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Khambatta K, Hollings A, Sauzier G, Sanglard LMVP, Klein AR, Tobin MJ, Vongsvivut J, Gibberd MR, Payne AD, Naim F, Hackett MJ. "Wax On, Wax Off": In Vivo Imaging of Plant Physiology and Disease with Fourier Transform Infrared Reflectance Microspectroscopy. ADVANCED SCIENCE (WEINHEIM, BADEN-WURTTEMBERG, GERMANY) 2021; 8:e2101902. [PMID: 34338438 PMCID: PMC8498906 DOI: 10.1002/advs.202101902] [Citation(s) in RCA: 0] [Impact Index Per Article: 0] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Grants] [Track Full Text] [Figures] [Subscribe] [Scholar Register] [Received: 05/07/2021] [Revised: 06/25/2021] [Indexed: 06/13/2023]
Abstract
Analysis of the epicuticular wax layer on the surface of plant leaves can provide a unique window into plant physiology and responses to environmental stimuli. Well-established analytical methodologies can quantify epicuticular wax composition, yet few methods are capable of imaging wax distribution in situ or in vivo. Here, the first report of Fourier transform infrared (FTIR) reflectance spectroscopic imaging as a non-destructive, in situ, method to investigate variation in epicuticular wax distribution at 25 µm spatial resolution is presented. The authors demonstrate in vivo imaging of alterations in epicuticular waxes during leaf development and in situ imaging during plant disease or exposure to environmental stressors. It is envisaged that this new analytical capability will enable in vivo studies of plants to provide insights into how the physiology of plants and crops respond to environmental stresses such as disease, soil contamination, drought, soil acidity, and climate change.
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Affiliation(s)
- Karina Khambatta
- School of Molecular and Life SciencesCurtin UniversityBentleyWestern Australia6102Australia
| | - Ashley Hollings
- School of Molecular and Life SciencesCurtin UniversityBentleyWestern Australia6102Australia
| | - Georgina Sauzier
- School of Molecular and Life SciencesCurtin UniversityBentleyWestern Australia6102Australia
| | - Lilian M. V. P. Sanglard
- Centre for Crop and Disease ManagementSchool of Molecular and Life SciencesCurtin UniversityBentleyWestern Australia6102Australia
| | - Annaleise R. Klein
- Infrared Microspectroscopy (IRM) BeamlineANSTO – Australian Synchrotron800 Blackburn RoadClaytonVictoria3168Australia
| | - Mark J. Tobin
- Infrared Microspectroscopy (IRM) BeamlineANSTO – Australian Synchrotron800 Blackburn RoadClaytonVictoria3168Australia
| | - Jitraporn Vongsvivut
- Infrared Microspectroscopy (IRM) BeamlineANSTO – Australian Synchrotron800 Blackburn RoadClaytonVictoria3168Australia
| | - Mark R. Gibberd
- Centre for Crop and Disease ManagementSchool of Molecular and Life SciencesCurtin UniversityBentleyWestern Australia6102Australia
| | - Alan D. Payne
- School of Molecular and Life SciencesCurtin UniversityBentleyWestern Australia6102Australia
| | - Fatima Naim
- Centre for Crop and Disease ManagementSchool of Molecular and Life SciencesCurtin UniversityBentleyWestern Australia6102Australia
| | - Mark J. Hackett
- School of Molecular and Life SciencesCurtin UniversityBentleyWestern Australia6102Australia
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Chen M, Zhang Y, Kong X, Du Z, Zhou H, Yu Z, Qin J, Chen C. Leaf Cuticular Transpiration Barrier Organization in Tea Tree Under Normal Growth Conditions. FRONTIERS IN PLANT SCIENCE 2021; 12:655799. [PMID: 34276719 PMCID: PMC8278822 DOI: 10.3389/fpls.2021.655799] [Citation(s) in RCA: 4] [Impact Index Per Article: 1.3] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Subscribe] [Scholar Register] [Received: 01/19/2021] [Accepted: 06/07/2021] [Indexed: 06/01/2023]
Abstract
The cuticle plays a major role in restricting nonstomatal water transpiration in plants. There is therefore a long-standing interest to understand the structure and function of the plant cuticle. Although many efforts have been devoted, it remains controversial to what degree the various cuticular parameters contribute to the water transpiration barrier. In this study, eight tea germplasms were grown under normal conditions; cuticle thickness, wax coverage, and compositions were analyzed from the epicuticular waxes and the intracuticular waxes of both leaf surfaces. The cuticular transpiration rates were measured from the individual leaf surface as well as the intracuticular wax layer. Epicuticular wax resistances were also calculated from both leaf surfaces. The correlation analysis between the cuticular transpiration rates (or resistances) and various cuticle parameters was conducted. We found that the abaxial cuticular transpiration rates accounted for 64-78% of total cuticular transpiration and were the dominant factor in the variations for the total cuticular transpiration. On the adaxial surface, the major cuticular transpiration barrier was located on the intracuticular waxes; however, on the abaxial surface, the major cuticular transpiration barrier was located on the epicuticular waxes. Cuticle thickness was not a factor affecting cuticular transpiration. However, the abaxial epicuticular wax coverage was found to be significantly and positively correlated with the abaxial epicuticular resistance. Correlation analysis suggested that the very-long-chain aliphatic compounds and glycol esters play major roles in the cuticular transpiration barrier in tea trees grown under normal conditions. Our results provided novel insights about the complex structure-functional relationships in the tea cuticle.
