Notburga Gierlinger
- Department of Nanobiotechnology, Institute of Biophysics, BOKU-University of Natural Resources and Life Sciences, Vienna, Austria.
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21
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Rybarczyk J, Khalenkow D, Kieckens E, Skirtach AG, Cox E, Vanrompay D. Lactoferrin translocates to the nucleus of bovine rectal epithelial cells in the presence of Escherichia coli O157:H7. Vet Res 2019; 50:75. [PMID: 31570109 PMCID: PMC6771091 DOI: 10.1186/s13567-019-0694-3] [Citation(s) in RCA: 6] [Impact Index Per Article: 1.2] [Reference Citation Analysis] [Abstract] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 05/01/2019] [Accepted: 08/22/2019] [Indexed: 01/12/2023] Open
Abstract
Enterohemorrhagic Escherichia coli (EHEC) O157:H7 is a foodborne pathogen which causes illness in humans. Ruminants are the main reservoirs and EHEC predominantly colonizes the epithelium of the recto-anal junction of cattle. Immunosuppression by EHEC promotes re-infection of cattle. However, bovine lactoferrin (bLF) apparently can overrule the immunosuppression by inducing EHEC-specific IgA responses at the mucosal site. The IgA responses are significantly correlated with reduced EHEC shedding and the absence of colonization at the rectal mucosa following re-infection. Therefore, to examine the interaction between bLF and bovine rectal epithelial cells, we first developed a method to establish a primary cell culture of epithelial cells of the rectum of cattle. Furthermore, we used LC–MS/MS to demonstrate the presence of secreted lactoferrin in bovine milk and the absence of a “delta” isoform which is known to translocate to the nucleus of cells. Nevertheless, lactoferrin derived from bovine milk was internalized by rectal epithelial cells and translocated to the nuclei. Moreover, nuclear translocation of bLF was significantly enhanced when the epithelial cells were inoculated with EHEC, as demonstrated by confocal fluorescence microscopy and confirmed by Raman microscopy and 3D imaging.
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Affiliation(s)
- Joanna Rybarczyk
- Department of Animal Sciences and Aquatic Ecology, Faculty of Bioscience Engineering, Ghent University, 9000, Ghent, Belgium.
| | - Dmitry Khalenkow
- Department of Molecular Biotechnology, Faculty of Bioscience Engineering, Ghent University, 9000, Ghent, Belgium
| | - Evelien Kieckens
- Department of Animal Sciences and Aquatic Ecology, Faculty of Bioscience Engineering, Ghent University, 9000, Ghent, Belgium
| | - Andre G Skirtach
- Department of Molecular Biotechnology, Faculty of Bioscience Engineering, Ghent University, 9000, Ghent, Belgium
| | - Eric Cox
- Laboratory of Immunology, Faculty of Veterinary Medicine, Ghent University, 9000, Ghent, Belgium
| | - Daisy Vanrompay
- Department of Animal Sciences and Aquatic Ecology, Faculty of Bioscience Engineering, Ghent University, 9000, Ghent, Belgium
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22
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Huss JC, Spaeker O, Gierlinger N, Merritt DJ, Miller BP, Neinhuis C, Fratzl P, Eder M. Temperature-induced self-sealing capability of Banksia follicles. J R Soc Interface 2019; 15:rsif.2018.0190. [PMID: 29925581 DOI: 10.1098/rsif.2018.0190] [Citation(s) in RCA: 8] [Impact Index Per Article: 1.6] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 03/17/2018] [Accepted: 05/18/2018] [Indexed: 11/12/2022] Open
Abstract
Many plants in fire-prone regions retain their seeds in woody fruits in the plant canopy until the passage of a fire causes the fruit to open and release the seeds. To enable this function, suitable tissues are required that effectively store and protect seeds until they are released. Here, we show that three different species of the Australian genus Banksia incorporate waxes at the interface of the two valves of the follicle enclosing the seeds, which melt between 45°C and 55°C. Since the melting temperature of the waxes is lower than the opening temperatures of the follicles in all investigated species (B. candolleana, B. serrata, B. attenuata), we propose that melting of these waxes allows the sealing of micro-fissures at the interface of the two valves while they are still closed. Such a self-sealing mechanism likely contributes to the structural integrity of the seed pods, and benefits seed viability and persistence during storage on the plants. Furthermore, we show in a simplified, bioinspired model system that temperature treatments seal artificially applied surface cuts and restore the barrier properties.
