This work was supported by a grant to PJ from the Biotechnology and Biological Sciences Research Council (BBSRC; grant ref. BB/K018442/1).

1. Growth of Arabidopsis Plants and the Stress Treatment
<ol>
	<li>Prepare 1 L of Murashige and Skoog (MS) medium by adding 4.3 g of MS Basal Salt Mixture, 10 g sucrose, 0.5 g 2-(N-morpholino) ethane sulfonic acid (MES) to deionized water up to 1 L, and adjust the pH to 5.7 with potassium hydroxide (KOH). Add 6 g of phytoagar and autoclave for 20 min at 120 &#176;C.
	<ol>
		<li>Before solidification, pour the medium into round Petri plates (diameter 9 cm, height 1.5 cm, with 20 - 25 mL MS medium per plate). Allow the plates to dry for ~1 h in a laminar flow hood before closing the lids.</li>
	</ol>
	</li>
	<li>Place Arabidopsis thaliana seeds into a 1.5 mL test tube for surface sterilization by adding 1 mL of 70% (v/v) ethanol containing 0.02% (v/v) Triton X-100 and continuously shaking for 5-10 min. For each genotype/condition, prepare 10 Petri plates each carrying ~100 - 150 seedlings.</li>
	<li>Wait for about 10 s&#160;until the seeds settle to the bottom of the tube, and then discard the supernatant by pipetting. Add 1 mL of 100% ethanol, and shake the tube again for 10 min.</li>
	<li>Prepare the laminar flow hood while the seeds are sterilizing. Take one piece of filter paper per sample, fold it in half to facilitate sowing, and soak it in 100% ethanol in the hood. Wait until it dries out completely. Note that 100% ethanol is used as it evaporates more quickly than 70% ethanol.</li>
	<li>Transfer the seeds onto the filter paper by pipetting using a 1 mL pipette tip cut ~5 mm from the fine end. Allow them to dry, which should take about 10 - 15 min.</li>
	<li>Sow ~100 - 150 sterilized seeds evenly onto each MS medium Petri plate, and seal each plate with surgical tape.</li>
	<li>Store the plates upside down at 4 &#176;C for 2 - 4 d&#160;to encourage and synchronize germination. Old seeds may need to stay longer (up to a week) at 4 &#176;C.</li>
	<li>Transfer the plates to a plant tissue culture chamber and leave them upside up. Grow the plants for 8 d&#160;under a long-day cycle (16 h&#160;100 &#181;mol&#183;m&#8722;2&#183;s&#8722;1 light, 8 h&#160;dark) at 20 &#176;C.</li>
	<li>For stress treatment, when the plants are 8 d&#160;old, in the flow hood, transfer them from the agar medium, by gently scraping them off by hand wearing ethanol-sterilized gloves, into a sterilized flask of liquid MS medium containing the stressor (e.g., 200 mM mannitol). Avoid carrying over agar medium. Cover the flask mouth with sterilized foil and allow the plants to grow under the same conditions as in step 1.8 for an additional 2 d&#160;on an orbital shaker with gentle shaking (~100 rpm).</li>
</ol>
2. Making a Precursor Protein by In Vitro&#160;Transcription/Translation
Note: This protocol assumes the use of Arabidopsis photosystem I subunit D precursor (pPsaD) as the template/preprotein, but the method is compatible with others.
<ol>
	<li>Clone the coding sequence (CDS) of pPsaD into the multiple cloning site (MCS) of the pBlueScript II SK vector (or any other similar vector with an upstream T7 promoter) 13. Purify the plasmid (pBSK-pPsaD) using a DNA isolation kit and verify the sequence by DNA sequencing. 
	NOTE: All these steps employ standard molecular cloning techniques.</li>
	<li>Determine the pBSK-pPsaD plasmid DNA concentration using a spectrophotometer set to measure absorbance at 260 nm. Dilute the plasmid to a final concentration of 10 ng/&#181;L.</li>
	<li>Run a 20 &#181;L PCR (for 35 cycles) using the diluted plasmid as template. Prepare the reaction as follows: 2 &#181;L 10&#215; polymerase buffer, 2 &#181;L 2 mM dNTPs, 1 &#181;L 5 mM M13 forward primer (5&#39;-TGT AAA ACG ACG GCC AGT-3&#39;), 1 &#181;L 5 mM M13 reverse primer (5&#39;-CAG GAA ACA GCT ATG ACC-3&#39;), 1 &#181;L diluted pBSK-pPsaD plasmid, 1 U Taq polymerase, and distilled water to make the total reaction volume up to 20 &#181;L. Use a standard PCR program, as follows: 95 &#176;C, 5 min; 35 cycles of [95 &#176;C, 30 sec; 56 &#176;C, 30 sec; 72 &#176;C, 30 sec); and 72 &#176;C, 5 min.</li>
	<li>Run 5 &#181;L of the PCR product on a 1% (w/v) agarose gel in TAE buffer (Tris-HCl, pH 7.6, 20 mM acetic acid, 1 mM EDTA) to verify correct amplification of the cDNA, and quantify the relevant band relative to standards to confirm the concentration. Store the rest of the product at &#8722;20 &#176;C for further applications.</li>
	<li>Prepare a 50 &#181;L reaction using a rabbit reticulocyte lysate based cell-free transcription/translation system compatible with PCR DNA, as follows: 40 &#181;L reticulocyte lysate from the transcription/translation system, 2.5 &#181;L radiolabeled [35S] methionine, 11 &#181;Ci/mL (specific activity: &#62;1,000 Ci/mmol), 2.5 &#181;L sterile distilled water, and 5 &#181;L pPsaD PCR product (100 - 800 ng). 
	Caution: Wear gloves, laboratory clothing and safety glasses when handling radioactive material. Monitor and decontaminate the working surface and equipment. Dispose of all radioactive waste in an approved waste container.</li>