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Affiliation(s)
- Mingjie Chen
- College of Life Sciences, Key Laboratory of Tea Biology of Henan Province, Xinyang Normal University, Xinyang, China
| | - Yi Zhang
- Tea Research Institute, Fujian Academy of Agricultural Sciences, Fuan, China
- Horticultural Plant Biology and Metabolomics Center, Haixia Institute of Science and Technology, Fujian Agriculture and Forestry University, Fuzhou, China
| | - Xiangrui Kong
- Tea Research Institute, Fujian Academy of Agricultural Sciences, Fuan, China
- The Fujian Research Branch of the National Tea Genetic Improvement Center, Fuzhou, China
| | - Zhenghua Du
- Horticultural Plant Biology and Metabolomics Center, Haixia Institute of Science and Technology, Fujian Agriculture and Forestry University, Fuzhou, China
| | - Huiwen Zhou
- College of Life Sciences, Key Laboratory of Tea Biology of Henan Province, Xinyang Normal University, Xinyang, China
| | - Zhaoxi Yu
- College of Life Sciences, Key Laboratory of Tea Biology of Henan Province, Xinyang Normal University, Xinyang, China
| | - Jianheng Qin
- College of Life Sciences, Key Laboratory of Tea Biology of Henan Province, Xinyang Normal University, Xinyang, China
| | - Changsong Chen
- Tea Research Institute, Fujian Academy of Agricultural Sciences, Fuan, China
- The Fujian Research Branch of the National Tea Genetic Improvement Center, Fuzhou, China
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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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4
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Matschi S, Vasquez MF, Bourgault R, Steinbach P, Chamness J, Kaczmar N, Gore MA, Molina I, Smith LG. Structure-function analysis of the maize bulliform cell cuticle and its potential role in dehydration and leaf rolling. PLANT DIRECT 2020; 4:e00282. [PMID: 33163853 PMCID: PMC7598327 DOI: 10.1002/pld3.282] [Citation(s) in RCA: 16] [Impact Index Per Article: 4.0] [Reference Citation Analysis] [Abstract] [Key Words] [Grants] [Track Full Text] [Subscribe] [Scholar Register] [Received: 06/08/2020] [Revised: 09/15/2020] [Accepted: 10/01/2020] [Indexed: 05/03/2023]
Abstract
The hydrophobic cuticle of plant shoots serves as an important interaction interface with the environment. It consists of the lipid polymer cutin, embedded with and covered by waxes, and provides protection against stresses including desiccation, UV radiation, and pathogen attack. Bulliform cells form in longitudinal strips on the adaxial leaf surface, and have been implicated in the leaf rolling response observed in drought-stressed grass leaves. In this study, we show that bulliform cells of the adult maize leaf epidermis have a specialized cuticle, and we investigate its function along with that of bulliform cells themselves. Bulliform cells displayed increased shrinkage compared to other epidermal cell types during dehydration of the leaf, providing a potential mechanism to facilitate leaf rolling. Analysis of natural variation was used to relate bulliform strip patterning to leaf rolling rate, providing further evidence of a role for bulliform cells in leaf rolling. Bulliform cell cuticles showed a distinct ultrastructure with increased cuticle thickness compared to other leaf epidermal cells. Comparisons of cuticular conductance between adaxial and abaxial leaf surfaces, and between bulliform-enriched mutants versus wild-type siblings, showed a correlation between elevated water loss rates and presence or increased density of bulliform cells, suggesting that bulliform cuticles are more water-permeable. Biochemical analysis revealed altered cutin composition and increased cutin monomer content in bulliform-enriched tissues. In particular, our findings suggest that an increase in 9,10-epoxy-18-hydroxyoctadecanoic acid content, and a lower proportion of ferulate, are characteristics of bulliform cuticles. We hypothesize that elevated water permeability of the bulliform cell cuticle contributes to the differential shrinkage of these cells during leaf dehydration, thereby facilitating the function of bulliform cells in stress-induced leaf rolling observed in grasses.