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Affiliation(s)
- Jessica C Huss
- Department of Biomaterials, Max Planck Institute of Colloids and Interfaces, Research Campus Golm, 14424 Potsdam, Germany
| | - Oliver Spaeker
- Department of Biomaterials, Max Planck Institute of Colloids and Interfaces, Research Campus Golm, 14424 Potsdam, Germany
| | - Notburga Gierlinger
- Department of Nanobiotechnology, Institute for Biophysics, BOKU - University of Natural Resources and Life Sciences, 1190 Vienna, Austria
| | - David J Merritt
- Kings Park Science, Department of Biodiversity Conservation and Attractions, Kings Park, WA 6005, Australia.,School of Biological Sciences, The University of Western Australia, Crawley, WA 6009, Australia
| | - Ben P Miller
- Kings Park Science, Department of Biodiversity Conservation and Attractions, Kings Park, WA 6005, Australia.,School of Biological Sciences, The University of Western Australia, Crawley, WA 6009, Australia
| | - Christoph Neinhuis
- Institute for Botany, Technische Universität Dresden, 01062 Dresden, Germany
| | - Peter Fratzl
- Department of Biomaterials, Max Planck Institute of Colloids and Interfaces, Research Campus Golm, 14424 Potsdam, Germany
| | - Michaela Eder
- Department of Biomaterials, Max Planck Institute of Colloids and Interfaces, Research Campus Golm, 14424 Potsdam, Germany
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23
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Lara I, Heredia A, Domínguez E. Shelf Life Potential and the Fruit Cuticle: The Unexpected Player. FRONTIERS IN PLANT SCIENCE 2019; 10:770. [PMID: 31244879 PMCID: PMC6581714 DOI: 10.3389/fpls.2019.00770] [Citation(s) in RCA: 70] [Impact Index Per Article: 14.0] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Subscribe] [Scholar Register] [Received: 03/19/2019] [Accepted: 05/28/2019] [Indexed: 05/18/2023]
Abstract
The plant cuticle is an extracellular barrier that protects the aerial, non-lignified parts of plants from the surrounding environment, and furthermore plays important functions in organ growth and development. The role of the cuticle in post-harvest quality of fruits is a topic currently driving a lot of interest since an increasing bulk of research data show its modulating influence on a number of important traits determining shelf life and storage potential, including water transpiration and fruit dehydration, susceptibility to rots, pests and disorders, and even firmness. Moreover, the properties of fruit cuticles keep evolving after harvest, and have also been shown to be highly responsive to the external conditions surrounding the fruit. Indeed, common post-harvest treatments will have an impact on cuticle integrity and performance that needs to be evaluated for a deeper understanding of changes in post-harvest quality. In this review, chemical and biophysical properties of fruit cuticles are summarized. An overview is also provided of post-harvest changes in cuticles and the effects thereupon of some post-harvest procedures, with the purpose of offering a comprehensive summary of currently available information. Identification of natural sources of variability in relevant quality traits would allow breeding for the improvement of post-harvest life of fruit commodities.
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Affiliation(s)
- Isabel Lara
- Unitat de Postcollita-XaRTA, AGROTÈCNIO, Departament de Química, Universitat de Lleida, Lleida, Spain
| | - Antonio Heredia
- IHSM La Mayora, Departamento de Biología Molecular y Bioquímica, Universidad de Málaga, Málaga, Spain
| | - Eva Domínguez
- IHSM La Mayora, Departamento de Mejora Genética y Biotecnología, Consejo Superior de Investigaciones Científicas, Málaga, Spain
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24
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Brennan M, McDonald A, Topp CFE. Use of Raman microspectroscopy to predict malting barley husk adhesion quality. PLANT PHYSIOLOGY AND BIOCHEMISTRY : PPB 2019; 139:587-590. [PMID: 31030026 DOI: 10.1016/j.plaphy.2019.04.024] [Citation(s) in RCA: 1] [Impact Index Per Article: 0.2] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Track Full Text] [Subscribe] [Scholar Register] [Received: 04/04/2019] [Revised: 04/17/2019] [Accepted: 04/17/2019] [Indexed: 06/09/2023]
Abstract
Good quality husk-caryopsis adhesion is essential for malting barley, but that quality is influenced by caryopsis surface lipid composition. Raman spectroscopy was applied to lipid extracts from barley caryopses of cultivars with differential adhesion qualities. Principal component regression indicated that Raman spectroscopy can distinguish among cultivars with good and poor quality adhesion due to differences in compounds associated with adhesion quality.
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Affiliation(s)
- Maree Brennan
- Scotland's Rural College, King's Buildings, West Mains Road, EH9 3JG, Edinburgh, United Kingdom; LERMAB, Faculté des Sciences et Technologies, Université de Lorraine, Nancy, France.
| | - Alison McDonald
- University of Edinburgh, King's Buildings, Edinburgh, United Kingdom
| | - Cairistiona F E Topp
- Scotland's Rural College, King's Buildings, West Mains Road, EH9 3JG, Edinburgh, United Kingdom
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25
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Effects of chemical treatments on the bioethanol yield and composition of Isoberlinia doka waste. SN APPLIED SCIENCES 2019. [DOI: 10.1007/s42452-019-0223-z] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 10/27/2022] Open
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26
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Dinant S, Wolff N, De Marco F, Vilaine F, Gissot L, Aubry E, Sandt C, Bellini C, Le Hir R. Synchrotron FTIR and Raman spectroscopy provide unique spectral fingerprints for Arabidopsis floral stem vascular tissues. JOURNAL OF EXPERIMENTAL BOTANY 2019; 70:871-884. [PMID: 30407539 DOI: 10.1093/jxb/ery396] [Citation(s) in RCA: 6] [Impact Index Per Article: 1.2] [Reference Citation Analysis] [Abstract] [MESH Headings] [Track Full Text] [Subscribe] [Scholar Register] [Received: 06/12/2018] [Accepted: 10/30/2018] [Indexed: 05/22/2023]
Abstract
Cell walls are highly complex structures that are modified during plant growth and development. For example, the development of phloem and xylem vascular cells, which participate in the transport of sugars and water as well as providing support, can be influenced by cell-specific wall composition. Here, we used synchrotron radiation-based Fourier-transform infrared (SR-FTIR) and Raman spectroscopy to analyse the cell wall composition of floral stem vascular tissues of wild-type Arabidopsis and the double-mutant sweet11-1 sweet12-1, which has impaired sugar transport. The SR-FTIR spectra showed that in addition to modified xylem cell wall composition, phloem cell walls in the double-mutant line were characterized by modified hemicellulose composition. Combining Raman spectroscopy with a classification and regression tree (CART) method identified combinations of Raman shifts that could distinguish xylem vessels and fibers. In addition, the disruption of the SWEET11 and SWEET12 genes impacted on xylem wall composition in a cell-specific manner, with changes in hemicelluloses and cellulose observed at the xylem vessel interface. These results suggest that the facilitated transport of sugars by transporters that exist between vascular parenchyma cells and conducting cells is important in ensuring correct phloem and xylem cell wall composition.
