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Cryo-laser scanning confocal microscopy of diffusible plant compounds
Plant Methods volume 14, Article number: 89 (2018)
The in vivo observation of diffusible components, such as ions and small phenolic compounds, remains a challenge in turgid plant organs. The analytical techniques used to localize such components in water-rich tissue with a large field of view are lacking. It remains an issue to limit compound diffusion during sample preparation and observation processes.
An experimental setup involving the infusion staining of plant tissue and the cryo-fixation and cryo-sectioning of tissue samples followed by fluorescence cryo-observation by laser scanning confocal microscopy (LSCM) was developed. This setup was successfully applied to investigate the structure of the apple fruit cortex and table grape berry and was shown to be relevant for localizing calcium, potassium and flavonoid compounds.
The cryo-approach was well adapted and opens new opportunities for imaging other diffusible components in hydrated tissues.
Plant growth involves intricate relations between cell water compartmentalization and cell wall mechanical properties . These relations involve cations for osmotic regulation and cell wall polysaccharide interactions, remodelling or deconstruction [2,3,4,5,6,7], but detailed knowledge on cation roles and interactions is impeded by their high mobility and/or low abundance in turgid tissue. Analytical methods for cation localization with a high spatial resolution are thus required. Due to the high water content of growing plant tissue, restraining the diffusion of mobile ions and preserving tissue integrity remain a challenge [8,9,10].
Specific chemical or physical fixation methods of plant tissue structures for microscopic observations exist . Cryo-techniques coupled to cryo-observation in large fields of view using fluorescent techniques are particularly suited to localize metallic cations and diffusible compounds at low concentrations. The cryogenic fixation of plant tissues for light microscopy, called cryo-observation, has been described  but has been rarely used in the fluorescent mode . This scarcity is most likely due to the difficulty in keeping the cold chain intact between sample cryo-fixation, cryo-sectioning and sample observation in frozen conditions. To that end, a method of fluorescence staining followed by cryo-fixation and cryo-observation by laser scanning confocal microscopy (LSCM) was developed and applied to the apple fruit cortex and table grape berry as models of turgid plant organs.
Staining of the sample with aqueous dye solutions must be completed prior to cryo-fixation. In the present case, it was achieved by the infusion or perfusion (Fig. 1) of fresh samples using acridine orange (AO), a fluorescent dye for the cell walls and anionic sites of cell organelles, DNA and RNA [14,15,16]. Compared to the direct staining of fresh sample sections, AO infusion was efficient, while perfusion showed limited dye diffusion in the vicinity of the capillary and required an increase of the laser intensity to reveal probe fluorescence. Although less efficient, the latter method may be useful to study specific tissue locations with limited operation artefacts. Due to its efficiency and simplicity, infusion staining was chosen in the following study. Such a staining method that is used prior to fixation and cutting a section has already been reported to successfully stain potassium in leaves .
The freezing process impacts turgid tissue structure due to ice crystal formation. The different cryo-fixation methods of AO infused samples were compared with regard to the apparent integrity of cell walls (Fig. 2). Observations at approximately − 25 °C revealed that slow freezing at − 20 °C (Fig. 2a, b), fast freezing in liquid nitrogen (Fig. 2c, d), and fast freezing in cold isopentane (Fig. 2e, f) impacted the overall tissue structure from most to least. These results agree with the impact of the rate of ice nucleation: the faster the freezing technique is, the less ice nucleation is present, and the better that structures are preserved. Slow-freezing under microwaves was also tested as an alternative to fast-freezing. Applying low-power microwaves during freezing drastically reduced the growth of ice nuclei and limited cell damage due to ice expansion . The fruit tissue cryo-fixed by this technique yielded remarkable results with regard to the preservation of its cell integrity (Fig. 2g, h). This was particularly the case for the grape berry, for which tissue integrity was the most difficult to preserve. However, this promising technique still needs development to optimize its parameters, such as microwave power, freezing temperature and processing time. The preservation of inner cells in apple and grape tissues was more efficient using cooled isopentane freezing (Fig. 2e, f) than using microwave freezing (Fig. 2g, h). This may be explained by the short processing time of isopentane freezing (60 s) compared to that of 3 h for the microwave technique due to the air blast freezer used. Furthermore, by avoiding the Leidenfrost effect, isopentane freezing was preferred over liquid nitrogen freezing. However, the measurement of cell wall thickness as a function of freezing conditions revealed an impact of the cooling rate on cell wall thickness (Fig. 3). Congo Red-stained apple cell walls at approximately 200 µm from the cuticle were 2.5-fold thicker in tissue frozen by cold isopentane than in fresh tissue (room temperature), while tissue frozen at − 20 °C or by liquid nitrogen gave an intermediate average thickness.