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Affiliation(s)
- Susanne Matschi
- Section of Cell and Developmental BiologyUniversity of California San DiegoLa JollaCAUSA
- Present address:
Department Biochemistry of Plant InteractionsLeibniz Institute of Plant BiochemistryWeinberg 3Halle (Saale)Germany
| | - Miguel F. Vasquez
- Section of Cell and Developmental BiologyUniversity of California San DiegoLa JollaCAUSA
| | | | - Paul Steinbach
- Howard Hughes Medical InstituteUniversity of California San DiegoLa JollaCAUSA
| | - James Chamness
- Plant Breeding and Genetics SectionSchool of Integrative Plant ScienceCornell UniversityIthacaNYUSA
- Present address:
Department of Genetics, Cell Biology, and DevelopmentUniversity of MinnesotaSaint PaulMN55108USA
| | - Nicholas Kaczmar
- Plant Breeding and Genetics SectionSchool of Integrative Plant ScienceCornell UniversityIthacaNYUSA
| | - Michael A. Gore
- Plant Breeding and Genetics SectionSchool of Integrative Plant ScienceCornell UniversityIthacaNYUSA
| | - Isabel Molina
- Department of BiologyAlgoma UniversitySault Ste. MarieONCanada
| | - Laurie G. Smith
- Section of Cell and Developmental BiologyUniversity of California San DiegoLa JollaCAUSA
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5
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Zhang Y, Du Z, Han Y, Chen X, Kong X, Sun W, Chen C, Chen M. Plasticity of the Cuticular Transpiration Barrier in Response to Water Shortage and Resupply in Camellia sinensis: A Role of Cuticular Waxes. FRONTIERS IN PLANT SCIENCE 2020; 11:600069. [PMID: 33505410 PMCID: PMC7829210 DOI: 10.3389/fpls.2020.600069] [Citation(s) in RCA: 2] [Impact Index Per Article: 0.5] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Subscribe] [Scholar Register] [Received: 09/21/2020] [Accepted: 11/26/2020] [Indexed: 05/08/2023]
Abstract
The cuticle is regarded as a non-living tissue; it remains unknown whether the cuticle could be reversibly modified and what are the potential mechanisms. In this study, three tea germplasms (Wuniuzao, 0202-10, and 0306A) were subjected to water deprivation followed by rehydration. The epicuticular waxes and intracuticular waxes from both leaf surfaces were quantified from the mature 5th leaf. Cuticular transpiration rates were then measured from leaf drying curves, and the correlations between cuticular transpiration rates and cuticular wax coverage were analyzed. We found that the cuticular transpiration barriers were reinforced by drought and reversed by rehydration treatment; the initial weak cuticular transpiration barriers were preferentially reinforced by drought stress, while the original major cuticular transpiration barriers were either strengthened or unaltered. Correlation analysis suggests that cuticle modifications could be realized by selective deposition of specific wax compounds into individual cuticular compartments through multiple mechanisms, including in vivo wax synthesis or transport, dynamic phase separation between epicuticular waxes and the intracuticular waxes, in vitro polymerization, and retro transportation into epidermal cell wall or protoplast for further transformation. Our data suggest that modifications of a limited set of specific wax components from individual cuticular compartments are sufficient to alter cuticular transpiration barrier properties.
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Affiliation(s)
- Yi Zhang
- Henan Key Laboratory of Tea Plant Biology, College of Life Sciences, Xinyang Normal University, Xinyang, China
- Horticultural Plant Biology and Metabolomics Center, Haixia Institute of Science and Technology, Fujian Agriculture and Forestry University, Fuzhou, China
| | - Zhenghua Du
- Horticultural Plant Biology and Metabolomics Center, Haixia Institute of Science and Technology, Fujian Agriculture and Forestry University, Fuzhou, China
| | - Yanting Han
- Henan Key Laboratory of Tea Plant Biology, College of Life Sciences, Xinyang Normal University, Xinyang, China
| | - Xiaobing Chen
- Horticultural Plant Biology and Metabolomics Center, Haixia Institute of Science and Technology, Fujian Agriculture and Forestry University, Fuzhou, China
| | - Xiangrui Kong
- Tea Research Institute, Fujian Academy of Agricultural Sciences, Fuan, China
| | - Weijiang Sun
- Anxi College of Tea Science, Fujian Agriculture and Forestry University, Fuzhou, China
| | - Changsong Chen
- Tea Research Institute, Fujian Academy of Agricultural Sciences, Fuan, China
| | - Mingjie Chen
- Henan Key Laboratory of Tea Plant Biology, College of Life Sciences, Xinyang Normal University, Xinyang, China
- *Correspondence: Mingjie Chen, ;
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6
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Effect of power ultrasound on quality of fresh-cut lettuce (cv. Vera) packaged in passive modified atmosphere. FOOD AND BIOPRODUCTS PROCESSING 2019. [DOI: 10.1016/j.fbp.2019.07.004] [Citation(s) in RCA: 14] [Impact Index Per Article: 2.8] [Reference Citation Analysis] [Track Full Text] [Subscribe] [Scholar Register] [Indexed: 11/17/2022]
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7
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Farber C, Wang R, Chemelewski R, Mullet J, Kurouski D. Nanoscale Structural Organization of Plant Epicuticular Wax Probed by Atomic Force Microscope Infrared Spectroscopy. Anal Chem 2019; 91:2472-2479. [PMID: 30624904 DOI: 10.1021/acs.analchem.8b05294] [Citation(s) in RCA: 30] [Impact Index Per Article: 6.0] [Reference Citation Analysis] [Abstract] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 12/24/2022]
Abstract
The cuticle covers external surfaces of plants, protecting them from biotic and abiotic stress factors. Epicuticular wax on the outer surface of the cuticle modifies reflectance and water loss from plant surfaces and has direct and indirect effects on photosynthesis. Variation in epicuticular wax accumulation, composition, and nanoscale structural organization impacts its biological function. Atomic force microscope infrared spectroscopy (AFM-IR) was utilized to investigate the internal and external surfaces of the cuticle of Sorghum bicolor, an important drought-tolerant cereal, forage, and high-biomass crop. AFM-IR revealed striking heterogeneity in chemical composition within and between the surfaces of the cuticle. The wax aggregate crystallinity and distribution of chemical functional groups across the surfaces was also probed and compared. These results, along with the noninvasive nondestructive nature of the method, suggest that AFM-IR can be used to investigate mechanisms of wax deposition and transport of charged molecules through the plant cuticle.