	<li>Incubate the reaction for 90 min in a 30 &#176;C water bath. Stop the reaction by placing the sample on ice.</li>
	<li>Remove 1 &#181;L of the reaction as a test sample (the same volume can also serve as an input control for step 5.7) for verification on standard sodium dodecyl sulfate polyacrylamide gel electrophoresis (SDS-PAGE) followed by autoradiography, fluorography&#160;or phosphor imaging. A good result is indicated by the observation of a distinct and strong band corresponding to the molecular weight of pPsaD (~23 kD). Store the rest of the reaction at &#8722;80 &#176;C for further applications.</li>
</ol>
3. Chloroplast Isolation
<ol>
	<li>Prepare the following stock solutions:
	<ol>
		<li>Prepare Chloroplast Isolation Buffer (CIB, 2x): 0.6 M sorbitol, 10 mM magnesium chloride (MgCl2), 10 mM Ethylene Glycol Tetraacetic Acid (EGTA), 10 mM ethylenediaminetetraacetic acid (EDTA), 20 mM sodium bicarbonate (NaHCO3), 40 mM 4-(2-hydroxyethyl)piperazine-1-ethanesulfonic acid (HEPES); adjust to pH 8.0 with KOH. Prepare 2 L of 2x CIB, make aliquots and keep them at -20 &#176;C for long-term storage, or at 4 &#176;C for short-term storage. To make 1x CIB, dilute the 2x CIB 1:1 with distilled water; this can be prepared freshly on the day of chloroplast isolation experiment.</li>
		<li>Prepare HEPES-MgSO4-Sorbitol buffer (HMS, 1x): 50 mM HEPES, 3 mM magnesium sulfate (MgSO4), 0.3 M sorbitol; adjust to pH 8.0 with sodium hydroxide (NaOH). Prepare 400 mL of buffer, make aliquots and keep them at -20 &#176;C for long-term storage, or at 4 &#176;C for short-term storage.</li>
	</ol>
	</li>
	<li>Conduct all of the following procedures in the cold room or on ice. Precool all of the solutions, devices, equipment, and rotors before starting.</li>
	<li>Prepare a continuous density gradient by mixing 13 mL Percoll, 13 mL 2x CIB buffer, and 5 mg glutathione in a 50 mL centrifuge tube, and centrifuging the mixture at 43,000 &#215; g for 30 min (brake off) at 4 &#176;C. After centrifugation, handle the tube with care to avoid disturbing the gradient and keep it on ice for later use.</li>
	<li>Transfer 100 mL of 1x CIB per genotype/condition to a 1 L beaker.
	<ol>
		<li>Remove the seedlings from the liquid medium by tipping them into a sieve, and transfer them into another CIB-containing beaker; then, rinse the tissue with the CIB to remove any residual liquid medium before replacing it with 100 mL of fresh CIB.</li>
	</ol>
	</li>
	<li>For homogenization, use a total of 100 mL of 1x CIB per sample in five consecutive rounds of homogenization, each round using 20 mL of fresh CIB held in a 50 mL beaker.
	<ol>
		<li>For the first round of homogenization, transfer the plant tissue into the 50 mL beaker by hand, allowing the previous holding buffer to drain through your fingers. Try to use most of the tissue in the first round, but make sure it is immersed with buffer; if this is not possible, introduce the remaining unused tissue at the second round.</li>
	</ol>
	</li>
	<li>Place probe of the tissue homogenizer into the tissue and homogenize with two pulses of 1 - 2 s&#160;each. Filter the homogenate through two layers of filtration cloth into a 250 mL centrifuge tube by gentle squeezing. Retain the filtrate, and transfer the tissue back to the 50 mL beaker.</li>
	<li>Place a second 20 mL CIB aliquot into the 50 mL beaker, adding any remaining tissue not used in the first round of homogenization, and repeat the homogenization and filtration steps. Thus, repeat steps 3.5 and 3.6 until all of the 100 mL of CIB has been used up (i.e., 5 aliquots of 20 mL), and combine the resulting filtrates.</li>
	<li>Centrifuge the pooled homogenate at 1,000 &#215; g for 5 min (brake on) at 4 &#176;C, and pour off the supernatant immediately following completion of the centrifugation, taking care not to disturb the pellet. Resuspend the pellet in the residual supernatant left in the tube by gently agitating the tube on ice. Do not resuspend vigorously by pipetting or vortexing.</li>
	<li>Gently transfer the homogenate onto the top of the premade continuous density gradient, using a Pasteur pipette to apply it via the wall of the receiving tube. Avoid disturbing the gradient. Centrifuge in a swinging-bucket rotor at 7,800 &#215; g for 10 min (brake off) at 4 &#176;C. 
	NOTE: Two green bands can be seen in the gradient after centrifugation: the lower band contains intact chloroplasts, and the upper band contains broken chloroplasts.</li>
	<li>Discard the top band by pipetting, and then transfer the lower band with a Pasteur pipette into a fresh 50 mL centrifuge tube, retaining a volume of up to 8 mL per gradient.</li>
	<li>Add ~25 mL of 1x HMS buffer into the tube and invert the tube twice to wash the Percoll from the chloroplasts. Place the tube again in the swinging-bucket rotor and centrifuge at 1,000 &#215; g for 5 min (brake on) at 4 &#176;C.</li>
	<li>Pour off the supernatant and carefully resuspend the chloroplast pellet in the residual HMS left in the tube by gently agitating the tube on ice. Add an additional 100 - 300 &#181;L of HMS if necessary (based on the size of the pellet and the counting in Section 4), but try not to dilute the sample too much.
	<ol>