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Affiliation(s)
- S Dinant
- Institut Jean-Pierre Bourgin, INRA, AgroParisTech, CNRS, Université Paris-Saclay,Versailles, France
| | - N Wolff
- Institut Jean-Pierre Bourgin, INRA, AgroParisTech, CNRS, Université Paris-Saclay,Versailles, France
| | - F De Marco
- Institut Jean-Pierre Bourgin, INRA, AgroParisTech, CNRS, Université Paris-Saclay,Versailles, France
| | - F Vilaine
- Institut Jean-Pierre Bourgin, INRA, AgroParisTech, CNRS, Université Paris-Saclay,Versailles, France
| | - L Gissot
- Institut Jean-Pierre Bourgin, INRA, AgroParisTech, CNRS, Université Paris-Saclay,Versailles, France
| | - E Aubry
- Institut Jean-Pierre Bourgin, INRA, AgroParisTech, CNRS, Université Paris-Saclay,Versailles, France
| | - C Sandt
- Synchrotron SOLEIL, Ligne SMIS, L'Orme des Merisiers, Gif sur Yvette, France
| | - C Bellini
- Institut Jean-Pierre Bourgin, INRA, AgroParisTech, CNRS, Université Paris-Saclay,Versailles, France
- Umeå Plant Science Centre, Department of Plant Physiology, Umeå University, Umeå, Sweden
| | - R Le Hir
- Institut Jean-Pierre Bourgin, INRA, AgroParisTech, CNRS, Université Paris-Saclay,Versailles, France
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Zancajo VMR, Diehn S, Filiba N, Goobes G, Kneipp J, Elbaum R. Spectroscopic Discrimination of Sorghum Silica Phytoliths. FRONTIERS IN PLANT SCIENCE 2019; 10:1571. [PMID: 31921236 PMCID: PMC6917640 DOI: 10.3389/fpls.2019.01571] [Citation(s) in RCA: 3] [Impact Index Per Article: 0.6] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Subscribe] [Scholar Register] [Received: 04/17/2019] [Accepted: 11/11/2019] [Indexed: 05/09/2023]
Abstract
Grasses accumulate silicon in the form of silicic acid, which is precipitated as amorphous silica in microscopic particles termed phytoliths. These particles comprise a variety of morphologies according to the cell type in which the silica was deposited. Despite the evident morphological differences, phytolith chemistry has mostly been analysed in bulk samples, neglecting differences between the varied types formed in the same species. In this work, we extracted leaf phytoliths from mature plants of Sorghum bicolor (L.) Moench. Using solid state NMR and thermogravimetric analysis, we show that the extraction methods alter greatly the silica molecular structure, its condensation degree and the trapped organic matter. Measurements of individual phytoliths by Raman and synchrotron FTIR microspectroscopies in combination with multivariate analysis separated bilobate silica cells from prickles and long cells, based on the silica molecular structures and the fraction and composition of occluded organic matter. The variations in structure and composition of sorghum phytoliths suggest that the biological pathways leading to silica deposition vary between these cell types.
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Affiliation(s)
- Victor M. R. Zancajo
- School of Analytical Sciences Adlershof (SALSA), Humboldt-Universität zu Berlin, Berlin, Germany
- Chemistry Department, Humboldt-Universität zu Berlin, Berlin, Germany
- BAM Federal Institute for Materials Research and Testing, Berlin, Germany
- *Correspondence: Victor M. R. Zancajo, ; Janina Kneipp, ; Rivka Elbaum,
| | - Sabrina Diehn
- Chemistry Department, Humboldt-Universität zu Berlin, Berlin, Germany
| | - Nurit Filiba
- Department of Chemistry, Bar Ilan University, Ramat Gan, Israel
| | - Gil Goobes
- Department of Chemistry, Bar Ilan University, Ramat Gan, Israel
| | - Janina Kneipp
- School of Analytical Sciences Adlershof (SALSA), Humboldt-Universität zu Berlin, Berlin, Germany
- Chemistry Department, Humboldt-Universität zu Berlin, Berlin, Germany
- BAM Federal Institute for Materials Research and Testing, Berlin, Germany
- *Correspondence: Victor M. R. Zancajo, ; Janina Kneipp, ; Rivka Elbaum,
| | - Rivka Elbaum
- R. H. Smith Institute of Plant Sciences and Genetics in Agriculture, The Hebrew University of Jerusalem, Rehovot, Israel
- *Correspondence: Victor M. R. Zancajo, ; Janina Kneipp, ; Rivka Elbaum,
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Jin K, Liu X, Wang K, Jiang Z, Tian G, Yang S, Shang L, Ma J. Imaging the dynamic deposition of cell wall polymer in xylem and phloem in Populus × euramericana. PLANTA 2018; 248:849-858. [PMID: 29938358 DOI: 10.1007/s00425-018-2931-9] [Citation(s) in RCA: 16] [Impact Index Per Article: 2.7] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Track Full Text] [Subscribe] [Scholar Register] [Received: 03/11/2018] [Accepted: 05/29/2018] [Indexed: 05/13/2023]
Abstract
Both G units and S units deposited in the whole lignification process of xylem fiber. The topochemical variations in newly formed xylem and phloem of Populus × euramericana were investigated by combined microscopic techniques. During xylem formation, earlier cell wall deposition in vessel and afterwards in the neighboring fiber was observed in situ. Raman images in xylem fiber emphasized that cell wall deposition was an ordered process which lignification started in cell corner following carbohydrates deposition. Higher deposition speed of carbohydrates was revealed at the beginning of the cell wall differentiation, and the syringyl (S) units deposition was more pronounced compared with guaiacyl (G) units at the earlier stage of lignification. The comparative analysis of cell wall composition in phloem fiber indicated that phloem formed earlier than xylem and the distribution of lignin monomers varied significantly with phloem fiber location. Furthermore, an interesting phenomenon was found that the outermost phloem fiber near the periderm displayed a multilayered structure with alternating broad and narrow layer, and the broad lamellae showed higher concentration of carbohydrates and S lignin. The cytological information including cell wall composition and lignin structure of xylem and phloem might be helpful to understand the wood growth progresses and facilitate utilization of woody plants.