Observation of diffusible compounds
As an application of the entire process on turgid plant organs, calcium, potassium and flavonoid compounds were localized in apple fruit and table grape berry tissue. Samples were independently infused with the calcium probe Fluo-3, potassium probe PBFI, and flavonoid probe DPBA. The samples were then fast-frozen in cold isopentane, cryo-sectioned and observed by cryo-LCSM (Fig. 4a–f). The results showed diffuse calcium staining in the cell wall, while fluorescence spots were observed within cells (Fig. 4a, b). Potassium and flavonoids were distributed in the entire fruit tissue (Fig. 4c–f), and specific locations appeared in the cytosol next to the cell walls (Fig. 4e, f). As a comparison, the direct staining of fresh sections yielded weaker labelling mainly due to the absence of intracellular staining (Fig. 4g–l). These observations may be attributed to low compound concentrations resulting from their diffusion during staining and loss during washes as well as from the higher diffusion of quenchers inducing faster fluorescence bleaching at room temperature [19, 20].
The experimental setup presented here was developed to image metallic cations and phenolic compound distributions in in vivo-like fleshy fruit by fluorescence confocal microscopy. Particular care was paid to the issues related to the low concentration and highly diffusible properties of these components. The fruit region of interest was established at the epidermal areas of grape and apple fruit. To allow full cell observation (range of cell diameter i.e., 10–100 µm) , section thicknesses needed to be adapted according to the tissue. Despite the particular physicochemical and mechanical characteristics of samples, sections with thicknesses of 100 µm were achieved but required dexterity for their handling, particularly for grape tissue. In addition, the physical state of the sample is essential when studying diffusible components . For turgid plant organs such as fleshy fruit, water, which amounts to 80–85% of their weight, determines the morphological, physiological and physical properties of tissues at room temperature or in frozen solid states. Cryo-fixation limits the diffusion and redistribution of highly diffusible components [22, 23] but has several drawbacks. First, it requires that the sample be stained before freezing, and second, it faces the issue of structural damage by ice crystals [24, 25]. We found that fresh tissue infusion remains the most efficient and user-friendly method. It is well adapted to turgid plant tissue due to its porosity and exchange properties. Applied to apple and grape tissues, labelling was observed up to the fifth or sixth cell layer from the exposed area (approximately 100 µm for each layer) after two hours of staining. To reduce tissue destruction by ice crystals, cryogenic techniques have been developed. Plunge freezing , jet freezing, or slam freezing in cryogenic fluid or high pressure freezing (HPF) transform liquid water to a vitreous solid phase . Currently, HPF is recognized as the method of choice for cryopreservation and is well adapted for ultramicrotome sections. This fast freezing process (≈ 0.5 ms) allows cell preservation up to 600 μm in thickness  and is optimal for investigating small cells and objects by the cryo-electron microscopy of vitreous samples (CEMOVIS) , cryo-correlative light transmission electron microscopy (cryo-CLEM)  or cryo-correlative light scanning electron microscopy . These techniques are suited for preparing samples for cryo-transmission electron microscopy (cryo-TEM), which has a field of view of smaller than 100 µm2 and is thus not suitable for large sample sizes when a field of view of more than 500 µm2 is required. In that context, hand freezing at atmospheric pressure remains the simplest, fastest and most repeatable method of cryo-fixation, as samples are dipped in a cryogen, such as cold isopentane. The hand freezing method used here was inspired by the freezing step involved in the Tokuyasu method, with no sucrose infiltration, as fruit tissues are naturally rich in osmolytes that logically act as natural cryoprotectants . Cryo-observation in light microscopy has already been developed , but to our knowledge, only a few commercial or homemade fluorescence microscopes equipped with a cryo-chamber cooled by liquid nitrogen are available. They are specifically used to observe vitrified ultrathin sections by fluorescence microscopy as a preliminary step prior to observation by cryo-TEM. In available cryo-fluorescence microscopy setups, dry lenses with relatively long working distances (WDs) and limited numerical apertures (NAs) are used . Recently, a prototype of a LSCM stage and objective lens were described for the high-resolution cryo-observation of sub-cellular localization of animal proteins . In our setup, the inverted optic of the LSCM possesses a short WD that maximizes the NA. These are key factors determining the fluorescence sensitivity and spatial resolution required to localize compounds at low concentrations, such as metallic cations or phenolic compounds in fruit tissue, with a large field of view.