		<li>Keep the chloroplasts on ice. Each time before the chloroplasts are used for downstream applications, shake the tube to resuspend them. Always use a cut pipette tip (with an enlarged pore) to transfer the chloroplasts.</li>
	</ol>
	</li>
</ol>
4. Analysis of the Yield and Intactness of Chloroplasts
<ol>
	<li>Add 5 &#181;L of isolated chloroplasts to 495 &#181;L of 1x HMS buffer in a 1.5 mL tube, and then mix gently by inverting the tube to obtain a 1:100 dilution.</li>
	<li>Place a cover glass on top of the counting chamber of the haemocytometer. Slowly pipette ~40 - 60 &#181;L of the diluted chloroplast suspension into the gap between the cover glass and the counting chamber. Using a phase-contrast microscope with a 10X or 20X&#160;objective, intact chloroplasts look round and bright and are surrounded by a halo of light. 
	NOTE: Under the microscope, there is a 1 mm2 counting area with 25 large squares, each containing 16 small squares in the center of the counting chamber.</li>
	<li>Count the number of chloroplasts in 10 large squares. The number of chloroplasts per large square should average between 10 and 30. If too few or too many chloroplasts are present, adjust the dilution factor (step 4.1 above) accordingly, and repeat the procedure.</li>
	<li>Calculate the number of chloroplasts per mL (concentration) as follows: n (the average number of chloroplasts per large square calculated in step 4.3) &#215; 25 (total number of large squares) &#215; 100 (the dilution factor) &#215; 104 (scaling factor to express data per 1 mL, since the volume above the 25 squares is 0.1 mm3).</li>
	<li>Calculate the actual yield of chloroplasts by multiplying the concentration by the volume of chloroplast suspension obtained in step 3.12. Normally, more than 50 &#215; 106 chloroplasts can be obtained.</li>
</ol>
5. Chloroplast Protein Import
<ol>
	<li>Prepare the following stock solutions:
	<ol>
		<li>Prepare 10x HMS buffer: 500 mM HEPES, 30 mM MgSO4, and 3.0 M sorbitol; adjust to pH 8.0 with NaOH. Prepare 50 mL of this buffer, aliquot, and store at &#8722;20 &#176;C for long-term storage and at 4 &#176;C for short-term storage.</li>
		<li>Prepare Import stop buffer: 50 mM EDTA dissolved in 1x HMS buffer. Prepare 50 mL of this buffer, aliquot, and store at &#8722;20 &#176;C.</li>
		<li>Prepare 2x Protein loading buffer: 60 mM Tris-HCl, pH 6.8, 10% (v/v) glycerol, 2% (w/v) SDS, 0.005% (w/v) bromophenol blue. Make 50 mL, and store at 4 &#176;C. Just before use, add 100 &#181;L of 1 M 1,4-dithiothreitol (DTT) to 900 &#181;L of buffer.</li>
	</ol>
	</li>
	<li>To run a time-course with 3 time-points, prepare 3 tubes each containing a 130 &#181;L aliquot of import stop buffer, and leave them on ice. Prepare a 450 &#181;L import reaction in a 2 mL tube (per genotype/condition). Thaw all ingredients just prior to use.
	<ol>
		<li>For one import reaction, typically use 10 &#215; 106 chloroplasts in A &#181;L volume; for example, if the chloroplast concentration is 2.5 &#215; 108 /mL, use 40 &#181;L chloroplast suspension. Three time-points will need 3 &#215; A &#181;L (i.e., 120 &#181;L in our example).</li>
		<li>Mix the reactions components on ice in the following order: distilled water (to make the total volume 600 &#181;L), B &#181;L 10x HMS buffer (where B = [600-3&#215;A]/10; i.e., 48 in our example), 12 &#181;L 1 M gluconic acid (potassium salt), 6 &#181;L 1 M NaHCO3, 6 &#181;L 20% (w/v) BSA, 30 &#181;L 100 mM adenosine 5&#8242;-triphosphate magnesium salt (MgATP), 24 &#181;L 250 mM methionine (not radiolabeled), and 30 &#181;L precursor protein. Immediately before starting the import reaction, add 3 &#215; A &#181;L of chloroplasts and mix by gently tapping the tube.</li>
	</ol>
	</li>
	<li>Incubate the reaction tube at 25 &#176;C in a water bath under 100 &#181;mol&#183;m&#8722;2&#183;s&#8722;1 light. Occasionally flick the tubes to resuspend chloroplasts.</li>
	<li>To conduct a time-course, withdraw 130 &#181;L aliquots from the reaction at the required time-points within the linear range of import, which for pPsaD is up to ~12 min (4-, 8- and 12-min time points are suitable in this case). The linear range period can vary for different proteins 14. Thus, it is suggested to test each individual preprotein before to optimize the time points.</li>
	<li>Immediately upon withdrawal, transfer each 130 &#181;L aliquot to a tube of ice-cold import stop buffer, mix by gently tapping the tube, and retain all tubes on ice until the time-course has been completed.</li>
	<li>Centrifuge all samples for 30 s&#160;at 12,000 &#215; g in a microfuge, discard the supernatants by pipetting, and resuspend pellets in 15 &#181;L of 2x Protein loading buffer by vortexing.</li>
	<li>Analyze all the samples plus the pPsaD input control (containing pPsaD equivalent to 10% of the amount added to each import reaction, from step 2.7) by standard SDS-PAGE and autoradiography, fluorography&#160;or phosphor imaging 15. Use image analysis software to quantify and analyze the results. To provide an indication of import efficiency, the amount of imported protein in different genotypes/conditions can be assessed by measuring the radioactivity associated with each mature band.</li>
</ol>

