We thank Dr. R. Terada, Dr. Z. Shimatani, and Dr. H. Tsuji for providing us with the OsMADS15-mOrange seeds; Dr. D. Kurihara for providing us with the NGCN construction; and Dr. R. Shim for editing our manuscript. This work was funded by JSPS KAKENHI (grant numbers JP20H05912, 20H05778, 20H05779) and by the SATREPS program (no. JPMJSA1706) of the JST and JICA.

1. Preparation of the fixative solution
<ol>
	<li>Transfer 70 mL of sterile water into a glass bottle and add 10 g of paraformaldehyde (PFA). 
	CAUTION: PFA is toxic; hence, wearing gloves is recommended.</li>
	<li>Add 2 mL of 1 N NaOH to dissolve the PFA solution.</li>
	<li>Dissolve the PFA solution with continuous stirring (300-500 rpm) at 60 &#176;C for about 1 h until the PFA solution is transparent.</li>
	<li>Add sterilized water to increase the volume of the PFA solution to 100 mL. 
	NOTE: The PFA solution was prepared freshly before use. Moreover, a PFA solution stored at 4 &#176;C can be used for approximately 2 months.</li>
	<li>Immediately before sampling, add 25 mL of 60 mM HEPES (pH 7.4), 3 mL of 1 M sucrose, and 2 mL of sterile water into 20 mL of 10 % PFA to prepare a 50 mL fixative solution.</li>
</ol>
2. Preparation of the clearing solution (CS)
<ol>
	<li>Weigh and mix 7.5 g of sodium deoxycholate, 5 g of xylitol, and 12.5 g of urea (see Table of Materials) in 50 mL of sterile water. 
	NOTE: Sodium deoxycholate powder was weighed in a general laboratory draft chamber to prevent airborne dispersion.</li>
	<li>Dissolve the ingredients (step 2.1.) using a magnetic stirrer to prepare the CS. 
	NOTE: The present study used in-house prepared clearing solution (CS), but a commercially available clearing solution, ClearSee (see Table of Materials), can also be used.</li>
	<li>Transfer the CS into a 50 mL conical tube and store it at room temperature (15-30 &#176;C) in the dark. 
	&#8203;NOTE: The CS can be stored for more than 1 year.</li>
</ol>
3. Sampling
<ol>
	<li>Cut the roots carefully without damaging the plants. Wash the plants with water to remove the dirt. 
	NOTE: This method studied the observation of tissues from the three-leaf stage (LS) to flag LS. The present study used the rice cultivars Nipponbare (Nip) and Taichung 65 (T65) at the 8-10 LS.</li>
	<li>Peel off the old outer leaves with hands and tweezers. There were about 2-3 leaves left.</li>
	<li>Cut the tissue from the SAM/young panicle to the base with a single-edged razor using a sliding motion to avoid crushing the cells (Figure 1A-C). If the position of the SAM/young panicle is not visible, cut it longer.</li>
	<li>Since the cross-section of the rice shoot has&#160;an oval shape (Figure 1D), shave off one side of the oval thinly in the direction of its long axis with a double-edged razor (Figure 1E-F). 
	NOTE: This step made it easier for the fixative solution to penetrate the sample. A horizontal cutting surface makes the sample easier to stick to a vibrating micro-slicer (see Table of Materials) tray.</li>
	<li>Confirm the position of the SAM/young panicle by the appearance of a whitish color in the sample (Figure 1G). Trim off excess tissue. 
	NOTE: The length of the sample should be adjusted to the maximum length that can be trimmed using a vibrating micro-slicer. If the sample is too long, divide it into several pieces.</li>
</ol>
4. Fixation of the samples
<ol>
	<li>Pipette 1 mL of the fixative solution (prepared in step 1.) to a 1.5 mL microcentrifuge tube and immediately put in the samples. 
	NOTE: Ensure that the amount of sample does not exceed 20% of the volume of the fixative solution.</li>
	<li>Cut a piece of paraffin film into 2.5 cm2. Shape the paraffin film into balls and place them on top of the samples to prevent them from floating out of the fixative solution.</li>
	<li>Place the tube containing the sample in a desiccator. Then, close the lid of the desiccator and start the vacuum pump to depressurize the inside of the desiccator until &#8722;0.095 MPa slowly.</li>
	<li>After closing the desiccator at &#8722;0.095 MPa, turn off the vacuum pump and allow it to stand for 30 min at room temperature. 
	NOTE: The vacuum level was such that bubbles appeared gradually in the samples.</li>
	<li>Open the desiccator slightly and slowly return it to atmospheric pressure. Reduce the pressure of the desiccator to &#8722;0.095 MPa, turn off the vacuum pump, and allow the mixture to stand for 30 min at room temperature.</li>
	<li>Open the desiccator slightly and slowly return it to atmospheric pressure. If the sample is correctly fixed, it sinks into the fixative solution. If it did not sink, reduce the pressure again.</li>
	<li>Remove the paraffin film, close the lid, and keep the tubes overnight at 4 &#176;C. 
	&#8203;NOTE: Samples were fixed in fixative solution for at least 2 h. It can be stored for ~1 week.</li>
</ol>
5. Trimming the fixed sample
<ol>
	<li>Remove the excess fixative solution from the sample using lint-free wipes. 
	NOTE: Excess fixative solution prevents the sample from sticking properly onto the tray.</li>
	<li>Fix the sample on a vibrating micro-slicer tray with instant glue. Place it on a tray with the flat side down, which was shaved off during sampling. 
	NOTE: Due to the structure of the rice shoot, it must be trimmed from the base toward the SAM/young panicle.</li>
	<li>Set the trimming conditions according to the fixed sample. 
	NOTE: In this study, trimming was set to THICK, 130 &#181;m; WIDE, 15 mm; FREQUENCY, 15%; and CUTTING SPEED, 32 mm.</li>
	<li>Adjust the sample position with the RVS or FWD button and the UP or DOWN button. Fill the tray with deionized water until all the samples are immersed. After filling the tray, press the START button. Place the trimmed samples on a glass slide with a drop of 1x PBS. 
	NOTE: Shift the position of the sample to the other side after each trimming since the hard sample wears out the razor blade.</li>
	<li>After checking the sample containing the target site under a stereomicroscope, transfer the trimmed sample to a multiwell plate with 1 mL of 1x PBS. 
	&#8203;NOTE: Choose the number of wells according to the size of the sample. In this study, a 12-multiwell plate was used.</li>
</ol>
6. Treatment with the clearing solution
<ol>
	<li>Remove the 1x PBS from the multiwell plate and add fresh 1x PBS. Let it stand for 1 min.</li>
	<li>Remove 1x PBS and add the CS. 
	NOTE: The amount of CS must be five times the sample volume.</li>
	<li>Place the multiwell plate containing the sample in a desiccator. Then, close the lid of the desiccator and start the vacuum pump to depressurize the inside of the desiccator until &#8722;0.09&#160;MPa slowly.</li>
	<li>After closing the desiccator at &#8722;0.09 MPa, turn off the vacuum pump and let it stand for 1 h at room temperature.</li>
	<li>Open the desiccator slightly and slowly return it to atmospheric pressure.</li>
	<li>Pour deionized water into the gap between the wells to prevent the evaporation of the CS. Store the multiwell plates at room temperature in the dark for clearing. 
	NOTE: Gently shake the multiwell plate every 1-2 days to diffuse the chlorophyll and other components.</li>
	<li>When the CS turns green, replace it with fresh solution.</li>
</ol>
7. Cell wall staining with chemical dye
<ol>
	<li>Pipet the calcofluor white solution (1 mL, final concentration: 1 mg/mL in the clearing solution, see Table of Materials) into a multiwell plate. Place the samples in the dye solution and incubate for 1 h. 
	NOTE: The volume of the dye must not exceed 10% of the volume of the CS.</li>
	<li>Wash the stained samples in another multiwell plate with 1 mL of the CS for at least 1 h.</li>
</ol>
8. Observation with a confocal laser microscope
<ol>
	<li>Place a drop of CS onto a microscope slide and transfer the treated (with CS) samples onto the slide. 
	NOTE: As the treated samples are soft, they must be carefully handled with tweezers.</li>
	<li>Cover the sample with a glass coverslip to prevent the evaporation of the CS. 
	NOTE: The CS precipitates easily.</li>
	<li>Observe the treated samples under a confocal laser microscope. 
	NOTE: After observation, the treated samples can be returned to the CS for further observations later.</li>
</ol>