The freezing of water-rich biological materials has been reported to affect cell contraction and the swelling of cell walls . In the present study, the cell wall thickness was observed to vary according to the apple cryo-fixation temperature. As postulated , the extracellular water medium freezes first and provokes an outward water flux from the cells to osmotically equilibrate intracellular and extracellular media. Water in biomaterials is also known to expand by almost 9% during freezing and develops transient stresses when the material is frozen from all sides . The cell wall swelling observed in relation to the freezing rate and temperature may be related to these mechanisms, but further studies are required to understand the water behaviour in the fruit cell wall during cryo-fixation. Although water flux and osmolyte redistribution may have occurred during sample cryo-fixation, which impacted the diffusible component distribution, these artefacts may have been limited. Indeed, the two types of calcium labelling distribution observed in both apple and grape tissues showing diffuse staining in cell walls and intense fluorescence spots in cells (Fig. 4a, b) were in agreement with their reported presence in nuclei, vesicles and plant cell walls [22, 35]. Furthermore, the observation of potassium labelling in the apoplast and cell wall of fresh tissue (Fig. 4i, j) and in cells (Fig. 4c, d) of frozen tissue was in agreement with its apoplastic, cytosolic and vacuolar location in fleshy fruit cells . In the literature, calcium and potassium were measured directly on isolated cells and organelles using a fluorescent probe. Lastly, flavonoid distribution mainly observed in the cytosol close to the cell wall supports their putative sites of synthesis. Conversely, their proposed accumulation in the vacuole was not dominant in the present observations in apple and grape, but such localization remains a matter of debate (Fig. 4e, f) . The cellular localization of these different diffusible compounds in the two fleshy fruit parenchymal tissues demonstrated the benefit of the cryo-method.
The localization of highly diffusible and low concentrated components such as metallic cations and flavonoids was achieved in fluorescence mode by LSCM. The reduction of component mobility was realized by keeping samples in a frozen state during the entire preparation process and by the design and adaptation of a cryo-LSCM setup for the observation of frozen sections. The successful localization of calcium, potassium and flavonoids in apple and grape fruits as a model of turgid tissue illustrated the benefits of the cryo-approach. The results indicated that the freezing temperature and cooling rate remain key parameters in the preservation of hydrated tissue integrity and require further studies to better control the associated osmotic-related structural rearrangements. The extension of this approach to other highly diffusible compounds will benefit from the development of specific and sensitive diffusible fluorescent markers. This approach opens new opportunities for studies of small metabolites and ions in the plant sciences.
The fruit tissue nomenclature used in this study is shown in Fig. 5. Gala apples and Italia white table grapes were obtained from a local retail store. Regions of interest corresponding to the apple cortex and grape berry with epidermis were sampled as cubes of approximately 0.125 cm3 using a razor blade (Fig. 1).
Sample preparation for microscopy
Samples were stained by infusion or perfusion before freezing according to different paths followed by cryo-sectioning and cryo-observation. For comparison, samples were also stained by a conventional method and observed in an unfrozen state.
Fluorescence stains: Acridine orange (AO hydrochloride salt; MERCK Calbiochem, France) was prepared as a 0.02% w/v solution in 0.01 M PBS buffer (pH 7). Congo Red stain (Congo Red powder, FLUKA, Switzerland) was prepared as a 0.1 mg/mL solution in deionized water at pH 5. Fluo-3 calcium probe (Fluo-3 pentapotassium salt, Thermo Fisher Scientific, France) and PBFI potassium probe (PBFI, tetraammonium salt, Thermo Fisher Scientific, France) were prepared as a 0.1 mg/mL solution in MES (25 mM) + Tris (10 mM) buffer (pH 6.0)  and kept as a stock solution in an amber flask at 4 °C. The phenolic probe DPBA (2-Aminoethyl diphenylborinate, Sigma-Aldrich, UK) was prepared by dissolving 20 mg in 5 mL of ethanol and 15 ml of phosphate buffer solution 0.01 M (pH 7).