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8
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Zeisler-Diehl V, Müller Y, Schreiber L. Epicuticular wax on leaf cuticles does not establish the transpiration barrier, which is essentially formed by intracuticular wax. JOURNAL OF PLANT PHYSIOLOGY 2018; 227:66-74. [PMID: 29653782 DOI: 10.1016/j.jplph.2018.03.018] [Citation(s) in RCA: 22] [Impact Index Per Article: 3.7] [Reference Citation Analysis] [Abstract] [Key Words] [MESH Headings] [Track Full Text] [Subscribe] [Scholar Register] [Received: 01/16/2018] [Accepted: 03/30/2018] [Indexed: 05/23/2023]
Abstract
It is well established that waxes built up the barrier properties of cuticles, since their extraction in organic solvent e.g. chloroform increases diffusion of water and organic compounds by 1-2 orders of magnitude. Leaf surface waxes can be divided in epicuticular (on the surface of the cuticular membrane) and intracuticular (embedded in the cutin polymer) waxes. Until today there are only limited investigations dealing with the question to what extent epi- or intracuticular waxes contribute to the formation of the transpiration barrier. For Prunus laurocerasus previous studies have shown that epicuticular waxes do not contribute to the formation of the transpiration barrier. This approach successfully established for P. laurocerasus was applied to further species in order to check whether this finding also applies to a broader spectrum of species. Epicuticular wax was mechanically removed using collodion from the surface of either isolated cuticular membranes or intact leaf discs of ten further plant species differing in total wax amounts, wax compositions and transport properties. Scanning electron microscopy, which was performed to independently verify the successful removal of the surface waxes, indicated that two consecutive treatments with collodion were sufficient for a complete removal of epicuticular wax. The treated surfaces appeared smooth after removal. The total wax amounts removed with the two collodion treatments and the residual amount of waxes after collodion treatment were quantified by gas chromatography and mass spectrometry. This showed that epicuticular waxes essentially consisted of long-chain aliphatic molecules (e.g. alkanes, primary alcohols, fatty acids), whereas intracuticular wax was composed of both, triterpenoids and long-chain aliphatic molecules. Cuticular transpiration using combined replicates was measured before and after removal of surface wax. Results clearly indicated that two consecutive collodion treatments, or the corresponding solvent treatments (diethyl ether:ethanol) serving as control, did not increase cuticular transpiration of the ten further leaf species investigated. Our results lead to the conclusion that epicuticular wax does not contribute to the formation of the transpiration barrier of leaves.
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Affiliation(s)
- Viktoria Zeisler-Diehl
- Institute of Cellular and Molecular Botany, Department of Ecophysiology, University of Bonn, Kirschallee 1, D-53115, Bonn, Germany
| | - Yannic Müller
- Institute of Cellular and Molecular Botany, Department of Ecophysiology, University of Bonn, Kirschallee 1, D-53115, Bonn, Germany
| | - Lukas Schreiber
- Institute of Cellular and Molecular Botany, Department of Ecophysiology, University of Bonn, Kirschallee 1, D-53115, Bonn, Germany.
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9
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Burkhow SJ, Stephens NM, Mei Y, Dueñas ME, Freppon DJ, Ding G, Smith SC, Lee YJ, Nikolau BJ, Whitham SA, Smith EA. Characterizing virus-induced gene silencing at the cellular level with in situ multimodal imaging. PLANT METHODS 2018; 14:37. [PMID: 29849743 PMCID: PMC5968576 DOI: 10.1186/s13007-018-0306-7] [Citation(s) in RCA: 5] [Impact Index Per Article: 0.8] [Reference Citation Analysis] [Abstract] [Key Words] [Grants] [Track Full Text] [Subscribe] [Scholar Register] [Received: 01/05/2018] [Accepted: 05/12/2018] [Indexed: 05/02/2023]
Abstract
BACKGROUND Reverse genetic strategies, such as virus-induced gene silencing, are powerful techniques to study gene function. Currently, there are few tools to study the spatial dependence of the consequences of gene silencing at the cellular level. RESULTS We report the use of multimodal Raman and mass spectrometry imaging to study the cellular-level biochemical changes that occur from silencing the phytoene desaturase (pds) gene using a Foxtail mosaic virus (FoMV) vector in maize leaves. The multimodal imaging method allows the localized carotenoid distribution to be measured and reveals differences lost in the spatial average when analyzing a carotenoid extraction of the whole leaf. The nature of the Raman and mass spectrometry signals are complementary: silencing pds reduces the downstream carotenoid Raman signal and increases the phytoene mass spectrometry signal. CONCLUSIONS Both Raman and mass spectrometry imaging show that the biochemical changes from FoMV-pds silencing occur with a mosaic spatial pattern at the cellular level, and the Raman images show carotenoid expression was reduced at discrete locations but not eliminated. The data indicate the multimodal imaging method has great utility to study the biochemical changes that result from gene silencing at the cellular spatial level of expression in many plant tissues including the stem and leaf. Our demonstrated method is the first to spatially characterize the biochemical changes as a result of VIGS at the cellular level using commonly available instrumentation.