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Authors have nothing to disclose.

We recently showed that chloroplast protein import can be actively regulated by stress, which is critical for chloroplast function and plant survival 3. In that study, to monitor such regulation, we modified our chloroplast isolation and in vitro import assay procedures in order to enable assessment of the import capacity of plants grown under stress conditions. The results indicated an important role for SP1 in chloroplast protein import regulation.
Conventional in vitro import assays use plants grown on standard MS agar medium6,17,18. In the case of the sp1 mutant described here, such conventional assays did not reveal any differences in protein import relative to the WT3. However, the role of SP1 in regulating protein import is clearly revealed when protein import is assessed under stress conditions using the methods described herein (Figure 1). While it may not be possible to directly compare import data from the stress conditions assay with those obtained from conventional assays (as the methods employ plants grown in liquid culture and on agar medium, respectively), comparisons between stress and non-stress conditions are feasible provided that the plants are all grown in the same liquid culture medium, with or without stressors.
Compared with the stress treatment on agar medium, liquid culture is more convenient for the treatment of the large numbers of plants needed for in vitro import assays. Moreover, it facilitates the uniform application of the stressor to all plants, which is particularly important for short-term stress treatments. The method presented here has been applied to study the osmotic stress using mannitol treatment, but could easily be adapted to a wide range of other stresses; for example, short-term salt stress and oxidative stress, for which the corresponding stressors could be similarly applied via liquid MS medium. For other types of stresses, we suggest the degree of stress is first optimized; overly severe treatments may have adverse effects on the yield and/or import competence of the isolated organelles.
There are several important steps within the protocol to which one should pay special attention, as detailed below.
The optimal agar concentration for the MS medium can differ (0.6 - 0.9%, w/v) depending on the manufacturer. Thus, it is recommended to empirically optimize the agar concentration before commencing experiments. The medium should not be so soft that it sticks to the tissue at the harvesting step (step 1.9), neither should it be so hard that it inhibits plant root development. The sucrose concentration can also be adjusted according to the plants used. When working with particularly sick mutants, MS medium supplemented with 2 - 3% (w/v) sucrose may help plants to grow better. When applying stress treatments, it is not good to transfer very old plants to the liquid medium (e.g., &#62;14 days old). This is because the more developed roots of older plants are more easily damaged during transferral.
With regard to the transcription/translation system, there are 2 major systems: those based on wheat germ, and those based on rabbit reticulocyte. These kits may use different templates, such as linearized plasmids, unlinearized plasmids, or PCR products. The kits are also specific for the T3, T7, and SP6 promoters. Note that the kit we recommend here is only suitable for use with PCR products and the T7 promoter. However, for unknown reasons, some radiolabeled preproteins made with this system might not work efficiently in the import assay; in such instances, one may consider trying a wheat germ extract system or a reticulocyte lysate system meant for plasmid templates. One may also improve the result of the transcription/translation reaction by modifying the reaction conditions according to the manufacturer&#39;s handbook.
It is important to start chloroplast isolation early in the morning (or early in the light cycle of the growth chamber) in order to avoid accumulation of starch inside the chloroplasts due to photosynthesis, which can hinder the isolation of intact organelles. The chloroplast isolation procedure has to be done quickly without any unnecessary delays, and the isolated chloroplasts must always be kept cold. This is to mitigate against the observation that isolated chloroplasts will gradually lose their viability, which is not good. If using newly thawed CIB or HMS buffer, be sure to mix the buffer well before use to obtain a homogeneous solution. The optimal conditions for the homogenization of plant material have been established empirically, and can vary if a different tissue homogenizer is used.
If the different plant genotypes contain similar chlorophyll levels, chlorophyll quantification can be used as an alternative way to normalize the samples before conducting the import assays. Chlorophyll can be determined spectrophotometrically following extraction of a sample of the isolated chloroplasts in 80% (v/v) aqueous acetone 19,20. However, if the import rates of plants showing different chlorophyll contents (e.g., mutants with chlorotic phenotypes) are to be compared, use chloroplast number counting to normalize the chloroplast samples in the import assays. It is particularly important to resuspend the chloroplasts thoroughly in step 3.11. Insufficient resuspension may leave aggregates of chloroplasts, which will make it difficult to count numbers accurately and thus will hinder the correct loading in import reactions. If severe aggregation is seen under the microscope (e.g., aggregates with &#62;10 chloroplast joined together), continue shaking the chloroplast sample on ice until the aggregates are removed. It is easier to resuspend the chloroplasts in a smaller volume of buffer.
It is important to be aware that protein import reactions (Section 5) must be conducted with appropriate precautions because of their radioactive nature. Necessary precautions include: wearing disposable gloves, laboratory clothing and safety glasses, monitoring and decontaminating the working surface and equipment, and disposing of all radioactive waste in an approved waste container. Also keep in mind that the correct osmotic pressure is critical for maintaining the intactness of chloroplasts during the import reactions, and this is chiefly maintained by the HMS buffer. Because 10x HMS is viscous, it should first be warmed up to RT, and then thoroughly mixed, and applied using a cut pipette tip to ensure measurement of accurate volumes. In the import reaction, cold methionine is added to inhibit the incorporation of free radiolabeled methionine into unrelated chloroplast proteins through organellar translation during the incubation step, while BSA is used to minimize proteolysis by acting as a substrate for proteases.