<ol><li>Kurihara, D., Mizuta, Y., Sato, Y., Higashiyama, T. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((ClearSee%3A+A+rapid+optical+clearing+reagent+for+whole-plant+fluorescence+imaging%5BTitle%5D)+AND+%22Development%22%5BJournal%5D)">ClearSee: A rapid optical clearing reagent for whole-plant fluorescence imaging.</a> Development. 142 (23), 4168-4179 (2015).</li>
<li>Hasegawa, J., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((Three-dimensional+imaging+of+plant+organs+using+a+simple+and+rapid+transparency+technique%5BTitle%5D)+AND+%22Plant+and+Cell+Physiology%22%5BJournal%5D)">Three-dimensional imaging of plant organs using a simple and rapid transparency technique.</a> Plant and Cell Physiology. 57 (3), 462-472 (2016).</li>
<li>Musielak, T. J., Slane, D., Liebig, C., Bayer, M. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((A+versatile+optical+clearing+protocol+for+deep+tissue+imaging+of+fluorescent+proteins+in+Arabidopsis+thaliana%5BTitle%5D)+AND+%22PLoS+One%22%5BJournal%5D)">A versatile optical clearing protocol for deep tissue imaging of fluorescent proteins in Arabidopsis thaliana.</a> PLoS One. 11 (8), 0161107(2016).</li>
<li>Pandey, K. B., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((Plant+roots+sense+soil+compaction+through+restricted+ethylene+diffusion%5BTitle%5D)+AND+%22Science%22%5BJournal%5D)">Plant roots sense soil compaction through restricted ethylene diffusion.</a> Science. 371 (6526), 276-280 (2021).</li>
<li>Ejaza, M., Bencivenga, S., Tavaresa, R., Busha, M., Sablowski, R. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((ARABIDOPSIS+THALIANA+HOMEOBOX+GENE+1+controls+plant+architecture+by+locally+restricting+environmental+responses%5BTitle%5D)+AND+%22Proceedings+of+the+National+Academy+of+Sciences+of+the+United+States+of+America%22%5BJournal%5D)">ARABIDOPSIS THALIANA HOMEOBOX GENE 1 controls plant architecture by locally restricting environmental responses.</a> Proceedings of the National Academy of Sciences of the United States of America. 118 (17), (2021).</li>
<li>Smetana, O., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((High+levels+of+auxin+signalling+define+the+stem-cell+organizer+of+the+vascular+cambium%5BTitle%5D)+AND+%22Nature%22%5BJournal%5D)">High levels of auxin signalling define the stem-cell organizer of the vascular cambium.</a> Nature. 565 (7740), 485-489 (2019).</li>
<li>Chu, T. T. H., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((Sub-cellular+markers+highlight+intracellular+dynamics+of+membrane+proteins+in+response+to+abiotic+treatments+in+rice%5BTitle%5D)+AND+%22Rice%22%5BJournal%5D)">Sub-cellular markers highlight intracellular dynamics of membrane proteins in response to abiotic treatments in rice.</a> Rice. 11 (1), 23(2018).</li>
<li>Nagaki, K., Yamaji, N., Murata, M. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((ePro-ClearSee%3A+A+simple+immunohistochemical+method+that+does+not+require+sectioning+of+plant+samples%5BTitle%5D)+AND+%22Scientific+Reports%22%5BJournal%5D)">ePro-ClearSee: A simple immunohistochemical method that does not require sectioning of plant samples.</a> Scientific Reports. 7, 42203(2017).</li>
<li>Sato, M., Akashi, H., Sakamoto, Y., Matsunaga, S., Tsuji, H. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((Whole-tissue+three-dimensional+imaging+of+rice+at+single-cell+resolution%5BTitle%5D)+AND+%22International+Journal+of+Molecular+Sciences%22%5BJournal%5D)">Whole-tissue three-dimensional imaging of rice at single-cell resolution.</a> International Journal of Molecular Sciences. 23 (1), 40(2022).</li>
<li>Matsuo, T., Hoshikawa, K. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((Science+of+the+Rice+Plant%3A+Morphology%5BTitle%5D)+AND+%22Food+and+Agriculture+Policy+Research+Center%22%5BJournal%5D)">Science of the Rice Plant: Morphology.</a> Food and Agriculture Policy Research Center. , Tokyo, Japan. (1993).</li>
<li>Kobayashi, K., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((Inflorescence+meristem+identity+in+rice+is+specified+by+overlapping+functions+of+three+AP1%2FFUL-Like+MADS+box+genes+and+PAP2%2C+a+SEPALLATA+MADS+box+gene%5BTitle%5D)+AND+%22Plant+Cell%22%5BJournal%5D)">Inflorescence meristem identity in rice is specified by overlapping functions of three AP1/FUL-Like MADS box genes and PAP2, a SEPALLATA MADS box gene.</a> Plant Cell. 24 (5), 1848-1859 (2012).</li>
<li>Tamaki, S., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((FT-like+proteins+induce+transposon+silencing+in+the+shoot+apex+during+floral+induction+in+rice%5BTitle%5D)+AND+%22Proceedings+of+the+National+Academy+of+Sciences+of+the+United+States+of+America%22%5BJournal%5D)">FT-like proteins induce transposon silencing in the shoot apex during floral induction in rice.</a> Proceedings of the National Academy of Sciences of the United States of America. 112 (8), 901-910 (2015).</li>
<li>Kodama, Y. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((Time+gating+of+chloroplast+autofluorescence+allows+clearer+fluorescence+imaging+In+Planta%5BTitle%5D)+AND+%22PLoS+One%22%5BJournal%5D)">Time gating of chloroplast autofluorescence allows clearer fluorescence imaging In Planta.</a> PLoS One. 11 (3), 0152484(2016).</li>
<li>Sakamoto, Y., et al. <a target="_blank" href="http://www.ncbi.nlm.nih.gov/pubmed?term=((Improved+clearing+method+contributes+to+deep+imaging+of+plant+organs%5BTitle%5D)+AND+%22Communications+Biology%22%5BJournal%5D)">Improved clearing method contributes to deep imaging of plant organs.</a> Communications Biology. 5 (1), 12(2022).</li>
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</ol>