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Affiliation(s)
- Sadie J. Burkhow
- The Ames Laboratory, U.S. Department of Energy, Iowa State University, Ames, IA 50011-3111 USA
- Department of Chemistry, Iowa State University, Ames, IA 50011-3111 USA
| | - Nicole M. Stephens
- The Ames Laboratory, U.S. Department of Energy, Iowa State University, Ames, IA 50011-3111 USA
- Department of Chemistry, Iowa State University, Ames, IA 50011-3111 USA
| | - Yu Mei
- Department of Plant Pathology and Microbiology, Iowa State University, Ames, IA 50011 USA
| | - Maria Emilia Dueñas
- The Ames Laboratory, U.S. Department of Energy, Iowa State University, Ames, IA 50011-3111 USA
- Department of Chemistry, Iowa State University, Ames, IA 50011-3111 USA
| | - Daniel J. Freppon
- The Ames Laboratory, U.S. Department of Energy, Iowa State University, Ames, IA 50011-3111 USA
- Department of Chemistry, Iowa State University, Ames, IA 50011-3111 USA
| | - Geng Ding
- Department of Biochemistry Biophysics, and Molecular Biology, Center for Metabolic Biology, Iowa State University, Ames, IA 50011 USA
| | - Shea C. Smith
- Engineering Research Center for Biorenewable Chemicals, Iowa State University, Ames, IA 50011 USA
| | - Young-Jin Lee
- The Ames Laboratory, U.S. Department of Energy, Iowa State University, Ames, IA 50011-3111 USA
- Department of Chemistry, Iowa State University, Ames, IA 50011-3111 USA
| | - Basil J. Nikolau
- Department of Biochemistry Biophysics, and Molecular Biology, Center for Metabolic Biology, Iowa State University, Ames, IA 50011 USA
| | - Steven A. Whitham
- Department of Plant Pathology and Microbiology, Iowa State University, Ames, IA 50011 USA
| | - Emily A. Smith
- The Ames Laboratory, U.S. Department of Energy, Iowa State University, Ames, IA 50011-3111 USA
- Department of Chemistry, Iowa State University, Ames, IA 50011-3111 USA
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10
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Fricker MD, Moger J, Littlejohn GR, Deeks MJ. Making microscopy count: quantitative light microscopy of dynamic processes in living plants. J Microsc 2016; 263:181-91. [PMID: 27145353 DOI: 10.1111/jmi.12403] [Citation(s) in RCA: 4] [Impact Index Per Article: 0.5] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Received: 12/03/2015] [Revised: 01/31/2016] [Accepted: 02/16/2016] [Indexed: 12/18/2022]
Abstract
Cell theory has officially reached 350 years of age as the first use of the word 'cell' in a biological context can be traced to a description of plant material by Robert Hooke in his historic publication 'Micrographia: or some physiological definitions of minute bodies'. The 2015 Royal Microscopical Society Botanical Microscopy meeting was a celebration of the streams of investigation initiated by Hooke to understand at the subcellular scale how plant cell function and form arises. Much of the work presented, and Honorary Fellowships awarded, reflected the advanced application of bioimaging informatics to extract quantitative data from micrographs that reveal dynamic molecular processes driving cell growth and physiology. The field has progressed from collecting many pixels in multiple modes to associating these measurements with objects or features that are meaningful biologically. The additional complexity involves object identification that draws on a different type of expertise from computer science and statistics that is often impenetrable to biologists. There are many useful tools and approaches being developed, but we now need more interdisciplinary exchange to use them effectively. In this review we show how this quiet revolution has provided tools available to any personal computer user. We also discuss the oft-neglected issue of quantifying algorithm robustness and the exciting possibilities offered through the integration of physiological information generated by biosensors with object detection and tracking.
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Affiliation(s)
- Mark D Fricker
- Department of Plant Sciences, University of Oxford, Oxford, U.K
| | - Julian Moger
- Department of Physics, University of Exeter, Exeter, Devon, U.K
| | | | - Michael J Deeks
- Department of Biosciences, University of Exeter, Exeter, Devon, U.K
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11
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Prats Mateu B, Hauser MT, Heredia A, Gierlinger N. Waterproofing in Arabidopsis: Following Phenolics and Lipids In situ by Confocal Raman Microscopy. Front Chem 2016; 4:10. [PMID: 26973831 PMCID: PMC4770935 DOI: 10.3389/fchem.2016.00010] [Citation(s) in RCA: 36] [Impact Index Per Article: 4.5] [Reference Citation Analysis] [Abstract] [Key Words] [Grants] [Track Full Text] [Download PDF] [Figures] [Journal Information] [Subscribe] [Scholar Register] [Received: 09/30/2015] [Accepted: 02/11/2016] [Indexed: 12/28/2022] Open
Abstract
Waterproofing of the aerial organs of plants imposed a big evolutionary step during the colonization of the terrestrial environment. The main plant polymers responsible of water repelling are lipids and lignin, which play also important roles in the protection against biotic/abiotic stresses, regulation of flux of gases and solutes, and mechanical stability against negative pressure, among others. While the lipids, non-polymerized cuticular waxes together with the polymerized cutin, protect the outer surface, lignin is confined to the secondary cell wall within mechanical important tissues. In the present work a micro cross-section of the stem of Arabidopsis thaliana was used to track in situ the distribution of these non-carbohydrate polymers by Confocal Raman Microscopy. Raman hyperspectral imaging gives a molecular fingerprint of the native waterproofing tissues and cells with diffraction limited spatial resolution (~300 nm) at relatively high speed and without any tedious sample preparation. Lipids and lignified tissues as well as their effect on water content was directly visualized by integrating the 1299, 1600, and 3400 cm(-1) band, respectively. For detailed insights into compositional changes of these polymers vertex component analysis was performed on selected sample positions. Changes have been elucidated in the composition of lignin within the lignified tissues and between interfascicular fibers and xylem vessels. Hydrophobizing changes were revealed from the epidermal layer to the cuticle as well as a change in the aromatic composition within the cuticle of trichomes. To verify Raman signatures of different waterproofing polymers additionally Raman spectra of the cuticle and cutin monomer from tomato (Solanum lycopersicum) as well as aromatic model polymers (milled wood lignin and dehydrogenation polymer of coniferyl alcohol) and phenolic acids were acquired.