Chloroplasts are highly abundant organelles that exist in the green tissues of plants. They are well-known for their critical role in photosynthesis, a process that uses light energy to convert carbon dioxide to sugar and thus support almost all life on earth 1. In addition, chloroplasts (and the broader family of related organelles called plastids) play many other vital roles in plants, including the biosynthesis of amino acids, lipids, pigments, and the sensing of environmental signals such as gravity and pathogen challenge. Photosynthesis generates reactive oxygen species (ROS) as by-products, which under certain circumstances have useful roles, but if overproduced can cause damaging or even lethal effects. The overproduction of ROS is particularly promoted by adverse environmental conditions, and thus chloroplasts are closely linked to responses to abiotic stresses, such as salinity and osmotic stresses 2.
Chloroplasts have a complex structure. Each chloroplast is surrounded by a double-membrane outer layer called the envelope, which consists of outer and inner membranes. Internally, there is another membrane system called the thylakoids, where the light reactions of photosynthesis take place. Between the two membrane systems there is an aqueous compartment call the stroma, which is involved in carbon fixation. A chloroplast may contain up to ~3,000 different proteins, and the vast majority of these proteins are synthesized in the cytosol in precursor form and need to be imported into the organelle through dedicated protein translocons in the envelope membranes 1. Interestingly, recent work has indicated that chloroplast protein import is actively regulated, and so is able to exert an important level of control over the chloroplast proteome. For example, it was reported in 2015 that protein import can respond to abiotic stress through the direct regulation of the abundance of the translocon at the outer envelope membrane of chloroplasts (TOC) by the ubiquitin-proteasome system 3.
Using purified chloroplasts and in vitro synthesized precursor proteins, protein import can be reconstituted in vitro 4,5. Thus, in vitro methods can be used to assess the rates of import in different mutant plants 6, which has been a critical approach for the analysis of putative components of the protein import machinery and for discovering the mechanisms underlying protein import and its regulation. Moreover, chloroplasts can be processed with further fractionation or protease digestion, following in vitro import, which can facilitate studies on the sub-organellar localization and topology of chloroplast proteins 7,8.
To study the regulation of protein import by stress, we have modified our routine chloroplast isolation method as we will describe here. Importantly, chloroplasts were isolated from plants that had been grown on standard Murashige and Skoog (MS) agar medium for 8 days and then transferred into liquid MS medium supplemented with stressor, providing a relatively short, controlled stress treatment. The yield and competency of chloroplasts isolated from such stress-treated plants are compatible with the downstream in vitro protein import assay 3. In addition to the chloroplast isolation protocol, we present our routine method for in vitro protein import, which has proven to be robust and is widely used 3,9-12.