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Affiliation(s)
- Kexia Jin
- Key Lab of Bamboo and Rattan Science & Technology, International Center for Bamboo and Rattan, Beijing, 100102, China
| | - Xinge Liu
- Key Lab of Bamboo and Rattan Science & Technology, International Center for Bamboo and Rattan, Beijing, 100102, China
| | - Kun Wang
- Key Lab of Bamboo and Rattan Science & Technology, International Center for Bamboo and Rattan, Beijing, 100102, China
| | - Zehui Jiang
- Key Lab of Bamboo and Rattan Science & Technology, International Center for Bamboo and Rattan, Beijing, 100102, China
| | - Genlin Tian
- Key Lab of Bamboo and Rattan Science & Technology, International Center for Bamboo and Rattan, Beijing, 100102, China
| | - Shumin Yang
- Key Lab of Bamboo and Rattan Science & Technology, International Center for Bamboo and Rattan, Beijing, 100102, China
| | - Lili Shang
- Key Lab of Bamboo and Rattan Science & Technology, International Center for Bamboo and Rattan, Beijing, 100102, China
| | - Jianfeng Ma
- Key Lab of Bamboo and Rattan Science & Technology, International Center for Bamboo and Rattan, Beijing, 100102, China.
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Prats-Mateu B, Bock P, Schroffenegger M, Toca-Herrera JL, Gierlinger N. Following laser induced changes of plant phenylpropanoids by Raman microscopy. Sci Rep 2018; 8:11804. [PMID: 30087373 PMCID: PMC6081397 DOI: 10.1038/s41598-018-30096-3] [Citation(s) in RCA: 19] [Impact Index Per Article: 3.2] [Reference Citation Analysis] [Abstract] [MESH Headings] [Grants] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 03/08/2018] [Accepted: 07/24/2018] [Indexed: 12/26/2022] Open
Abstract
Raman microscopy is a powerful imaging technique for biological materials providing information about chemistry in context with microstructure. A 532 nm laser is often used as excitation source, because high spatial resolution and signal intensity can be achieved. The latter can be controlled by laser power and integration time, whereby high power and long times give good signal to noise ratio. However, most biological materials absorb in the VIS range and fluorescence masking the signal or even sample degradation might be hindering. Here, we show that on lignified plant cell walls even very short integration times and low laser powers induce a change in the ratio of the lignin bands at 1660 and 1600 cm-1. Time series on lignin model compounds revealed this change only in aromatic molecules with two OH-groups, such as coniferyl alcohol. Therefore, we conclude that monolignols are present in the cell wall and responsible for the observed effect. The solvent selectivity of the changes points to a laser induced polymerization process. The results emphasize how crucial careful adjustment of experimental parameters in Raman imaging of biological materials is and show the potential of time series and repeated imaging to get additional insights (e.g. monolignols).
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Affiliation(s)
- Batirtze Prats-Mateu
- Institute for Biophysics, Department of Nanobiotechnology, BOKU-University of Natural Resources and Life Sciences, Muthgasse 11/II, 1190, Vienna, Austria
| | - Peter Bock
- Institute for Biophysics, Department of Nanobiotechnology, BOKU-University of Natural Resources and Life Sciences, Muthgasse 11/II, 1190, Vienna, Austria
| | - Martina Schroffenegger
- Institute of Biologically inspired materials, Department of Nanobiotechnology, BOKU-University of Natural Resources and Life Sciences, Muthgasse 11/II, 1190, Vienna, Austria
| | - José Luis Toca-Herrera
- Institute for Biophysics, Department of Nanobiotechnology, BOKU-University of Natural Resources and Life Sciences, Muthgasse 11/II, 1190, Vienna, Austria
| | - Notburga Gierlinger
- Institute for Biophysics, Department of Nanobiotechnology, BOKU-University of Natural Resources and Life Sciences, Muthgasse 11/II, 1190, Vienna, Austria.
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Prats-Mateu B, Felhofer M, de Juan A, Gierlinger N. Multivariate unmixing approaches on Raman images of plant cell walls: new insights or overinterpretation of results? PLANT METHODS 2018; 14:52. [PMID: 29997681 PMCID: PMC6031114 DOI: 10.1186/s13007-018-0320-9] [Citation(s) in RCA: 16] [Impact Index Per Article: 2.7] [Reference Citation Analysis] [Abstract] [Key Words] [Grants] [Track Full Text] [Subscribe] [Scholar Register] [Received: 01/31/2018] [Accepted: 06/25/2018] [Indexed: 05/24/2023]
Abstract
BACKGROUND Plant cell walls are nanocomposites based on cellulose microfibrils embedded in a matrix of polysaccharides and aromatic polymers. They are optimized for different functions (e.g. mechanical stability) by changing cell form, cell wall thickness and composition. To reveal the composition of plant tissues in a non-destructive way on the microscale, Raman imaging has become an important tool. Thousands of Raman spectra are acquired, each one being a spatially resolved molecular fingerprint of the plant cell wall. Nevertheless, due to the multicomponent nature of plant cell walls, many bands are overlapping and classical band integration approaches often not suitable for imaging. Multivariate data analysing approaches have a high potential as the whole wavenumber region of all thousands of spectra is analysed at once. RESULTS Three multivariate unmixing algorithms, vertex component analysis, non-negative matrix factorization and multivariate curve resolution-alternating least squares were applied to find the purest components within datasets acquired from micro-sections of spruce wood and Arabidopsis. With all three approaches different cell wall layers (including tiny S1 and S3 with 0.09-0.14 µm thickness) and cell contents were distinguished and endmember spectra with a good signal to noise ratio extracted. Baseline correction influences the results obtained in all methods as well as the way in which algorithm extracts components, i.e. prioritizing the extraction of positive endmembers by sequential orthogonal projections in VCA or performing a simultaneous extraction of non-negative components aiming at explaining the maximum variance in NMF and MCR-ALS. Other constraints applied (e.g. closure in VCA) or a previous principal component analysis filtering step in MCR-ALS also contribute to the differences obtained. CONCLUSIONS VCA is recommended as a good preliminary approach, since it is fast, does not require setting many input parameters and the endmember spectra result in good approximations of the raw data. Yet the endmember spectra are more correlated and mixed than those retrieved by NMF and MCR-ALS methods. The latter two give the best model statistics (with lower lack of fit in the models), but care has to be taken about overestimating the rank as it can lead to artificial shapes due to peak splitting or inverted bands.