The conventional staining of fruit sections (see below for sectioning details) was performed by applying 2 mL of staining solution onto the sections for 5–10 min at room temperature. Sections were then rinsed 3 times with buffer for approximately 5 min each.
Staining by infusion of fruit samples: Cubes of apple and grape were bathed in staining solutions for 2 h at 5 °C (Fig. 1a).
Staining by perfusion of entire fruit: Staining solution was introduced in specific areas of the entire fruit using a syringe (5 mL) filled with 2 mL of staining solution connected to 10 cm of capillary tubing (inner diam. 1 mm) inserted in the fruit. The tubing was perforated at the contact zone in the fruit, with a 10-mm length and a 0.8-mm pore size (approximately 10 apertures) to allow for the diffusion of the stain. To ensure the flow of the stain in the fruit, the syringe outlet was set 10 cm above the capillary outlet. The flow rate was approximately 125 µL/h. Diffusion was applied overnight at 5 °C (Fig. 1b).
Cryo-fixation was achieved following several methods to obtain different cooling rates:
The slow freezing of samples at − 20 °C was conducted for at least 24 h in a conventional freezer.
Two fast-freezing methods were tested using the cryogen: for the first one, the sample was directly plunged in liquid nitrogen, whereas for the second one, it was plunged in isopentane (2-methylbutan anhydrous > 99%, SIGMA) cooled by liquid nitrogen. In both cases, the freezing duration was 60 s.
Freezing under microwave  was conducted with the following parameters: microwave equipment (SAIREM, France) operated at a frequency of 2450 MHz, the microwave chamber stabilization time was 30 min at 5 °C, a temperature of − 30 °C was set using an air blaster (ACFRI, France), the microwave power was 5 ± 0.1 W, and the duration of freezing was 3 h.
Fresh specimens were sectioned at room temperature using a vibrating blade microtome (Vibratome HM 650 V, MICROM, France), stained by a conventional method and collected between 60 × 24 mm glass cover slips (#1) (Thermo Fisher Scientific, Germany) separated by a 250-µm-thick spacer (Gene Frame, 25 µL, 1 × 1 cm2, Thermo Fisher Scientific, UK). The sectioning parameters used were a section frequency of 60 Hz, a vibration amplitude of 1.0 mm, and a cutting speed of 1.0 mm/sec. Sections were cut to a thickness of 100 µm.
Frozen specimens were cryo-sectioned using a cryotome (microtome cryostat HM 500 OM, MICROM, France) operated at − 20 °C. The sample cube was fixed on the support section using a water droplet free of cryo-protectant. The cryotome steel blade was a type C profile (16 cm length). The cutting speed was fixed at 1 mm/sec, and the thickness of the sections was 100 µm. Sections were picked up and placed between two 22 × 22 mm #1 glass cover slips (Thermo Fisher Scientific, Germany), which were sealed by frozen water microdroplets.
In all cases, sectioning was performed on the stained sample contact area.
The transfer of cold sections within cover slips to the confocal microscope was conducted rapidly over liquid nitrogen.
Laser scanning confocal microscopy (LSCM) observations
LSCM (Eclipse Ti inverted microscope, NIKON Inc. Japan) was used both in bright field and fluorescence modes. Observations were made using a 20 × magnification objective lens and, if needed, a numerical zoom of 3x. The laser excitation and fluorescence emission wavelengths were 488 nm for acridine orange, 500–530 nm for Fluo-3 and DPBA dyes, 488 nm and 600 nm for Congo Red dye, and 375 nm and 500–530 nm for PBFI dye. Laser intensity and gain were adjusted visually for sample fluorescence.
Cryo-observation by LSCM
The critical points to manage for LSCM cryo-observation were sample section warming induced by environmental factors and by the laser during observation as well as frost formation on the sample slide. The sample slide was placed onto a Peltier stage (PE100, Linkam Scientific, Epsom UK) under which an adaptable flexible rubber seal was fixed between the objective lens and the stage (Fig. 6). This closed space between the lens and the stage was flushed by a cooled nitrogen gas flux to prevent frost formation on the sample slide. A glass container filled with dry ice was placed on top of the sample slide. The measured temperature of the Peltier stage was approximately − 25 °C. The container transparency allowed the microscope optical condenser to observe the sample in a bright field.