<table border="0" cellpadding="0" cellspacing="0" width="1048">
	<colgroup>
		<col />
		<col />
		<col />
		<col />
	</colgroup>
	<tbody>
		<tr height="21">
			<td height="21" style="height:21px;width:475px;">Murashige and Skoog basal salt&#160;</td>
			<td style="width:175px;">Melford</td>
			<td style="width:119px;">M0221</td>
			<td style="width:280px;"></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:475px;">phytoagar</td>
			<td style="width:175px;">Melford</td>
			<td style="width:119px;">P1003</td>
			<td style="width:280px;"></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:475px;">2-(N-morpholino) ethane sulfonic acid (MES)</td>
			<td style="width:175px;">Melford</td>
			<td style="width:119px;">B2002</td>
			<td style="width:280px;"></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:475px;">triton X-100&#160;</td>
			<td style="width:175px;">Fisher</td>
			<td style="width:119px;">BPE151-500</td>
			<td style="width:280px;"></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:475px;">surgical tape (e.g., Micropore, 3M)</td>
			<td style="width:175px;">3M</td>
			<td style="width:119px;">1530-1</td>
			<td style="width:280px;"></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:475px;">filter paper</td>
			<td style="width:175px;">Fisher</td>
			<td style="width:119px;">FB59023</td>
			<td style="width:280px;"></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:475px;">Percoll</td>
			<td style="width:175px;">Fisher</td>
			<td style="width:119px;">10607095</td>
			<td style="width:280px;"></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:475px;">ethylene glycol tetraacetic acid (EGTA)</td>
			<td style="width:175px;">Sigma</td>
			<td style="width:119px;">E4378</td>
			<td style="width:280px;"></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:475px;">ethylenediaminetetraacetic acid (EDTA)</td>
			<td style="width:175px;">Fisher</td>
			<td style="width:119px;">D/0700/53</td>
			<td style="width:280px;"></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:475px;">4-(2-hydroxyethyl)piperazine-1-ethanesulfonic acid (HEPES)</td>
			<td style="width:175px;">Melford</td>
			<td style="width:119px;">B2001</td>
			<td style="width:280px;"></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:475px;">filtration cloth (Miracloth)</td>
			<td style="width:175px;">Calbiochem</td>
			<td style="width:119px;">475855</td>
			<td style="width:280px;"></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:475px;">50 mL centrifuge tube</td>
			<td style="width:175px;">Fisher</td>
			<td style="width:119px;">CFT-595-040M</td>
			<td style="width:280px;"></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:475px;">250 mL centrifuge bottle</td>
			<td style="width:175px;">Fisher</td>
			<td style="width:119px;">CFT-891-V</td>
			<td style="width:280px;"></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:475px;">Polytron (e.g., Kinematica PT10-35)</td>
			<td style="width:175px;">Fisher</td>
			<td style="width:119px;">11010070</td>
			<td style="width:280px;"></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:475px;">Polytron probe (e.g., Kinematica PTA20S)</td>
			<td style="width:175px;">Fisher</td>
			<td style="width:119px;">11030083</td>
			<td style="width:280px;"></td>
		</tr>
		<tr height="42">
			<td height="42" style="height:42px;width:475px;">centrifuge (e.g., Beckman Coulter Avanti JXN-26, for 50 and 250 mL tubes)</td>
			<td style="width:175px;">Beckman Coulter</td>
			<td style="width:119px;">B34182</td>
			<td style="width:280px;"></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:475px;">fixed-angle rotor for 250 mL bottles (e.g., JLA-16.250)</td>
			<td style="width:175px;">Beckman Coulter</td>
			<td style="width:119px;">363930</td>
			<td style="width:280px;"></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:475px;">fixed-angle rotor for 50 mL tubes (e.g., JA-25.50)</td>
			<td style="width:175px;">Beckman Coulter</td>
			<td style="width:119px;">363058</td>
			<td style="width:280px;"></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:475px;">swinging-bucket rotor for 50 mL tubes (e.g., JS-13.1)</td>
			<td style="width:175px;">Beckman Coulter</td>
			<td style="width:119px;">346963</td>
			<td style="width:280px;"></td>
		</tr>
		<tr height="24">
			<td height="24" style="height:24px;width:475px;">radiolabeled [35S] methionine</td>
			<td style="width:175px;">Perkin Elmer</td>
			<td style="width:119px;">NEG072002MC</td>
			<td style="width:280px;"></td>
		</tr>
		<tr height="42">
			<td height="42" style="height:42px;width:475px;">rabbit reticulocyte lysate based cell-free translation system (TNT T7 Quick kit for PCR DNA)</td>
			<td style="width:175px;">Promega</td>
			<td style="width:119px;">L5540</td>
			<td style="width:280px;"></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:475px;">phase-contrast microscope (e.g., Nikon Eclipse 80i)</td>
			<td style="width:175px;">Nikon</td>
			<td style="width:119px;">unavailable</td>
			<td style="width:280px;"></td>
		</tr>
		<tr height="24">
			<td height="24" style="height:24px;width:475px;">haemocytometer (Improved Neubauer BS748 chamber)</td>
			<td style="width:175px;">Hawksley Technology</td>
			<td style="width:119px;">AC1000</td>
			<td style="width:280px;">0.1 mm depth, 1/400 mm2</td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:475px;">cover glasses</td>
			<td style="width:175px;">VWR</td>
			<td style="width:119px;">16004-094</td>
			<td style="width:280px;">22 mm &#215; 22 mm, thickness 0.13-0.17 mm</td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:475px;">1.5 mL microfuge tubes</td>
			<td style="width:175px;">Sarstedt</td>
			<td style="width:119px;">72.690.001</td>
			<td style="width:280px;"></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:475px;">2 mL microfuge tubes</td>
			<td style="width:175px;">Starlab</td>
			<td style="width:119px;">S1620-2700</td>
			<td></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:475px;">microfuge (e.g., Eppendorf 5415D)</td>
			<td style="width:175px;">Eppendorf</td>
			<td style="width:119px;">unavailable</td>
			<td style="width:280px;"></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:475px;">Nanodrop 2000 spectrophotometer or similar</td>
			<td style="width:175px;">Thermo Fisher</td>
			<td style="width:119px;">SPR-700-310L</td>
			<td style="width:280px;"></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:475px;">gluconic acid (potassium salt)</td>
			<td style="width:175px;">Fisher</td>
			<td style="width:119px;">22932-2500</td>
			<td style="width:280px;"></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:475px;">bovine serum albumin (BSA)</td>
			<td style="width:175px;">Sigma</td>
			<td style="width:119px;">A7906</td>
			<td style="width:280px;"></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:475px;">MgATP</td>
			<td style="width:175px;">Sigma</td>
			<td style="width:119px;">A9187</td>
			<td style="width:280px;"></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:475px;">methionine</td>
			<td style="width:175px;">Sigma</td>
			<td style="width:119px;">M6039</td>
			<td style="width:280px;"></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:475px;">bromophenol blue</td>
			<td style="width:175px;">Fisher</td>
			<td style="width:119px;">B/P620/44</td>
			<td style="width:280px;"></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:475px;">glycerol&#160;</td>
			<td style="width:175px;">Fisher</td>
			<td style="width:119px;">G/0650/17</td>
			<td style="width:280px;"></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:475px;">SDS</td>
			<td style="width:175px;">Fisher</td>
			<td style="width:119px;">S/5200/53</td>
			<td style="width:280px;"></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:475px;">Tris Base&#160;</td>
			<td style="width:175px;">Melford</td>
			<td style="width:119px;">B2005</td>
			<td style="width:280px;"></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:475px;">dithiothreitol (DTT)</td>
			<td style="width:175px;">Melford</td>
			<td style="width:119px;">MB1015</td>
			<td></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:475px;">image analysis software (e.g., Aida Image Analyzer)</td>
			<td style="width:175px;">Raytest</td>
			<td style="width:119px;">unavailable</td>
			<td></td>
		</tr>
	</tbody>
</table>