The authors have no conflicts of interest to declare.

Critical steps of the protocol 
The critical steps in this protocol are fixation and trimming. Rice shoots have hard, thick, or layered tissues that limit penetration of the fixative solution. To improve the permeability of the fixative solution, one side of the tissue was thinly shaved at sampling, as shown in Figure 1E-F.&#160;In addition, the vacuum treatments were repeated twice using higher pressure. Furthermore, the samples were fixed overnight at 4 &#176;C instead of the usual 2 h fixation at 4 &#176;C.
The key point in the trimming step is to determine the thickness of the tissues to be prepared to observe the fluorescent proteins while preserving their internal structure following a short period of CS treatment. As shown in Figure 2C, the 1 mm thick samples, hand-trimmed as thin as possible, became transparent in only a limited number of tissues even after 3 months of CS treatment. Therefore, the trimming step is essential for deep fluorescence observation of adult rice shoots. In this study, the samples were trimmed to a thickness of 130 &#181;m, as shown in Figure 2D. The 130 &#181;m thickness allowed for clearing the leaves after 1 week of CS treatment and the whole sample after 2 weeks. Adult rice shoots at the 9-10 LS were used in this study. Thick but softer tissues from younger rice shoots may be cleared faster with the CS treatment. The thickness of the samples and the duration of the CS treatment should be adjusted according to the tissue type, condition, and thickness of the 3D structure to be observed.
Modifications and troubleshooting methods 
The CS precipitated easily at low temperatures. The precipitated CS cannot preserve the fluorescent proteins; hence, care must be taken when storing the samples at the proper temperature. In addition, both the CS and fixative solution&#160;have no antiseptic effect; therefore, fluorescent proteins will be degraded if contaminated. Soil-grown rice is prone to fungal growth; hence, the sampling and handling of samples must be performed with care to avoid contamination.
Excess fluorescent dyes in the buffer may give off background fluorescence and interfere with microscopic observations. For example, a calcofluor white solution containing Evans blue dye was previously used. After staining for 1 h and washing for 1 h, the fluorescent proteins of OsMADS15-mOrange were observed using a 555 nm laser. However, fluorescent proteins could not be observed because of the background fluorescence derived from Evans blue dye. This background fluorescence was almost eliminated by washing the samples for 2 h. Moreover, the fluorescent proteins were clearer if the samples were left overnight. Therefore, a pure calcofluor white solution was used in this study. Background fluorescence derived from the fluorescent dye should be checked using different laser wavelengths before observations.
Limitations of the method 
As shown in Figure 3, deep fluorescent proteins were observed in the samples that were 130 &#181;m thick after 2 weeks of CS treatment. This is consistent with the results shown in Figure 2D, where the 130 &#181;m thick sample became transparent after 2 weeks of CS treatment. However, as shown in Figure 3A, auto-fluorescence of the cytoplasm was still noticeable in the nodes after 2 weeks and was only completely removed after 4 weeks of CS treatment. Nodes have a high cell density and, therefore, require a longer time to remove auto-fluorescent materials.
As shown in Figure 3C, deep fluorescent proteins were observed in the leaves without CS treatment, but the brightness was weaker than that in the nodes and internodes at the same depth of 20 &#181;m. After 1 week of CS treatment, the fluorescent proteins were brighter. Chlorophyll is abundant in leaves and absorbs 488 nm of excitation light. They also have orange/red auto-fluorescence, which can interfere with the observation of fluorescent proteins using a 555 nm laser. After 1 week of CS treatment, chlorophyll and other auto-fluorescent materials were removed, resulting in high signal-to-noise ratio images.
The depths that could be observed in tissues after 2 weeks and 4 weeks of CS treatment were not significantly different, although the fluorescent proteins appeared weaker after 4 weeks (Figure 3). Normally, the brightness of fluorescent proteins and auto-fluorescence weakens with time, resulting in a higher signal-to-noise ratio. Therefore, fluorescent proteins can be observed more clearly by adjusting the microscopic conditions and image processing. Based on these results, it was concluded that 2 weeks of CS treatment could facilitate the observation of deep fluorescent proteins, given our sample conditions. However, 4 weeks are needed to observe clearer images that completely exclude the auto-fluorescent materials.
Structures with strong autofluorescence, such as vascular bundles and multi-arm cells, cannot be cleared in the CS. To observe these structures without autofluorescence, it is necessary to use a time-gating method12 or to obtain images by spectroscopy of the fluorescence spectrum. A two-photon microscope may be more suitable for observing deeper tissues if thicker tissues are observed.
Significance of the method with respect to existing and alternative methods 
Generally, the internal structures of rice plants have been observed using either cryostat or vibratome sectioning. A cryostat is suitable for preparing thin sections, which allow easier observation, but the preparation of the samples and the operation of the equipment are time-consuming. Reconstructing the original 3D structure from thin sections is also difficult. The vibratome is relatively easy to operate and suitable for producing thick sections. However, thick sections of target tissues only allow observations of the cut surface and not deep tissues that light cannot reach. For these reasons, neither method is suitable for deep fluorescence observations.
This study addressed challenges in deep fluorescence observation in rice shoots, such as the limited tissue penetration of the CS and the poor object resolution under a confocal microscope, by combining existing methods. As shown in Figure 4, we observed fluorescent proteins (OsMADS15-mOrange) expressed in the deep tissues of adult rice shoots from the young panicle to the base. Figure 4D focuses on the floret and shows deep fluorescent proteins at 3 &#181;m intervals. Tissues over &#8722;130 &#181;m depth were observed after 2 weeks of CS treatment, but only the tissues within &#8722;27 &#181;m depth were observed (data not shown) in the floret at the same size and growth stage without CS treatment. The current improved protocol allowed observation not only of overexpression of genes but also natural gene expression in the deep tissues of adult rice shoots.
Importance and potential applications of the method in specific research areas 
This protocol, which optimizes the deep fluorescence observation of adult rice shoots, enables the efficient clearing of hard, thick, or layered tissues by trimming off unnecessary tissues and increasing the permeability of the CS. In addition, the thickness of the samples for analysis was optimized to allow continuous and structural deep fluorescence observation using a confocal laser microscope, which normally cannot resolve thick or opaque tissues.
It is difficult to compare rice samples at different growth stages because the fluorescent proteins degrade over time in the fixative and PBS solutions. However, the fluorescent proteins in the CS can be stored for more than 5 months1. The long shelf life of the CS is a major advantage for deep fluorescence observation in rice.
Recently, many clearing technologies have been developed, making it possible to observe deep tissues in 3D while preserving their internal structures. These technologies have continued to evolve, and new clearing solutions have been developed. A good example is iTOMEI14, which enables efficient chlorophyll removal and brighter fluorescence detection. Another example is ClearSeeAlpha15, which prevents the browning of tissues during clearing treatment and makes them appear transparent. Combining these clearing solutions with the present method may allow more efficient and effective clearing.
It is expected that the current method will help gain new insights through deep imaging of not only rice but also other plants.