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Affiliation(s)
- Batirtze Prats-Mateu
- Department of Nanobiotechnology, BOKU-University of Natural Resources and Life Sciences, Muthgasse 11/II, 1190 Vienna, Austria
| | - Martin Felhofer
- Department of Nanobiotechnology, BOKU-University of Natural Resources and Life Sciences, Muthgasse 11/II, 1190 Vienna, Austria
| | - Anna de Juan
- Chemometrics Group, University of Barcelona, Diagonal 645, 08028 Barcelona, Spain
| | - Notburga Gierlinger
- Department of Nanobiotechnology, BOKU-University of Natural Resources and Life Sciences, Muthgasse 11/II, 1190 Vienna, Austria
- Institute for Building Materials, Eidgenössische Technische Hochschule Zurich Hönggerberg, 8093 Zurich, Switzerland
- Applied Wood Research Laboratory, Empa-Swiss Federal Laboratories for Material Testing and Research, Überlandstrasse 129, 8600 Dübendorf, Switzerland
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Zhu N, Wu D, Chen K. Label-free visualization of fruit lignification: Raman molecular imaging of loquat lignified cells. PLANT METHODS 2018; 14:58. [PMID: 30008794 PMCID: PMC6043974 DOI: 10.1186/s13007-018-0328-1] [Citation(s) in RCA: 21] [Impact Index Per Article: 3.5] [Reference Citation Analysis] [Abstract] [Key Words] [Grants] [Track Full Text] [Subscribe] [Scholar Register] [Received: 03/26/2018] [Accepted: 07/06/2018] [Indexed: 05/10/2023]
Abstract
BACKGROUND Flesh lignification, leading to increased fruit firmness, has been reported in several kinds of fruit. Understanding the mechanisms underlying fruit lignification is important to optimize the postharvest storage strategies and reduce the quality deterioration of postharvest fruit. Especially cellular level investigation of lignin deposition in fruits provides novel insight for deciphering the mechanisms underlying fruit lignification. The primary objective of this study was to establish a procedure of using Raman microspectroscopy technique to depict fruit lignification at the cell level. RESULTS Lignified cells, a special kind of cells contained high lignin content, were found abundantly scattered in red-fleshed 'Luoyangqing' loquat. Whereas these special lignified cells were barely detected in 'Baisha' loquat flesh. Dominant Raman bands of lignified cells were found primarily attributed to lignin (1664, 1628, 1603, 1467, and 1272 cm-1), cellulose (1383, 1124 and 1098 cm-1) and pectin (852 and 1740 cm-1). The band intensity correlation analysis indicated the peak at 1335 cm-1 assigned to either lignin or cellulose in previous works was related to lignin for the lignified cells. Multi-peaks Gaussian fitting successfully resolved the overlapped fingerprint peaks of lignin in 1550-1700 cm-1 into three independent peaks, which were assigned to different functional groups of lignin. Furthermore, the spatially resolved Raman images of lignified cells were generated, indicating that lignin and cellulose saturated the whole lignified cells, pectin mainly located in the cell corner, and the parenchyma cells contained little lignin. In addition, both phloroglucinol-HCl staining and autofluorescence analysis confirmed the results of lignin distribution of Raman microscopic analysis. CONCLUSIONS A procedure for the simultaneous visualization of the main components of the flesh cells without labeling by high-resolution Raman microspectroscopy has been established. With Raman microscopic imaging technique, we can add a microscopic level to cell compositions, essential for a detailed molecular understanding of loquat lignification. Such method can be further used to chemically monitor the textural changes during the ripening process or postharvest storage of other fruits and vegetables.
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Affiliation(s)
- Nan Zhu
- College of Agriculture and Biotechnology, Zhejiang Provincial Key Laboratory of Horticultural Plant Integrative Biology/The State Agriculture Ministry Laboratory of Horticultural Plant Growth/Development and Quality Improvement, Zhejiang University, Zijingang Campus, Hangzhou, 310058 People’s Republic of China
| | - Di Wu
- College of Agriculture and Biotechnology, Zhejiang Provincial Key Laboratory of Horticultural Plant Integrative Biology/The State Agriculture Ministry Laboratory of Horticultural Plant Growth/Development and Quality Improvement, Zhejiang University, Zijingang Campus, Hangzhou, 310058 People’s Republic of China
| | - Kunsong Chen
- College of Agriculture and Biotechnology, Zhejiang Provincial Key Laboratory of Horticultural Plant Integrative Biology/The State Agriculture Ministry Laboratory of Horticultural Plant Growth/Development and Quality Improvement, Zhejiang University, Zijingang Campus, Hangzhou, 310058 People’s Republic of China
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De Meester B, de Vries L, Özparpucu M, Gierlinger N, Corneillie S, Pallidis A, Goeminne G, Morreel K, De Bruyne M, De Rycke R, Vanholme R, Boerjan W. Vessel-Specific Reintroduction of CINNAMOYL-COA REDUCTASE1 (CCR1) in Dwarfed ccr1 Mutants Restores Vessel and Xylary Fiber Integrity and Increases Biomass. PLANT PHYSIOLOGY 2018; 176:611-633. [PMID: 29158331 PMCID: PMC5761799 DOI: 10.1104/pp.17.01462] [Citation(s) in RCA: 65] [Impact Index Per Article: 10.8] [Reference Citation Analysis] [Abstract] [MESH Headings] [Grants] [Track Full Text] [Subscribe] [Scholar Register] [Received: 10/06/2017] [Accepted: 11/14/2017] [Indexed: 05/19/2023]
Abstract
Lignocellulosic biomass is recalcitrant toward deconstruction into simple sugars due to the presence of lignin. To render lignocellulosic biomass a suitable feedstock for the bio-based economy, plants can be engineered to have decreased amounts of lignin. However, engineered plants with the lowest amounts of lignin exhibit collapsed vessels and yield penalties. Previous efforts were not able to fully overcome this phenotype without settling in sugar yield upon saccharification. Here, we reintroduced CINNAMOYL-COENZYME A REDUCTASE1 (CCR1) expression specifically in the protoxylem and metaxylem vessel cells of Arabidopsis (Arabidopsis thaliana) ccr1 mutants. The resulting ccr1 ProSNBE:CCR1 lines had overcome the vascular collapse and had a total stem biomass yield that was increased up to 59% as compared with the wild type. Raman analysis showed that monolignols synthesized in the vessels also contribute to the lignification of neighboring xylary fibers. The cell wall composition and metabolome of ccr1 ProSNBE:CCR1 still exhibited many similarities to those of ccr1 mutants, regardless of their yield increase. In contrast to a recent report, the yield penalty of ccr1 mutants was not caused by ferulic acid accumulation but was (largely) the consequence of collapsed vessels. Finally, ccr1 ProSNBE:CCR1 plants had a 4-fold increase in total sugar yield when compared with wild-type plants.