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Affiliation(s)
- Batirtze Prats Mateu
- Department of Material Sciences and Process Engineering, University of Natural Resources and Life SciencesVienna, Austria
| | - Marie Theres Hauser
- Department of Applied Genetics and Cell Biology, University of Natural Resources and Life SciencesVienna, Austria
| | - Antonio Heredia
- Department of Molecular Biology and Biochemistry, University of MalagaMalaga, Spain
| | - Notburga Gierlinger
- Department of Material Sciences and Process Engineering, University of Natural Resources and Life SciencesVienna, Austria
- Institute for Building Materials, Eidgenössische Technische Hochschule ZürichZürich, Switzerland
- Applied Wood Research Laboratory, Empa-Swiss Federal Laboratories for Material Testing and ResearchDübendorf, Switzerland
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12
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Littlejohn GR, Mansfield JC, Parker D, Lind R, Perfect S, Seymour M, Smirnoff N, Love J, Moger J. In vivo chemical and structural analysis of plant cuticular waxes using stimulated Raman scattering microscopy. PLANT PHYSIOLOGY 2015; 168:18-28. [PMID: 25783412 PMCID: PMC4424026 DOI: 10.1104/pp.15.00119] [Citation(s) in RCA: 21] [Impact Index Per Article: 2.3] [Reference Citation Analysis] [Abstract] [MESH Headings] [Grants] [Track Full Text] [Subscribe] [Scholar Register] [Received: 01/27/2015] [Accepted: 03/16/2015] [Indexed: 05/29/2023]
Abstract
The cuticle is a ubiquitous, predominantly waxy layer on the aerial parts of higher plants that fulfils a number of essential physiological roles, including regulating evapotranspiration, light reflection, and heat tolerance, control of development, and providing an essential barrier between the organism and environmental agents such as chemicals or some pathogens. The structure and composition of the cuticle are closely associated but are typically investigated separately using a combination of structural imaging and biochemical analysis of extracted waxes. Recently, techniques that combine stain-free imaging and biochemical analysis, including Fourier transform infrared spectroscopy microscopy and coherent anti-Stokes Raman spectroscopy microscopy, have been used to investigate the cuticle, but the detection sensitivity is severely limited by the background signals from plant pigments. We present a new method for label-free, in vivo structural and biochemical analysis of plant cuticles based on stimulated Raman scattering (SRS) microscopy. As a proof of principle, we used SRS microscopy to analyze the cuticles from a variety of plants at different times in development. We demonstrate that the SRS virtually eliminates the background interference compared with coherent anti-Stokes Raman spectroscopy imaging and results in label-free, chemically specific confocal images of cuticle architecture with simultaneous characterization of cuticle composition. This innovative use of the SRS spectroscopy may find applications in agrochemical research and development or in studies of wax deposition during leaf development and, as such, represents an important step in the study of higher plant cuticles.
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Affiliation(s)
- George R Littlejohn
- School of Biosciences, College of Life and Environmental Sciences (G.R.L., N.S., J.L.), and Department of Physics and Astronomy, College of Engineering, Mathematics, and Physical Sciences (J.C.M., J.M.), University of Exeter, Exeter, Devon EX4 4QD, United Kingdom;Biodomain Technology Group, Shell International Exploration and Production, Inc., Westhollow Technology Center, Houston, Texas 77082 (D.P.); andSyngenta, Jealott's Hill International Research Centre, Bracknell, Berkshire RG42 6EY, United Kingdom (R.L., S.P., M.S.)
| | - Jessica C Mansfield
- School of Biosciences, College of Life and Environmental Sciences (G.R.L., N.S., J.L.), and Department of Physics and Astronomy, College of Engineering, Mathematics, and Physical Sciences (J.C.M., J.M.), University of Exeter, Exeter, Devon EX4 4QD, United Kingdom;Biodomain Technology Group, Shell International Exploration and Production, Inc., Westhollow Technology Center, Houston, Texas 77082 (D.P.); andSyngenta, Jealott's Hill International Research Centre, Bracknell, Berkshire RG42 6EY, United Kingdom (R.L., S.P., M.S.)
| | - David Parker
- School of Biosciences, College of Life and Environmental Sciences (G.R.L., N.S., J.L.), and Department of Physics and Astronomy, College of Engineering, Mathematics, and Physical Sciences (J.C.M., J.M.), University of Exeter, Exeter, Devon EX4 4QD, United Kingdom;Biodomain Technology Group, Shell International Exploration and Production, Inc., Westhollow Technology Center, Houston, Texas 77082 (D.P.); andSyngenta, Jealott's Hill International Research Centre, Bracknell, Berkshire RG42 6EY, United Kingdom (R.L., S.P., M.S.)