Cell wall thickness measurement
Cell wall thickness was specifically evaluated on four apple fruit samples after staining with Congo Red (a cell wall specific dye) and observed at room temperature after slow freezing at − 20 °C and after fast freezing by liquid nitrogen and by isopentane. Four sections per sample were recovered, and five cell wall measurements (a total of 80 measurements) were performed on the cell layer at approximately 200 µm from the cuticle using NIS Analysis software (Nikon).
Hamant O, Traas J. The mechanics behind plant development. N Phytol. 2010;185(2):369–85.
Jarvis MC, Briggs SPH, Knox JP. Intercellular adhesion and cell separation in plants. Plant, Cell Environ. 2003;26:977–89.
White PJ, Broadley MR. Calcium in plants. Ann Bot. 2003;92(4):487–511.
Dumville JC, Fry SC. Solubilisation of tomato fruit pectins by ascorbate: a possible non-enzymatic mechanism of fruit softening. Planta. 2003;217:951–61.
Francoz E, Ranocha P, Nguyen-Kim H, Jamet E, Burlat V, Dunand C. Roles of cell wall peroxidases in plant development. Phytochemistry. 2015;112:15–21.
Rice RW. The physiological role of minerals in the plant. In: Datnoff LE, Elmer WH, Huber DM, editors. Mineral nutrition and plant disease. St Paul: APS Press; 2007. p. 9–29.
Sattelmacher B. The apoplast and its significance for plant mineral nutrition. N Phytol. 2000;149:167–92.
Mentré P. Preservation of the diffusible cations for SIMS microscopy. I. A problem related to the state of water in the cell. Biol Cell. 1992;74(1):19–30.
Chandra S, Morrison GH. Sample preparation of animal tissues and cell cultures for secondary ion mass spectrometry (SIMS) microscopy. Biol Cell. 1992;74(1):31–42.
Moore KL, Chen Y, van de Meene AM, Hughes L, Liu W, Geraki T, Mosselmans F, McGrath SP, Grovenor C, Zhao FJ. Combined NanoSIMS and synchrotron X-ray fluorescence reveal distinct cellular and subcellular distribution patterns of trace elements in rice tissues. N Phytol. 2014;201(1):104–15.
Palin R, Geitmann A. The role of pectin in plant morphogenesis. Biosystems. 2012;109(3):397–402.
Echlin P. Low-temperature microscopy and analysis. Berlin: Springer; 1992.
Kitin P, Voelker SL, Meinzer FC, Beeckman H, Strauss SH, Lachenbruch B. Tyloses and phenolic deposits in xylem vessels impede water transport in low-lignin transgenic poplars: a study by cryo-fluorescence microscopy. Plant Physiol. 2010;154(2):887–98.
Widholm JM. The use of fluorescein diacetate and phenosafranine for determining viability of cultured plant cells. Stain Technol. 1972;47(4):189–94.
Houtman CJ, Kitin P, Houtman JCD, Hammel KE, Hunt CG. Acridine orange indicates early oxidation of wood cell walls by fungi. PLoS ONE. 2016;11(7):e0159715.
Nafisi S, Saboury AA, Keramat N, Neault J-F, Tajmir-Riahi H-A. Stability and structural features of DNA intercalation with ethidium bromide, acridine orange and methylene blue. J Mol Struct. 2007;827(1–3):35–43.
Mühling KH, Sattelmacher B. Determination of apoplastic K + in intact leaves by ratio imaging of PBFI fluorescence. J Exp Bot. 1997;48(8):1609–14.
Xanthakis E, Le-Bail A, Ramaswamy H. Development of an innovative microwave assisted food freezing process. Innov Food Sci Emerg Technol. 2014;26:176–81.
Lakowicz JR. Principles of fluorescence spectroscopy. 3rd ed. New York: Springer; 2006.
Nahmani M, Lanahan C, DeRosier D, Turrigiano GG. High-numerical-aperture cryogenic light microscopy for increased precision of superresolution reconstructions. Proc Natl Acad Sci U S A. 2017;114(15):3832–6.