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Affiliation(s)
- Barbara De Meester
- Department of Plant Biotechnology and Bioinformatics, Ghent University, B-9052 Ghent, Belgium
- VIB Center for Plant Systems Biology, B-9052 Ghent, Belgium
| | - Lisanne de Vries
- Department of Plant Biotechnology and Bioinformatics, Ghent University, B-9052 Ghent, Belgium
- VIB Center for Plant Systems Biology, B-9052 Ghent, Belgium
| | - Merve Özparpucu
- Institute for Building Materials, Swiss Federal Institute of Technology Zürich, 8093 Zuerich, Switzerland
- Applied Wood Materials, Swiss Federal Laboratories of Materials Science and Technology, 8600 Duebendorf, Switzerland
| | - Notburga Gierlinger
- Institute for Biophysics, University of Natural Resources and Life Sciences Vienna, 1190 Vienna, Austria
| | - Sander Corneillie
- Department of Plant Biotechnology and Bioinformatics, Ghent University, B-9052 Ghent, Belgium
- VIB Center for Plant Systems Biology, B-9052 Ghent, Belgium
| | - Andreas Pallidis
- Department of Plant Biotechnology and Bioinformatics, Ghent University, B-9052 Ghent, Belgium
- VIB Center for Plant Systems Biology, B-9052 Ghent, Belgium
| | - Geert Goeminne
- Department of Plant Biotechnology and Bioinformatics, Ghent University, B-9052 Ghent, Belgium
- VIB Center for Plant Systems Biology, B-9052 Ghent, Belgium
- VIB Metabolomics Core, B-9052 Ghent, Belgium
| | - Kris Morreel
- Department of Plant Biotechnology and Bioinformatics, Ghent University, B-9052 Ghent, Belgium
- VIB Center for Plant Systems Biology, B-9052 Ghent, Belgium
- VIB Metabolomics Core, B-9052 Ghent, Belgium
| | - Michiel De Bruyne
- Department of Plant Biotechnology and Bioinformatics, Ghent University, B-9052 Ghent, Belgium
- VIB Center for Plant Systems Biology, B-9052 Ghent, Belgium
| | - Riet De Rycke
- Department of Plant Biotechnology and Bioinformatics, Ghent University, B-9052 Ghent, Belgium
- VIB Center for Plant Systems Biology, B-9052 Ghent, Belgium
| | - Ruben Vanholme
- Department of Plant Biotechnology and Bioinformatics, Ghent University, B-9052 Ghent, Belgium
- VIB Metabolomics Core, B-9052 Ghent, Belgium
| | - Wout Boerjan
- Department of Plant Biotechnology and Bioinformatics, Ghent University, B-9052 Ghent, Belgium
- VIB Center for Plant Systems Biology, B-9052 Ghent, Belgium
- VIB Metabolomics Core, B-9052 Ghent, Belgium
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Huss JC, Schoeppler V, Merritt DJ, Best C, Maire E, Adrien J, Spaeker O, Janssen N, Gladisch J, Gierlinger N, Miller BP, Fratzl P, Eder M. Climate-Dependent Heat-Triggered Opening Mechanism of Banksia Seed Pods. ADVANCED SCIENCE (WEINHEIM, BADEN-WURTTEMBERG, GERMANY) 2018; 5:1700572. [PMID: 29375977 PMCID: PMC5770687 DOI: 10.1002/advs.201700572] [Citation(s) in RCA: 12] [Impact Index Per Article: 2.0] [Reference Citation Analysis] [Abstract] [Key Words] [Grants] [Track Full Text] [Subscribe] [Scholar Register] [Received: 09/06/2017] [Revised: 11/03/2017] [Indexed: 05/22/2023]
Abstract
Heat-triggered fruit opening and delayed release of mature seeds are widespread among plants in fire-prone ecosystems. Here, the material characteristics of the seed-containing follicles of Banksia attenuata (Proteaceae), which open in response to heat frequently caused by fire, are investigated. Material analysis reveals that long-term dimensional stability and opening temperatures of follicles collected across an environmental gradient increase as habitats become drier, hotter, and more fire prone. A gradual increase in the biaxial curvature of the hygroscopic valves provides the follicles in the driest region with the highest flexural rigidity. The irreversible deformation of the valves for opening is enabled via a temperature-dependent reduction of the elastic modulus of the innermost tissue layer, which then allows releasing the stresses previously generated by shrinkage of the fiber bundles in the adjacent layer during follicle drying. These findings illustrate the level of sophistication by which this species optimizes its fruit opening mechanism over a large distribution range with varying environmental conditions, and may not only have great relevance for developing biomimetic actuators, but also for elucidating the species' capacity to cope with climatic changes.