| | - Rob Lind
- School of Biosciences, College of Life and Environmental Sciences (G.R.L., N.S., J.L.), and Department of Physics and Astronomy, College of Engineering, Mathematics, and Physical Sciences (J.C.M., J.M.), University of Exeter, Exeter, Devon EX4 4QD, United Kingdom;Biodomain Technology Group, Shell International Exploration and Production, Inc., Westhollow Technology Center, Houston, Texas 77082 (D.P.); andSyngenta, Jealott's Hill International Research Centre, Bracknell, Berkshire RG42 6EY, United Kingdom (R.L., S.P., M.S.)
| | - Sarah Perfect
- School of Biosciences, College of Life and Environmental Sciences (G.R.L., N.S., J.L.), and Department of Physics and Astronomy, College of Engineering, Mathematics, and Physical Sciences (J.C.M., J.M.), University of Exeter, Exeter, Devon EX4 4QD, United Kingdom;Biodomain Technology Group, Shell International Exploration and Production, Inc., Westhollow Technology Center, Houston, Texas 77082 (D.P.); andSyngenta, Jealott's Hill International Research Centre, Bracknell, Berkshire RG42 6EY, United Kingdom (R.L., S.P., M.S.)
| | - Mark Seymour
- School of Biosciences, College of Life and Environmental Sciences (G.R.L., N.S., J.L.), and Department of Physics and Astronomy, College of Engineering, Mathematics, and Physical Sciences (J.C.M., J.M.), University of Exeter, Exeter, Devon EX4 4QD, United Kingdom;Biodomain Technology Group, Shell International Exploration and Production, Inc., Westhollow Technology Center, Houston, Texas 77082 (D.P.); andSyngenta, Jealott's Hill International Research Centre, Bracknell, Berkshire RG42 6EY, United Kingdom (R.L., S.P., M.S.)
| | - Nicholas Smirnoff
- School of Biosciences, College of Life and Environmental Sciences (G.R.L., N.S., J.L.), and Department of Physics and Astronomy, College of Engineering, Mathematics, and Physical Sciences (J.C.M., J.M.), University of Exeter, Exeter, Devon EX4 4QD, United Kingdom;Biodomain Technology Group, Shell International Exploration and Production, Inc., Westhollow Technology Center, Houston, Texas 77082 (D.P.); andSyngenta, Jealott's Hill International Research Centre, Bracknell, Berkshire RG42 6EY, United Kingdom (R.L., S.P., M.S.)
| | - John Love
- School of Biosciences, College of Life and Environmental Sciences (G.R.L., N.S., J.L.), and Department of Physics and Astronomy, College of Engineering, Mathematics, and Physical Sciences (J.C.M., J.M.), University of Exeter, Exeter, Devon EX4 4QD, United Kingdom;Biodomain Technology Group, Shell International Exploration and Production, Inc., Westhollow Technology Center, Houston, Texas 77082 (D.P.); andSyngenta, Jealott's Hill International Research Centre, Bracknell, Berkshire RG42 6EY, United Kingdom (R.L., S.P., M.S.)
| | - Julian Moger
- School of Biosciences, College of Life and Environmental Sciences (G.R.L., N.S., J.L.), and Department of Physics and Astronomy, College of Engineering, Mathematics, and Physical Sciences (J.C.M., J.M.), University of Exeter, Exeter, Devon EX4 4QD, United Kingdom;Biodomain Technology Group, Shell International Exploration and Production, Inc., Westhollow Technology Center, Houston, Texas 77082 (D.P.); andSyngenta, Jealott's Hill International Research Centre, Bracknell, Berkshire RG42 6EY, United Kingdom (R.L., S.P., M.S.)
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13
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Heredia-Guerrero JA, Benítez JJ, Domínguez E, Bayer IS, Cingolani R, Athanassiou A, Heredia A. Infrared and Raman spectroscopic features of plant cuticles: a review. FRONTIERS IN PLANT SCIENCE 2014; 5:305. [PMID: 25009549 PMCID: PMC4069575 DOI: 10.3389/fpls.2014.00305] [Citation(s) in RCA: 160] [Impact Index Per Article: 16.0] [Reference Citation Analysis] [Abstract] [Key Words] [Track Full Text] [Subscribe] [Scholar Register] [Received: 04/30/2014] [Accepted: 06/09/2014] [Indexed: 05/04/2023]
Abstract
The cuticle is one of the most important plant barriers. It is an external and continuous lipid membrane that covers the surface of epidermal cells and whose main function is to prevent the massive loss of water. The spectroscopic characterization of the plant cuticle and its components (cutin, cutan, waxes, polysaccharides and phenolics) by infrared and Raman spectroscopies has provided significant advances in the knowledge of the functional groups present in the cuticular matrix and on their structural role, interaction and macromolecular arrangement. Additionally, these spectroscopies have been used in the study of cuticle interaction with exogenous molecules, degradation, distribution of components within the cuticle matrix, changes during growth and development and characterization of fossil plants.