Recently developed clearing technology has made it possible to observe the deep tissues of plants while preserving their internal structure1,2,3. In the dicot model plant Arabidopsis, many studies on fluorescent protein imaging have been conducted using clearing technology to eliminate refractive index mismatches and remove auto-fluorescent materials4,5,6. Although the use of clearing technology7,8 and 3D imaging at cellular resolution9 have been reported in rice (Oryza sativa L.), a monocot model plant and a globally important crop, these are limited to relatively thin and soft organs, such as roots, leaves, and shoot apical meristem (SAM), which are easy to observe.
The shoot is the main organ constituting the aboveground parts of vascular plants. In rice, shoots are composed of a series of vertically stacked &#34;phytomers,&#34; comprising axillary buds, leaves, and the stem10. At the tip of the shoot, the SAM is composed of undifferentiated stem cells in the center. Phytomers are formed by the differentiation of cells derived from the SAM. After the plants shift from the vegetative to the reproductive phase, rice stems elongate and the SAM differentiates into young panicles10. This developmental change is accompanied by fluctuations in the expression of various genes in the stems and SAM/young panicles. To understand the mechanisms underlying cell differentiation into various tissues, it is important to structurally observe the cell morphology and gene expression in internal shoot tissues. However, the deep imaging of stems (nodes and internodes) in the shoot presents a challenge because of the inefficiency of clearing solutions to penetrate the tissue. Stems immediately undergo a rapid volume increase from lateral growth after differentiation from the SAM. The hardening of the rice node tissues due to the thickening of the vascular bundles and the horizontal complex link of the nodal vascular anastomosis, in addition to the high repellency of rice shoots, all contribute to limiting the penetration of the CS in stems10.
This study aimed to observe changes in gene expression in rice shoot tissues using a structural deep fluorescence technique. This work optimizes a clearing protocol for rice to continuously observe gene expression from the SAM/young panicle to the base in a 3D structure, rather than on a flat surface, using a confocal laser microscope.

<table><tbody><tr><td>1.5 mL microcentrifuge tube</td><td>BIO-BIK</td><td>ST-0150F</td><td></td></tr><tr><td>12-multiwell plate</td><td>Corning</td><td>353043</td><td></td></tr><tr><td>50 mL conical tube</td><td>Corning</td><td>352070</td><td></td></tr><tr><td>Calcofluor white solution</td><td>Sigma-Aldrich</td><td>910090</td><td></td></tr><tr><td>ClearSee</td><td>FUJIFILM Wako Pure Chemical</td><td>031-25151</td><td>This can be made or purchased.</td></tr><tr><td>Confocal laser microscope</td><td>Carl Zeiss</td><td>LSM700</td><td></td></tr><tr><td>Desiccator</td><td>SANPLATEC</td><td></td><td>Custom made of acrylic. 30 cm (L), 30 cm (W), 14.5 cm (H)</td></tr><tr><td>Glass coverslip (18 &amp;times; 18 No.1)</td><td>MATSUNAMI</td><td>C018181</td><td></td></tr><tr><td>HEPES</td><td>FUJIFILM Wako Pure Chemical</td><td>342-01375</td><td></td></tr><tr><td>Microscope slide (76 &amp;times; 26)</td><td>MATSUNAMI</td><td>S2441</td><td></td></tr><tr><td>Paraffin film</td><td>Bemis</td><td>PM-996</td><td></td></tr><tr><td>Paraformaldehyde</td><td>FUJIFILM Wako Pure Chemical</td><td>162-16065</td><td></td></tr><tr><td>Sodium deoxycholate</td><td>Tokyo Chemical Industry</td><td>C0316</td><td></td></tr><tr><td>Sucrose</td><td>FUJIFILM Wako Pure Chemical</td><td>190-00013</td><td></td></tr><tr><td>UBQpro::NLS-sGFP-nClover3-mNeonGreen (&lt;em&gt;UBQpro::NGCN&lt;/em&gt;)</td><td>provided by Dr. Kurihara</td><td></td><td></td></tr><tr><td>Urea</td><td>FUJIFILM Wako Pure Chemical</td><td>211-01213</td><td></td></tr><tr><td>Vacuum pump</td><td>AS One</td><td>AS-01</td><td></td></tr><tr><td>Vibrating micro-slicer</td><td>DOSAKA</td><td>DTK-3000</td><td></td></tr><tr><td>Xylitol</td><td>FUJIFILM Wako Pure Chemical</td><td>248-00545</td><td></td></tr></tbody></table>

deep fluorescence observation in rice shoots via clearing technology

The recently developed clearing technology that eliminates refractive index mismatches and diminishes auto-fluorescent material has made it possible to observe plant tissues in three dimensions (3D) while preserving their internal structures. In rice (Oryza sativa L.), a monocot model plant and a globally important crop, clearing technology has been reported in organs that are relatively easy to observe, such as the roots and leaves. Applications of clearing technology in shoot apical meristem (SAM) and stems have also been reported, but only to a limited degree because of the poor penetration of the clearing solution (CS) in these tissues. The limited efficiency of the clearing solutions in these tissues has been attributed to auto-fluorescence, thickening, and hardening of the tissues in the stem as the vascular bundles and epidermis develop and layering of the SAM with water-repellent leaves. The present protocol reports the optimization of a clearing approach for continuous and 3D observation of gene expression from the SAM/young panicle to the base of the shoots during development. Fixed tissue samples expressing a fluorescent protein reporter were trimmed into sections using a vibrating micro-slicer. When an appropriate thickness was achieved, the CS was applied. By specifically targeting the central tissue, the penetration rate and uniformity of the CS increased, and the time required to make the tissue transparent decreased. Additionally, clearing of the trimmed sections enabled the observation of the internal structure of the whole shoot from a macro perspective. This method has potential applications in deep imaging of tissues of other plant species that are difficult to clear.