analysis of protein import into chloroplasts isolated from stressed plants

Chloroplasts are organelles with many vital roles in plants, which include not only photosynthesis but numerous other metabolic and signaling functions. Furthermore, chloroplasts are critical for plant responses to various abiotic stresses, such as salinity and osmotic stresses. A chloroplast may contain up to ~3,000 different proteins, some of which are encoded by its own genome. However, the majority of chloroplast proteins are encoded in the nucleus and synthesized in the cytosol, and these proteins need to be imported into the chloroplast through translocons at the chloroplast envelope membranes. Recent studies have shown that the chloroplast protein import can be actively regulated by stress. To biochemically investigate such regulation of protein import under stress conditions, we developed the method described here as a quick and straightforward procedure that can easily be achieved in any laboratory. In this method, plants are grown under normal conditions and then exposed to stress conditions in liquid culture. Plant material is collected, and chloroplasts are then released by homogenization. The crude homogenate is separated by density gradient centrifugation, enabling isolation of the intact chloroplasts. Chloroplast yield is assessed by counting, and chloroplast intactness is checked under a microscope. For the protein import assays, purified chloroplasts are incubated with 35S radiolabeled in vitro translated precursor proteins, and time-course experiments are conducted to enable comparisons of import rates between genotypes under stress conditions. We present data generated using this method which show that the rate of protein import into chloroplasts from a regulatory mutant is specifically altered under osmotic stress conditions.

An example chloroplast protein import experiment with 3 time-points is shown in Figure 1. PsaD is an ~18 kD component of photosystem I exposed to the stroma, with a precursor form of ~23 kD16. PsaD was selected here for the&#160;in vitro&#160;protein import assay because its steady-state levels are elevated in the&#160;sp1&#160;mutant, relative to WT, under stress conditions, suggesting a change in its import efficiency in the mutant&#160;3. The sp1 mutant carries a defect in an important regulator of the chloroplast protein import machinery &#8212; the SP1 protein 3. For chloroplasts isolated from plants grown under normal conditions, there was no obvious difference in PsaD import between sp1 and WT (data not shown)3. However, using the methods described here to assess PsaD import into chloroplasts isolated from osmotically stressed plants, a clear difference was detected. While we observed the&#160;accumulation of the mature protein form in a time-dependent manner with both genotypes, the rate of import was significantly lower for WT chloroplasts than for sp1 chloroplasts (Figure 1), which is consistent with our previous results&#160;3, and reveals an important role for the SP1 protein in regulating the chloroplast import of PsaD under stress conditions.&#160;
<img alt="Figure 1" src="/files/ftp_upload/54717/54717fig1.jpg" /> 
Figure 1. A Protein Import Assay Conducted using Chloroplasts Isolated from Plants Grown under Osmotic Stress Conditions. Chloroplasts were isolated from a&#160;10-day-old WT (Col-0) and a&#160;sp1 mutant Arabidopsis plants grown under stress conditions (200 mM mannitol) for 2 d. (A) Protein import was conducted using [35S]-methionine-labeled pPsaD and allowed to proceed for 4, 8 and 12 min before analysis by SDS-PAGE and phosphor imaging. In parallel, the pPsaD 10% input control comprising in vitro translated protein (IVT) was analyzed. The precursor (pre) and mature (mat) forms of pPsaD are indicated, while in between there are two bands that likely correspond to truncated or proteolyzed translation products because their intensity did not change during the time course&#160;(*). (B) To compare the rates of import into chloroplasts from WT and sp1 plants grown under stress conditions, the intensity of each band corresponding to imported mature protein in A was quantified. All data are expressed as percentages of the amount of imported protein in chloroplasts from WT plants after 12 min. <a href="http://cloudflare.jove.com/files/ftp_upload/54717/54717fig1large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>

Watch this Scientific Journal Video about Analysis of Protein Import into Chloroplasts Isolated from Stressed Plants at JoVE.com

Analysis of Protein Import into Chloroplasts Isolated from Stressed Plants | Biology | Video

Analysis of Protein Import into Chloroplasts Isolated from Stressed Plants

Here we describe a new method to study protein import into isolated chloroplasts under stress. The method is rapid and straightforward, and can be applied to study the consequences of different stress conditions for chloroplast protein import, and the corresponding regulatory mechanisms.

Chloroplasts are organelles with many vital roles in plants, which include not only photosynthesis but numerous other metabolic and signaling functions. ...

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20.9K Views.  University of Oxford. Here we describe a new method to study protein import into isolated chloroplasts under stress. The method is rapid and straightforward, and can be applied to study the consequences of different stress conditions for chloroplast protein import, and the corresponding regulatory mechanisms.

Video: Analysis of Protein Import into Chloroplasts Isolated from Stressed Plants

Staining of Proteins in Gels with Coomassie G-250 without Organic Solvent and Acetic Acid

In classical protein staining protocols using Coomassie Brilliant Blue (CBB), solutions with high contents of toxic and flammable organic solvents (Methanol, Ethanol or 2-Propanol) and acetic acid are used for fixation, staining and destaining of proteins in a gel after SDS-PAGE. To speed up the procedure, heating the staining solution in the microwave oven for a short time is frequently used. This usually results in evaporation of toxic or hazardous Methanol, Ethanol or 2-Propanol and a strong smell of acetic acid in the lab which should be avoided due to safety considerations. In a protocol originally published in two patent applications by E.M. Wondrak (US2001046709 (A1), US6319720 (B1)), an alternative composition of the staining solution is described in which no organic solvent or acid is used. The CBB is dissolved in bidistilled water (60-80mg of CBB G-250 per liter) and 35 mM HCl is added as the only other compound in the staining solution. The CBB staning of the gel is done after SDS-PAGE and thorough washing of the gel in bidistilled water. By heating the gel during the washing and staining steps, the process can be finished faster and no toxic or hazardous compunds are evaporating. The staining of proteins occurs already within 1 minute after heating the gel in staining solution and is fully developed after 15-30 min with a slightly blue background that is destained completely by prolonged washing of the stained gel in bidistilled water, without affecting the stained protein bands.