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Affiliation(s)
- José A. Heredia-Guerrero
- Nanophysics, Istituto Italiano di TecnologiaGenova, Italy
- *Correspondence: José A. Heredia-Guerrero, Smart Materials Group, Nanophysics, Istituto Italiano di Tecnologia, Via Morego 30, Genova, 16163, Italy e-mail:
| | - José J. Benítez
- Instituto de Ciencias de Materiales de Sevilla, CSIC-USSeville, Spain
| | - Eva Domínguez
- Instituto de Hortofruticultura Subtropical y Mediterránea La Mayora, CSIC-UMAMálaga, Spain
| | - Ilker S. Bayer
- Nanophysics, Istituto Italiano di TecnologiaGenova, Italy
| | | | | | - Antonio Heredia
- Instituto de Hortofruticultura Subtropical y Mediterránea La Mayora, CSIC-UMAMálaga, Spain
- Departamento de Bioquímica y Biología Molecular, Facultad de Ciencias, Universidad de MálagaMálaga, Spain
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14
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Mansfield JC, Littlejohn GR, Seymour MP, Lind RJ, Perfect S, Moger J. Label-free Chemically Specific Imaging in Planta with Stimulated Raman Scattering Microscopy. Anal Chem 2013; 85:5055-63. [DOI: 10.1021/ac400266a] [Citation(s) in RCA: 62] [Impact Index Per Article: 5.6] [Reference Citation Analysis] [Track Full Text] [Journal Information] [Subscribe] [Scholar Register] [Indexed: 11/30/2022]
Affiliation(s)
| | | | - Mark P. Seymour
- Syngenta, Jealott’s Hill International Research Centre, Bracknell, Berkshire
RG42 6EY, United Kingdom
| | - Rob J. Lind
- Syngenta, Jealott’s Hill International Research Centre, Bracknell, Berkshire
RG42 6EY, United Kingdom
| | - Sarah Perfect
- Syngenta, Jealott’s Hill International Research Centre, Bracknell, Berkshire
RG42 6EY, United Kingdom
| | - Julian Moger
- School of
Physics, University of Exeter, Exeter EX4
4QL, United Kingdom
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15
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Krafft C, Cervellati C, Paetz C, Schneider B, Popp J. Distribution of amygdalin in apricot (Prunus armeniaca) seeds studied by Raman microscopic imaging. APPLIED SPECTROSCOPY 2012; 66:644-9. [PMID: 22732534 DOI: 10.1366/11-06521] [Citation(s) in RCA: 8] [Impact Index Per Article: 0.7] [Reference Citation Analysis] [Abstract] [Track Full Text] [Subscribe] [Scholar Register] [Indexed: 05/09/2023]
Abstract
Amygdalin is a cyanogenic glycoside found in the seeds of several plants belonging to the Rosaceae family. Cyanogenic glycosides can be specifically probed by Raman spectroscopy due to an inherent nitrile group which shows a well-resolved band near 2245 cm(-1). In the current study the subcellular distribution of amygdalin in thin apricot (Prunus armeniaca) seed sections is probed by high-resolution Raman imaging with a step size of 2.5 μm. Further, Raman images and line maps were collected from four apricot seeds with step sizes between 30 and 70 μm. The data were processed by functional group mapping and the spectral unmixing algorithm vertex component analysis. Spectral contributions of amygdalin, lipids, and cellulose were identified. One seed had low amygdalin content in its center and higher content toward its epidermis. The other three specimens showed different distributions of amygdalin, with highest concentration in the center and local concentration spots throughout the seed. We conclude from these preliminary results on Raman imaging in apricot seeds that amygdalin is unevenly distributed and its location does not follow the same pattern for all seeds. The observed biological variability of the amygdalin distribution cannot yet be explained satisfactorily and requires further investigation.
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16
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Medyukhina A, Vogler N, Latka I, Kemper S, Böhm M, Dietzek B, Popp J. Automated classification of healthy and keloidal collagen patterns based on processing of SHG images of human skin. JOURNAL OF BIOPHOTONICS 2011; 4:627-636. [PMID: 21595044 DOI: 10.1002/jbio.201100028] [Citation(s) in RCA: 5] [Impact Index Per Article: 0.4] [Reference Citation Analysis] [Abstract] [MESH Headings] [Track Full Text] [Subscribe] [Scholar Register] [Received: 04/06/2011] [Revised: 04/30/2011] [Accepted: 05/02/2011] [Indexed: 05/30/2023]
Abstract
All-optical microspectroscopic and tomographic tools have a great potential for the clinical investigation of human skin and skin diseases. However, automated optical tomography or even microscopy generate immense data sets. Therefore, in order to implement such diagnostic tools into the medical practice in both hospitals and private practice, there is a need for automated data handling and image analysis ideally implementing automized scores to judge the physiological state of a tissue section. In this contribution, the potential of an image processing algorithm for the automated classification of skin into normal or keloid based on second-harmonic generation (SHG) microscopic images is demonstrated. Such SHG data is routinely recorded within a multimodal imaging approach. The classification of the tissue implemented in the algorithm employs the geometrical features of collagen patterns that differ depending on the constitution, i.e., physiological status of the skin.
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Affiliation(s)
- Anna Medyukhina
- Institute of Photonic Technology, Albert-Einstein-Str. 9, 07745 Jena, Germany
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