First, the extent to which the hard and thick tissues of adult rice plants could be made transparent by the clearing treatment was validated. Nip at the 9-10 LS, which is the panicle formation stage, and 12-16 mm long tissues cut out from the young panicle to the base of the shoot were used. These samples, including the young panicle, were fixed in the fixative solution and observed before and after 1-4 weeks of the clearing treatment (Figure 2). The untrimmed samples remained green and did not become transparent after 4 weeks or even after 3 months of treatment with the clearing solution (Figure 2A). In samples that were peeled off all leaves, the internodes&#160;turned white&#160;after 1 week of treatment with the CS, although the nodes remained green. This sample did not become transparent after 4 weeks (Figure 2B). After 3 months of the treatment with the CS, only the young panicle became transparent. The hand-trimmed samples changed to white, except for the outer leaves and vascular bundles, after 1 week of treatment with the CS. Some parts of the leaves, young panicle, and internodes became translucent but did not become transparent after 4 weeks (Figure 2C). After 3 months, only the young panicle and inner leaves became transparent. The samples that were trimmed to 130 &#181;m thickness with the vibrating micro-slicer became translucent after 1 week of treatment with the CS, with the leaves turning transparent. After 2 weeks, the sample was almost transparent and remained unchanged after 4 weeks (Figure 2D). After 3 months, the samples became completely transparent.
Next, the depth by which the clearing treatment allowed gene expression observations in the shoot of T65 at the 8 LS was validated. The UBQpro::NLS-sGFP-nClover3-mNeonGreen (UBQpro::NGCN, see Table of Materials) expressed shoots were used. Tissue samples were fixed in the fixative solution before trimming them to 130 &#181;m thickness using a vibrating micro-slicer. The samples were then observed under a confocal laser microscope (laser: 488 nm/13%, objective: 20x, pinhole: 0.93 AU, averaging: 16, detector gain: 800) at 10 &#181;m intervals in the z-axis direction every week from 0-4 weeks of treatment with the CS. The representative results are shown in Figure 3. All figures were adjusted with the same processing to compare the fluorescence intensity. In the node without the treatment, faint fluorescent signals were observed at a depth of &#8722;40 &#181;m (Figure 3A). The observable depth was &#8722;60 &#181;m after 1 week of the CS treatment and &#8722;90 &#181;m after 2 weeks, but auto-fluorescence of the cytoplasm was noticeable at both weeks at a depth of &#8722;20 &#181;m. The autofluorescence became somewhat weaker after 3 weeks and was no longer visible after 4 weeks. Fluorescent signals were observed at a depth of &#8722;80 &#181;m at 3 weeks and at a depth of &#8722;100 &#181;m at 4 weeks. In the internode, fluorescent signals were observed at a depth of &#8722;60 &#181;m without the CS treatment (Figure 3B). The observable depth was &#8722;90 &#181;m after 1 week to 3 weeks of the CS treatment and &#8722;100 &#181;m after 4 weeks, but auto-fluorescence in the cytoplasm was noticeable at a depth of &#8722;20 &#181;m after 1 week. Auto-fluorescence was no longer visible after 2 weeks. In the leaves, fluorescent signals were observed at a depth of &#8722;90 &#181;m without the CS treatment (Figure 3C). The fluorescent signals were observed deeper in the leaves than in the nodes and internodes. However, the fluorescent signals were weaker. The fluorescent signals became clear after 1 week of CS treatment and were observed at a depth of &#8722;120 &#181;m. After 2 weeks and 3 weeks, fluorescent signals were observed at a depth of &#8722;110 &#181;m and, after 4 weeks, at a depth of &#8722;120 &#181;m.
Finally, the expression of the transcription factor OsMADS1511 fused with mOrange12 was observed, which regulates the transition of SAM from the vegetative to the reproductive phase13. Tissue samples from Nip at the 10 LS with OsMADS15-mOrange were fixed, trimmed to 130 &#181;m thickness, and treated with the CS for 2 weeks. Figure 4 shows that the clearing solution could be used simultaneously to observe the fluorescent proteins (OsMADS15-mOrange) of natural gene expression and fluorescent dye staining (calcofluor white). The whole floret at depths from 0 to &#8722;130 &#181;m was observed, and the 3D image was reconstructed from 43 z-stack images at 3 &#181;m intervals (Figure 4E).
<img alt="Figure 1" class="xfigimg" src="/files/ftp_upload/64116/64116fig01.jpg" /> 
Figure 1: Sampling position and processing. (A) Nip seedling at the 8 LS under the short-day condition. (B) Enlarged view of the base. (C) A sample cut-out from the SAM/young panicle to the base. (D) An oval cross-section from C (inset). (E) Thinly shaving off one side of the shoot with a blade. (F) Thinly shaved surface. (G) Sample showing internode elongation. The whitish section indicated by the arrowheads is nodes. The upper side of the upper node has the young panicle. Scale bars: (A) 10 cm, (B-C,E-G) 1 cm, (D) 0.5 cm. <a href="https://www.jove.com/files/ftp_upload/64116/64116fig01large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 2" class="xfigimg" src="/files/ftp_upload/64116/64116fig02.jpg" /> 
Figure 2: Tissue clearing depends on the sample thickness and CS treatment period. (A) Untrimmed samples with partial shoots including the young panicle. Maximum thickness: 4 mm. (B) All leaves peeled off from the samples to expose the young panicle. Maximum thickness: 2.5 mm. yp: young panicle, in: internode; arrowheads indicate node. (C) Samples that were hand-trimmed to 1 mm thickness. (D) Samples trimmed with the vibrating micro-slicer to 130 &#181;m thickness. Scale bar: 5 mm. <a href="https://www.jove.com/files/ftp_upload/64116/64116fig02large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 3" class="xfigimg" src="/files/ftp_upload/64116/64116fig03.jpg" /> 
Figure 3: The depth of fluorescence observation depends on the tissue type and CS treatment period. Deep imaging of UBQpro::NGCN in the (A) node, (B) internode, and (C) leaf. &#34;Merge&#34; means the images were fused with the differential interference contrast (DIC) image and all z-stack images. Images in which no fluorescence was observed were marked as &#34;n.d.&#34; (not detected). Settings of the confocal laser microscopy are as follows: laser: 488 nm/13%, objective: 20x, pinhole: 0.93 AU, averaging: 16, detector gain: 800, interval: 10 &#181;m. Scale bars: 50 &#181;m. <a href="https://www.jove.com/files/ftp_upload/64116/64116fig03large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 4" class="xfigimg" src="/files/ftp_upload/64116/64116fig04.jpg" /> 
Figure 4: Deep fluorescence observation of OsMADS15-mOrange. (A) The DIC image of Nip at the 10 LS. yp: young panicle, le: leaf, no: node, in: internode; arrowheads indicate florets. (B) Fluorescence image of OsMADS15-mOrange. Yellow dots indicate the fluorescent proteins of OsMADS15-mOrange at the nucleus. The cell wall was stained cyan with the calcofluor white solution. (C) Enlarged view of the young panicle. (D) Deep imaging of the floret. pa: palea, le: lemma, fm: floral meristem; asterisks indicate stamen primordia. The confocal laser microscope was set as follows: OsMADS15-mOrange; laser: 555 nm/13%, objective: 20x, pinhole: 0.96 AU, averaging: 16, detector gain: 800, interval: 3 &#181;m. Calcofluor white; laser: 405 nm/3%, objective: 20x, pinhole: 0.93 AU, averaging: 16, detector gain: 470, interval: 3 &#181;m. (E) The 3D image of the figure (D) constructed from the z-stack images. Scale bars: (A-B) 1 mm, (C) 500 &#181;m, (D) 40 &#181;m. <a href="https://www.jove.com/files/ftp_upload/64116/64116fig04large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>