Bain JM, Robertson RN. The physiology of growth in apple fruits. I. Cell size, cell number, and fruit development. Aust J Sci Res B. 1951;4(2):75–107.
Hare DJ, New EJ, de Jonge MD, McColl G. Imaging metals in biology: balancing sensitivity, selectivity and spatial resolution. Chem Soc Rev. 2015;44(17):5941–58.
McRae R, Bagchi P, Sumalekshmy S, Fahrni CJ. In Situ Imaging of Metals in Cells and Tissues. Chem Rev. 2009;109(10):4780–827.
Moor H. Theory and practice of high pressure freezing. In: Steinbrecht RA, Zierold K, editors. Cryotechniques in biological electron microscopy. Berlin: Springer; 1987. p. 175–91.
Dahl R, Staehelin LA. High-pressure freezing for the preservation of biological structure: theory and practice. J Elec Mic Tech. 1989;13(3):165–74.
Ryan PR, Newman IA, Arif I. Rapid calcium exchange for protons and potassium in cell walls of Chara. Plant, Cell Environ. 1992;15(6):675–83.
Kanno H, Speedy RJ, Angell CA. Supercooling of water to − 92 °C under pressure. Science. 1975;189:880–1.
Moore KL, Lombi E, Zhao F-J, Grovenor CRM. Elemental imaging at the nanoscale: NanoSIMS and complementary techniques for element localisation in plants. Anal Bioanal Chem. 2012;402(10):3263–73.
Al-Amoudi A, Chang JJ, Leforestier A, McDowall A, Salamin LM, Norlén LP, Richter K, Blanc NS, Studer D, Dubochet J. Cryo-electron microscopy of vitreous sections. The EMBO Journal. 2004;23:3583–8.
Schorb M, Briggs JA. Correlated cryo-fluorescence and cryo-electron microscopy with high spatial precision and improved sensitivity. Ultramicroscopy. 2014;143:24–32.
Strnad M, Elsterova J, Schrenkova J, Vancova M, Rego RO, Grubhoffer L, Nebesarova J. Correlative cryo-fluorescence and cryo-scanning electron microscopy as a straightforward tool to study host-pathogen interactions. Sci Rep. 2015;5:18029.
Tokuyasu KT. A technique for ultracryotomy of cell suspensions and tissues. The Journal of Cell Biology. 1973;57(2):551–65.
Floury J, Le Bail A, Pham QT. A three-dimensional numerical simulation of the osmotic dehydration of mango and effect of freezing on the mass transfer rates. J Food Engin. 2008;85(1):1–11.
Ishii T, Matsunaga T, Pellerin P, O’Neill MA, Darvill A, Albersheim P. The plant cell wall polysaccharide rhamnogalacturonan II self-assembles into a covalently cross-linked dimer. J Biol Chem. 1999;274(19):13098–104.
Bush DS. Calcium regulation in plant cells and its role in signaling. Annu Rev Plant Biol. 1995;46(1):95–122.
Rogiers SY, Coetzee ZA, Walker RR, Deloire A, Tyerman SD: Potassium in the Grape (Vitis vinifera L.) Berry: Transport and Function. Front Plant Sci 2017, 8:1629.
Kitamura S: Transport of flavonoids: from cytosolic synthesis to vacuolar accumulation. In: The science of flavonoids. Springer; 2006: 123–146.
Hanyu Y, Ichikawa M, Matsumoto G. An improved cryofixation method: cryoquenching of small tissue blocks during microwave irradiation. J Microsc. 1992;165(2):255–71.
KV, ML, RS, CG designed the study. KV performed the experiments and analysed the data. KV drafted the manuscript. ML, RS, CG, CR revised the manuscript. All authors read and approved the final manuscript.
Prof. Alain Lebail and Piyush-Kumar Jha, Ph.D., of the GEPEA team, ONIRIS (Nantes, France), are thanked for their discussions on microwave freezing, making their microwave equipment available and helping with its operation.
The authors declare that they have no competing interests.
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Vidot, K., Gaillard, C., Rivard, C. et al. Cryo-laser scanning confocal microscopy of diffusible plant compounds. Plant Methods 14, 89 (2018). https://doi.org/10.1186/s13007-018-0356-x
- Cryogenic fixation
- Cryo-confocal microscopy
- Metallic ions