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Affiliation(s)
- Jessica C. Huss
- Department of BiomaterialsMax‐Planck Institute of Colloids and InterfacesResearch Campus Golm14424PotsdamGermany
| | - Vanessa Schoeppler
- BCUBE‐Center for Molecular BioengineeringTechnische Universität DresdenDresden01307Germany
| | - David J. Merritt
- Kings Park and Botanic GardenKings ParkWA6005Australia
- School of Biological SciencesThe University of Western AustraliaCrawleyWA6009Australia
| | - Christine Best
- Kings Park and Botanic GardenKings ParkWA6005Australia
- School of Biological SciencesThe University of Western AustraliaCrawleyWA6009Australia
| | - Eric Maire
- INSA‐LyonMATEISCNRS UMR5510University of LyonF‐69621VilleurbanneFrance
| | - Jérôme Adrien
- INSA‐LyonMATEISCNRS UMR5510University of LyonF‐69621VilleurbanneFrance
| | - Oliver Spaeker
- Department of BiomaterialsMax‐Planck Institute of Colloids and InterfacesResearch Campus Golm14424PotsdamGermany
| | - Nils Janssen
- Department of BiomaterialsMax‐Planck Institute of Colloids and InterfacesResearch Campus Golm14424PotsdamGermany
| | | | - Notburga Gierlinger
- Department of NanobiotechnologyUniversity of Natural Resources and Life Science (BOKU)Muthgasse 11/II1190ViennaAustria
| | - Ben P. Miller
- Kings Park and Botanic GardenKings ParkWA6005Australia
- School of Biological SciencesThe University of Western AustraliaCrawleyWA6009Australia
| | - Peter Fratzl
- Department of BiomaterialsMax‐Planck Institute of Colloids and InterfacesResearch Campus Golm14424PotsdamGermany
| | - Michaela Eder
- Department of BiomaterialsMax‐Planck Institute of Colloids and InterfacesResearch Campus Golm14424PotsdamGermany
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Soukup M, Martinka M, Bosnić D, Čaplovičová M, Elbaum R, Lux A. Formation of silica aggregates in sorghum root endodermis is predetermined by cell wall architecture and development. ANNALS OF BOTANY 2017; 120:739-753. [PMID: 28651339 PMCID: PMC5714252 DOI: 10.1093/aob/mcx060] [Citation(s) in RCA: 14] [Impact Index Per Article: 2.0] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Track Full Text] [Subscribe] [Scholar Register] [Received: 01/19/2017] [Revised: 03/13/2017] [Accepted: 04/14/2017] [Indexed: 05/18/2023]
Abstract
Background and Aims Deposition of silica in plant cell walls improves their mechanical properties and helps plants to withstand various stress conditions. Its mechanism is still not understood and silica-cell wall interactions are elusive. The objective of this study was to investigate the effect of silica deposition on the development and structure of sorghum root endodermis and to identify the cell wall components involved in silicification. Methods Sorghum bicolor seedlings were grown hydroponically with (Si+) or without (Si-) silicon supplementation. Primary roots were used to investigate the transcription of silicon transporters by quantitative RT-PCR. Silica aggregation was induced also under in vitro conditions in detached root segments. The development and architecture of endodermal cell walls were analysed by histochemistry, microscopy and Raman spectroscopy. Water retention capability was compared between silicified and non-silicified roots. Raman spectroscopy analyses of isolated silica aggregates were also carried out. Key Results Active uptake of silicic acid is provided at the root apex, where silicon transporters Lsi1 and Lsi2 are expressed. The locations of silica aggregation are established during the development of tertiary endodermal cell walls, even in the absence of silicon. Silica aggregation takes place in non-lignified spots in the endodermal cell walls, which progressively accumulate silicic acid, and its condensation initiates at arabinoxylan-ferulic acid complexes. Silicification does not support root water retention capability; however, it decreases root growth inhibition imposed by desiccation. Conclusion A model is proposed in which the formation of silica aggregates in sorghum roots is predetermined by a modified cell wall architecture and takes place as governed by endodermal development. The interaction with silica is provided by arabinoxylan-ferulic acid complexes and interferes with further deposition of lignin. Due to contrasting hydrophobicity, silicification and lignification do not represent functionally equivalent modifications of plant cell walls.