Watch this Scientific Journal Video about Deep Fluorescence Observation in Rice Shoots via Clearing Technology at JoVE.com

Deep Fluorescence Observation in Rice Shoots via Clearing Technology

The present protocol describes a clearing technique for rice shoots, which are difficult to prepare for internal structural observations owing to the hard, thick, or layered nature of the tissues. This method facilitates continuous and deep fluorescence observations, even in adult rice plants.

Deep Fluorescence Observation in Rice Shoots via Clearing Technology

The recently developed clearing technology that eliminates refractive index mismatches and diminishes auto-fluorescent material has made it possible to ...

deep-fluorescence-observation-in-rice-shoots-via-clearing-technology

Research

JoVE Journal

Biology

2.8K Views.  Nagoya University. Deze methode pakt de uitdagingen aan in Deep Fluorescence Observation in Rice Shoots, zoals een beperkte weefselpenetratie van de clearingoplossing en de echte resolutie onder confocale microscoop. Het belangrijkste voordeel van deze techniek is een structuurobservatie van veel grote weefsels vanuit een macroperspectief, zelfs prompts met harde en dikke weefsels, zoals volwassen scheuten. Deze methode is van toepassing op diepe beeldvorming van harde en dikke weefsels bij brede plantensoorten...

Video: Deep Fluorescence Observation in Rice Shoots via Clearing Technology

Multiphoton Microscopy of Cleared Mouse Brain Expressing YFP

Multiphoton microscopy of intrinsic fluorescence and second harmonic generation (SHG) of whole mouse organs is made possible by optically clearing the organ before imaging.1,2 However, for organs that contain fluorescent proteins such as GFP and YFP, optical clearing protocols that use methanol dehydration and clear using benzyl alcohol:benzyl benzoate (BABB) while unprotected from light3 do not preserve the fluorescent signal. The protocol presented here is a novel way in which to perform whole organ optical clearing on mouse brain while preserving the fluorescence signal of YFP expressed in neurons. Altering the optical clearing protocol such that the organ is dehydrated using an ethanol graded series has been found to reduce the damage to the fluorescent proteins and preserve their fluorescent signal for multiphoton imaging.4 Using an optimized method of optical clearing with ethanol-based dehydration and clearing by BABB while shielded from light, we show high-resolution multiphoton images of yellow fluorescent protein (YFP) expression in the neurons of a mouse brain more than 2 mm beneath the tissue surface.

Multiphoton microscopy of whole mouse organs is possible by optically clearing the organ before imaging, but not all protocols preserve the fluorescent signal of fluorescent proteins. Using an optical clearing method with ethanol-based dehydration and benzyl alcohol:benzyl benzoate clearing, we show high-resolution multiphoton images of whole mouse brain expressing YFP.

Multiphoton microscopy of intrinsic fluorescence and second harmonic generation (SHG) of whole mouse organs is made possible by optically clearing the ...

Neuroscience

Whole-mount Clearing and Staining of Arabidopsis Flower Organs and Siliques

Due to its formidable tools for molecular genetic studies, Arabidopsis thaliana is one of the most prominent model species in plant biology and, especially, in plant reproductive biology. However, plant morphological, anatomical, and ultrastructural analyses traditionally involve time-consuming embedding and sectioning procedures for bright field, scanning, and electron microscopy. Recent progress in confocal fluorescence microscopy, state-of-the-art 3-D computer-aided microscopic analyses, and the continuous refinement of molecular techniques to be used on minimally processed whole-mount specimens, has led to an increased demand for developing efficient and minimal sample processing techniques. In this protocol, we describe techniques for properly dissecting Arabidopsis flowers and siliques, basic clearing techniques, and some staining procedures for whole-mount observations of reproductive structures.

Whole-mount Clearing and Staining of Arabidopsis Flower Organs and Siliques

In this protocol, we describe techniques for the proper dissection of Arabidopsis flowers and siliques, some basic clearing techniques, and selected staining procedures for whole-mount observations of reproductive structures.

Due to its formidable tools for molecular genetic studies, Arabidopsis thaliana is one of the most prominent model species in plant biology and, ...

Developmental Biology

Transverse Sectioning of Mature Rice (Oryza sativa L.) Kernels for Scanning Electron Microscopy Imaging Using Pipette Tips as Immobilization Support

Starch granules (SGs) exhibit different morphologies depending on the plant species, especially in the endosperm of the Poaceae family. Endosperm phenotyping can be used to classify genotypes based on SG morphotype using scanning electron microscopic (SEM) analysis. SGs can be visualized using SEM by slicing through the kernel (pericarp, aleurone layers, and endosperm) and exposing the organellar contents. Current methods require the rice kernel to be embedded in plastic resin and sectioned using a microtome or embedded in a truncated pipette tip and sectioned by hand using a razor blade. The former method requires specialized equipment and is time-consuming, while the latter introduces a new host of problems depending on rice genotype. Chalky rice varieties, particularly, pose a problem for this type of sectioning due to the friable nature of their endosperm tissue. Presented here is a technique for preparing translucent and chalky rice kernel sections for microscopy, requiring only pipette tips and a scalpel blade. Preparing the sections within the confines of a pipette tip prevents rice kernel endosperm from shattering (for translucent or &#8216;vitreous&#8217; phenotypes) and crumbling (for chalky phenotypes). Using this technique, endosperm cell patterning and the structure of intact SGs can be observed.

Transverse Sectioning of Mature Rice Oryza sativa L. Kernels for Scanning Electron Microscopy Imaging Using Pipette Tips as Immobilization Support

This protocol allows for the preparation of transverse sections of cereal seeds (e.g., rice) for the analysis of endosperm and starch granule morphology using scanning electron microscopy.

Starch granules (SGs) exhibit different morphologies depending on the plant species, especially in the endosperm of the Poaceae family. Endosperm ...

Biochemistry

Rapid Optical Clearing for Semi-High-Throughput Analysis of Tumor Spheroids

Tumor spheroids are fast becoming commonplace in basic cancer research and drug development. Obtaining data regarding protein expression within the spheroid at the cellular level is important for analysis, yet existing techniques are often expensive, laborious, use non-standard equipment, cause significant size distortion, or are limited to relatively small spheroids. This protocol presents a new method of mounting and clearing spheroids that address these issues while allowing for confocal analysis of the inner structure of spheroids. In contrast to existing approaches, this protocol provides for rapid mounting and clearing of a large number of spheroids using standard equipment and laboratory supplies. Mounting spheroids in a pH-neutral agarose-PBS gel solution before introducing a refractive-index-matched clearing solution minimizes size distortion common to other similar techniques. This allows for detailed quantitative and statistical analysis where the accuracy of size measurements is paramount. Furthermore, compared to liquid clearing solutions, the agarose gel technique keeps spheroids fixed in place, allowing for the collection of three-dimensional (3D) confocal images. The present article elaborates how the method yields high-quality two- and 3D images that provide information about inter-cell variability and inner spheroid structure.

Tumor spheroids are becoming increasingly utilized to assess tumor cell-microenvironment interactions and therapy response. The present protocol describes a robust but simple method for semi-high-throughput imaging of 3D tumor spheroids using rapid optical clearing.

Tumor spheroids are fast becoming commonplace in basic cancer research and drug development. Obtaining data regarding protein expression within the ...

Cancer Research

Visualizing Early Infection Sites of Rice Blast Disease (Magnaporthe oryzae) on Barley (Hordeum vulgare) Using a Basic Microscope and a Smartphone

Understanding how plants and pathogens interact, and whether that interaction culminates in defense or disease, is required to develop stronger and more sustainable strategies for plant health. Advances in methods that more effectively image plant-pathogen samples during infection and colonization have yielded tools such as the rice leaf sheath assay, which has been useful in monitoring infection and early colonization events between rice and the fungal pathogen, Magnaporthe oryzae. This hemi-biotrophic pathogen causes severe disease loss in rice and related monocots, including millet, rye, barley, and more recently, wheat. The leaf sheath assay, when performed correctly, yields an optically clear plant section, several layers thick, which allows researchers to perform live-cell imaging during pathogen attack or generate fixed samples stained for specific features. Detailed cellular investigations into the barley-M. oryzae interaction have lagged behind those of the rice host, in spite of the growing importance of this grain as a food source for animals and humans and as fermented beverages. Reported here is the development of a barley leaf sheath assay for intricate studies of M. oryzae interactions during the first 48 h post-inoculation. The leaf sheath assay, regardless of which species is being studied, is delicate; provided is a protocol that covers everything, from barley growth conditions and obtaining a leaf sheath, to inoculation, incubation, and imaging of the pathogen on plant leaves. This protocol can be optimized for high-throughput screening using something as simple as a smartphone for imaging purposes.

Visualizing Early Infection Sites of Rice Blast Disease Magnaporthe oryzae on Barley Hordeum vulgare Using a Basic Microscope and a Smartphone

This is a straightforward protocol of a barley leaf sheath assay using minimal reagents and common laboratory equipment (including a basic smartphone). The purpose is to visualize the early infection process of blast disease in labs without access to advanced microscopy equipment.

Understanding how plants and pathogens interact, and whether that interaction culminates in defense or disease, is required to develop stronger and more ...

A Simple Method for Imaging Arabidopsis Leaves Using Perfluorodecalin as an Infiltrative Imaging Medium

The problem of acquiring high-resolution images deep into biological samples is widely acknowledged1. In air-filled tissue such as the spongy mesophyll of plant leaves or vertebrate lungs further difficulties arise from multiple transitions in refractive index between cellular components, between cells and airspaces and between the biological tissue and the rest of the optical system. Moreover, refractive index mismatches lead to attenuation of fluorophore excitation and signal emission in fluorescence microscopy. We describe here the application of the perfluorocarbon, perfluorodecalin (PFD), as an infiltrative imaging medium which optically improves laser scanning confocal microscopy (LSCM) sample imaging at depth, without resorting to damaging increases in laser power and has minimal physiological impact2. We describe the protocol for use of PFD with Arabidopsis thaliana leaf tissue, which is optically complex as a result of its structure (Figure 1). PFD has a number of attributes that make it suitable for this use3. The refractive index of PFD (1.313) is comparable with that of water (1.333) and is closer to that of cytosol (approx. 1.4) than air (1.000). In addition, PFD is readily available, non-fluorescent and is non-toxic. The low surface tension of PFD (19 dynes cm-1) is lower than that of water (72 dynes cm-1) and also below the limit (25 - 30 dyne cm-1) for stomatal penetration4, which allows it to flood the spongy mesophyll airspaces without the application of a potentially destructive vacuum or surfactant. Finally and crucially, PFD has a great capacity for dissolving CO2 and O2, which allows gas exchange to be maintained in the flooded tissue, thus minimizing the physiological impact on the sample. These properties have been used in various applications which include partial liquid breathing and lung inflation5,6, surgery7, artificial blood8, oxygenation of growth media9, and studies of ice crystal formation in plants10. Currently, it is common to mount tissue in water or aqueous buffer for live confocal imaging. We consider that the use of PFD as a mounting medium represents an improvement on existing practice and allows the simple preparation of live whole leaf samples for imaging.

A Simple Method for Imaging Arabidopsis Leaves Using Perfluorodecalin as an Infiltrative Imaging Medium

We describe the use of perfluorodecalin as an infiltrative mounting medium. This is a simple method for improving depth of imaging in Arabidopsis thaliana leaf tissue with minimal physiological impact.

The problem of acquiring high-resolution images deep into biological samples is widely acknowledged1. In air-filled tissue such as the spongy mesophyll of ...