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Affiliation(s)
- Milan Soukup
- Department of Plant Physiology, Faculty of Natural Sciences, Comenius University in Bratislava, Ilkovicova 6, 84215 Bratislava, Slovak Republic
- The Robert H. Smith Institute of Plant Sciences and Genetics in Agriculture, The Hebrew University of Jerusalem, 76100 Rehovot, Israel
| | - Michal Martinka
- Department of Plant Physiology, Faculty of Natural Sciences, Comenius University in Bratislava, Ilkovicova 6, 84215 Bratislava, Slovak Republic
| | - Dragana Bosnić
- Institute of Molecular Genetics and Genetic Engineering, University of Belgrade, Vojvode Stepe 444a, 11010 Belgrade, Serbia
| | - Mária Čaplovičová
- Department of Geology of Mineral Deposits, Faculty of Natural Sciences, Comenius University in Bratislava, Ilkovicova 6, 842 15 Bratislava, Slovak Republic
| | - Rivka Elbaum
- The Robert H. Smith Institute of Plant Sciences and Genetics in Agriculture, The Hebrew University of Jerusalem, 76100 Rehovot, Israel
| | - Alexander Lux
- Department of Plant Physiology, Faculty of Natural Sciences, Comenius University in Bratislava, Ilkovicova 6, 84215 Bratislava, Slovak Republic
- Institute of Chemistry, Slovak Academy of Sciences, Dubravska cesta 9, 84538 Bratislava, Slovak Republic
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Gierlinger N. New insights into plant cell walls by vibrational microspectroscopy. APPLIED SPECTROSCOPY REVIEWS 2017; 53:517-551. [PMID: 30057488 PMCID: PMC6050719 DOI: 10.1080/05704928.2017.1363052] [Citation(s) in RCA: 60] [Impact Index Per Article: 8.6] [Reference Citation Analysis] [Abstract] [Key Words] [Grants] [Track Full Text] [Subscribe] [Scholar Register] [Indexed: 05/02/2023]
Abstract
Vibrational spectroscopy provides non-destructively the molecular fingerprint of plant cells in the native state. In combination with microscopy, the chemical composition can be followed in context with the microstructure, and due to the non-destructive application, in-situ studies of changes during, e.g., degradation or mechanical load are possible. The two complementary vibrational microspectroscopic approaches, Fourier-Transform Infrared (FT-IR) Microspectroscopy and Confocal Raman spectroscopy, are based on different physical principles and the resulting different drawbacks and advantages in plant applications are reviewed. Examples for FT-IR and Raman microscopy applications on plant cell walls, including imaging as well as in-situ studies, are shown to have high potential to get a deeper understanding of structure-function relationships as well as biological processes and technical treatments. Both probe numerous different molecular vibrations of all components at once and thus result in spectra with many overlapping bands, a challenge for assignment and interpretation. With the help of multivariate unmixing methods (e.g., vertex components analysis), the most pure components can be revealed and their distribution mapped, even tiny layers and structures (250 nm). Instrumental as well as data analysis progresses make both microspectroscopic methods more and more promising tools in plant cell wall research.
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Affiliation(s)
- Notburga Gierlinger
- Department of Nanobiotechnology, University of Natural Resources and Life Sciences, Vienna, Austria
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Liu J, Kim JI, Cusumano JC, Chapple C, Venugopalan N, Fischetti RF, Makowski L. The impact of alterations in lignin deposition on cellulose organization of the plant cell wall. BIOTECHNOLOGY FOR BIOFUELS 2016; 9:126. [PMID: 27330560 PMCID: PMC4912819 DOI: 10.1186/s13068-016-0540-z] [Citation(s) in RCA: 17] [Impact Index Per Article: 2.1] [Reference Citation Analysis] [Abstract] [Key Words] [Grants] [Track Full Text] [Subscribe] [Scholar Register] [Received: 03/04/2016] [Accepted: 06/02/2016] [Indexed: 05/04/2023]
Abstract
BACKGROUND Coordination of synthesis and assembly of the polymeric components of cell walls is essential for plant growth and development. Given the degree of co-mingling and cross-linking among cell wall components, cellulose organization must be dependent on the organization of other polymers such as lignin. Here we seek to identify aspects of that codependency by studying the structural organization of cellulose fibrils in stems from Arabidopsis plants harboring mutations in genes encoding enzymes involved in lignin biosynthesis. Plants containing high levels of G-lignin, S-lignin, H-lignin, aldehyde-rich lignin, and ferulic acid-containing lignin, along with plants with very low lignin content were grown and harvested and longitudinal sections of stem were prepared and dried. Scanning X-ray microdiffraction was carried out using a 5-micron beam that moved across the sections in 5-micron steps and complete diffraction patterns were collected at each raster point. Approximately, 16,000 diffraction patterns were analyzed to determine cellulose fibril orientation and order within the tissues making up the stems. RESULTS Several mutations-most notably those exhibiting (1) down-regulation of cinnamoyl CoA reductase which leads to cell walls deficient in lignin and (2) defect of cinnamic acid 4-hydroxylase which greatly reduces lignin content-exhibited significant decrease in the proportion of oriented cellulose fibrils in the cell wall. Distinctions between tissues were maintained in all variants and even in plants exhibiting dramatic changes in cellulosic order the trends between tissues (where apparent) were generally maintained. The resilience of cellulose to degradative processes was investigated by carrying out the same analysis on samples stored in water for 30 days prior to data collection. This treatment led to significant loss of cellulosic order in plants rich in aldehyde or H-lignin, less change in wild type, and essentially no change in samples with high levels of G- or S-lignin. CONCLUSIONS These studies demonstrate that changes in lignin biosynthesis lead to significant disruption in the orientation and order of cellulose fibrils in all tissues of the stem. These dramatic phenotypic changes, in mutants with lignin rich in aldehyde or H-units, correlate with the impact the mutations have on the enzymatic degradation of the plant cell wall.
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Affiliation(s)
- Jiliang Liu
- />Department of Bioengineering, Northeastern University, 360 Huntington Ave, Boston, MA 02148 USA
| | - Jeong Im Kim
- />Department of Biochemistry, Purdue University, 175 South University Street, West Lafayette, IN 47907 USA
| | - Joanne C. Cusumano
- />Department of Biochemistry, Purdue University, 175 South University Street, West Lafayette, IN 47907 USA
| | - Clint Chapple
- />Department of Biochemistry, Purdue University, 175 South University Street, West Lafayette, IN 47907 USA
| | - Nagarajan Venugopalan
- />GM/CA CAT, XSD, Advanced Photon Source, Argonne National Laboratory, 9700 Cass Ave, Lemont, IL 60439 USA
| | - Robert F. Fischetti
- />GM/CA CAT, XSD, Advanced Photon Source, Argonne National Laboratory, 9700 Cass Ave, Lemont, IL 60439 USA
| | - Lee Makowski
- />Department of Bioengineering, Northeastern University, 360 Huntington Ave, Boston, MA 02148 USA
- />Department of Chemistry and Chemical Biology, Northeastern University, 360 Huntington Ave, Boston, MA 02148 USA
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