Agrobacterium-Mediated Genetic Transformation, Transgenic Production, and Its Application for the Study of Male Reproductive Development in Rice

Male sterility is an important agronomic trait for hybrid seed production that is usually characterized by functional defects in male reproductive organs/gametes. Recent advances in CRISPR-Cas9 genome editing technology allow for high editing efficacy and timesaving knockout mutations of endogenous candidate genes at specific sites. Additionally, Agrobacterium-mediated genetic transformation of rice is also a key method for gene modification, which has been widely adopted by many public and private laboratories. In this study, we applied CRISPR-Cas9 genome editing tools and successfully generated three male sterile mutant lines by targeted genome editing of OsABCG15 in a japonica cultivar. We used a modified Agrobacterium-mediated rice transformation method that could provide excellent means of genetic emasculation for hybrid seed production in rice. Transgenic plants can be obtained within 2&#8211;3 months and homozygous transformants were screened by genotyping using PCR amplification and Sanger sequencing. Basic phenotypic characterization of the male sterile homozygous line was performed by microscopic observation of the rice male reproductive organs, pollen viability analysis by iodine potassium iodide (I2-KI) staining semi-thin cross-sectioning of developing anthers.

Agrobacterium-Mediated Genetic Transformation, Transgenic Production, and Its Application for the Study of Male Reproductive Development in Rice

This work describes the use of CRISPR-Cas9 genome editing technology to knockout endogenous gene OsABCG15 followed by a modified Agrobacterium-mediated transformation protocol to produce a stable male-sterile line in rice.

Male sterility is an important agronomic trait for hybrid seed production that is usually characterized by functional defects in male reproductive ...

Optical Clearing of Plant Tissues for Fluorescence Imaging

It is challenging to directly observe the internal structure of multi-layered and opaque plant specimens, without dissection, under a microscope. In addition, autofluorescence attributed to chlorophyll hampers the observation of fluorescent proteins in plants. For a long time, various clearing reagents have been used to make plants transparent. However, conventional clearing reagents diminish fluorescent signals; therefore, it has not been possible to observe the cellular and intracellular structures with fluorescent proteins. Reagents were developed that can clear plant tissues by removing chlorophyll while maintaining fluorescent protein stability. A detailed protocol is provided here for the optical clearing of plant tissues using clearing reagents, ClearSee (CS) or ClearSeeAlpha (CSA). The preparation of cleared plant tissues involves three steps: fixation, washing, and clearing. Fixation is a crucial step in maintaining the cellular structures and intracellular stability of fluorescent proteins. The incubation time for clearing depends on the tissue type and species. In Arabidopsis thaliana, the time required for clearing with CS was 4 days for leaves and roots, 7 days for seedlings, and 1 month for pistils. CS also required a relatively short time of 4 days to make the gametophytic leaves of Physcomitrium patens transparent. In contrast, pistils in tobacco and torenia produced brown pigment due to oxidation during CS treatment. CSA reduced the brown pigment by preventing oxidation and could make tobacco and torenia pistils transparent, although it took a relatively long time (1 or 2 months). CS and CSA were also compatible with staining using chemical dyes, such as DAPI (4',6-diamidino-2-phenylindole) and Hoechst 33342 for DNA and Calcofluor White, SR2200, and Direct Red 23 for the cell wall. This method can be useful for whole-plant imaging to reveal intact morphology, developmental processes, plant-microbe interactions, and nematode infections.

Here, a method is described for making plant tissues transparent while maintaining the stability of fluorescent proteins. This technique facilitates deep imaging of cleared plant tissues without physical sectioning.

It is challenging to directly observe the internal structure of multi-layered and opaque plant specimens, without dissection, under a microscope. In ...

Combining Clearing and Fluorescence Microscopy for Visualising Changes in Gene Expression and Physiological Responses to Plasmodiophora brassicae

Infection of Brassica crops by the soilborne protist Plasmodiophora brassicae leads to gall formation on the underground organs. The formation of galls requires cellular reprogramming and changes in the metabolism of the infected plant. This is necessary to establish a pathogen-oriented physiological sink toward which the host nutrients are redirected. For a complete understanding of this particular plant-pathogen interaction and the mechanisms by which host growth and development are subverted and repatterned, it is essential to track and observe the internal changes accompanying gall formation with cellular resolution. Methods combining fluorescent stains and fluorescent proteins are often employed to study anatomical and physiological responses in plants. Unfortunately, the large size of galls and their low transparency act as major hurdles in performing whole-mount observations under the microscope. Moreover, low transparency limits the employment of fluorescence microscopy to study clubroot disease progression and gall formation. This article presents an optimized method for fixing and clearing galls to facilitate epifluorescence and confocal microscopy for inspecting P. brassicae-infected galls. A tissue-clearing protocol for rapid optical clearing was used followed by vibratome sectioning to detect anatomical changes and localize gene expression with promoter fusions and reporter lines tagged with fluorescent proteins. This method will prove useful for studying cellular and physiological responses in other pathogen-triggered structures in plants, such as nematode-induced syncytia and root knots, as well as leaf galls and deformations caused by insects.

Combining Clearing and Fluorescence Microscopy for Visualising Changes in Gene Expression and Physiological Responses to Plasmodiophora brassicae

The present protocol describes an optimized method for the histological observation of galls induced by Plasmodiophora brassicae. Vibratome sections of hypocotyls are cleared before fluorescence imaging to study the involvement of transcription factors and phytohormones during disease progression. This protocol overcomes resin embedding limitations, enabling in planta visualization of fluorescent proteins.

Infection of Brassica crops by the soilborne protist Plasmodiophora brassicae leads to gall formation on the underground organs. The formation of galls ...

Real-Time Detection of Reactive Oxygen Species Production in Immune Response in Rice with a Chemiluminescence Assay

Reactive oxygen species (ROS) play vital roles in a variety of biological processes, including the sensing of abiotic and biotic stresses. Upon pathogen infection or challenge with pathogen-associated chemicals (pathogen-associated molecular patterns [PAMPs]), an array of immune responses, including a ROS burst, are quickly induced in plants, which is called PAMP-triggered immunity (PTI). A ROS burst is a hallmark PTI response, which is catalyzed by a group of plasma membrane-localized NADPH oxidases-the RBOH family proteins. The vast majority of ROS comprise hydrogen peroxide (H2O2), which can be easily and steadily detected by a luminol-based chemiluminescence method. Chemiluminescence is a photon-producing reaction in which luminol, or its derivative (such as L-012), undergoes a redox reaction with ROS under the action of a catalyst. This paper describes an optimized L-012-based chemiluminescence method to detect apoplast ROS production in real-time upon PAMP elicitation in rice tissues. The method is easy, steady, standardized, and highly reproducible under firmly controlled conditions.

Here, we describe a method for the real-time detection of apoplastic reactive oxygen species (ROS) production in rice tissues in pathogen-associated molecular pattern-triggered immune response. This method is simple, standardized, and generates highly reproducible results under controlled conditions.

Reactive oxygen species (ROS) play vital roles in a variety of biological processes, including the sensing of abiotic and biotic stresses. Upon pathogen ...

Deep Fluorescence Observation in Rice Shoots via Clearing Technology

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