A short protocol for protein staining with Coomassie Brilliant Blue (CBB) G-250 in polyacrylamide gels is described without using organic solvents or acetic acid as in the classical staining procedures with CBB.

In classical protein staining protocols using Coomassie Brilliant Blue (CBB), solutions with high contents of toxic and flammable organic solvents ...

Using the GELFREE 8100 Fractionation System for Molecular Weight-Based Fractionation with Liquid Phase Recovery

The GELFREE 8100 Fractionation System is a novel protein fractionation system designed to maximize protein recovery during molecular weight based fractionation. The system is comprised of single-use, 8-sample capacity cartridges and a benchtop GELFREE Fractionation Instrument. During separation, a constant voltage is applied between the anode and cathode reservoirs, and each protein mixture is electrophoretically driven from a loading chamber into a specially designed gel column gel. Proteins are concentrated into a tight band in a stacking gel, and separated based on their respective electrophoretic mobilities in a resolving gel. As proteins elute from the column, they are trapped and concentrated in liquid phase in the collection chamber, free of the gel. The instrument is then paused at specific time intervals, and fractions are collected using a pipette. This process is repeated until all desired fractions have been collected. If fewer than 8 samples are run on a cartridge, any unused chambers can be used in subsequent separations.
This novel technology facilitates the quick and simple separation of up to 8 complex protein mixtures simultaneously, and offers several advantages when compared to previously available fractionation methods. This system is capable of fractionating up to 1mg of total protein per channel, for a total of 8mg per cartridge. Intact proteins over a broad mass range are separated on the basis of molecular weight, retaining important physiochemical properties of the analyte. The liquid phase entrapment provides for high recovery while eliminating the need for band or spot cutting, making the fractionation process highly reproducible1.

The accompanying video describes the use of the GELFREE 8100 Fractionation System, which partitions complex protein samples on the basis of molecular weight and recovers the fractions in liquid phase. The video describes how the technology works, how it is used, and provides resultant data, with polyacrylamide gel electrophoresis analysis of fractionated bovine liver homogenate.

The GELFREE 8100 Fractionation System is a novel protein fractionation system designed to maximize protein recovery during molecular weight based ...

Measuring Spatial and Temporal Ca2+ Signals in Arabidopsis Plants

Developmental and environmental cues induce Ca2+ fluctuations in plant cells. Stimulus-specific spatial-temporal Ca2+ patterns are sensed by cellular Ca2+ binding proteins that initiate Ca2+ signaling cascades. However, we still know little about how stimulus specific Ca2+ signals are generated. The specificity of a Ca2+ signal may be attributed to the sophisticated regulation of the activities of Ca2+ channels and/or transporters in response to a given stimulus. To identify these cellular components and understand their functions, it is crucial to use systems that allow a sensitive and robust recording of Ca2+ signals at both the tissue and cellular levels. Genetically encoded Ca2+ indicators that are targeted to different cellular compartments have provided a platform for live cell confocal imaging of cellular Ca2+ signals. Here we describe instructions for the use of two Ca2+ detection systems: aequorin based FAS (film adhesive seedlings) luminescence Ca2+ imaging and case12 based live cell confocal fluorescence Ca2+ imaging. Luminescence imaging using the FAS system provides a simple, robust and sensitive detection of spatial and temporal Ca2+ signals at the tissue level, while live cell confocal imaging using Case12 provides simultaneous detection of cytosolic and nuclear Ca2+ signals at a high resolution.

Measuring Spatial and Temporal Ca2+ Signals in Arabidopsis Plants

Ca2+ signaling regulates diverse biological processes in plants. Here we present approaches for monitoring abiotic stress induced spatial and temporal Ca2+ signals in Arabidopsis cells and tissues using the genetically encoded Ca2+ indicators Aequorin or Case12.

Developmental and environmental cues induce Ca2+ fluctuations in plant cells. Stimulus-specific spatial-temporal Ca2+ patterns are sensed by cellular Ca2+ ...

Green Fluorescent Protein-based Expression Screening of Membrane Proteins in Escherichia coli

The production of recombinant membrane proteins for structural and functional studies remains technically challenging due to low levels of expression and the inherent instability of many membrane proteins once solubilized in detergents. A protocol is described that combines ligation independent cloning of membrane proteins as GFP fusions with expression in Escherichia coli detected by GFP fluorescence. This enables the construction and expression screening of multiple membrane protein/variants to identify candidates suitable for further investment of time and effort. The GFP reporter is used in a primary screen of expression by visualizing GFP fluorescence following SDS polyacrylamide gel electrophoresis (SDS-PAGE). Membrane proteins that show both a high expression level with minimum degradation as indicated by the absence of free GFP, are selected for a secondary screen. These constructs are scaled and a total membrane fraction prepared and solubilized in four different detergents. Following ultracentrifugation to remove detergent-insoluble material, lysates are analyzed by fluorescence detection size exclusion chromatography (FSEC). Monitoring the size exclusion profile by GFP fluorescence provides information about the mono-dispersity and integrity of the membrane proteins in different detergents. Protein: detergent combinations that elute with a symmetrical peak with little or no free GFP and minimum aggregation are candidates for subsequent purification. Using the above methodology, the heterologous expression in E. coli of SED (shape, elongation, division, and sporulation) proteins from 47 different species of bacteria was analyzed. These proteins typically have ten transmembrane domains and are essential for cell division. The results show that the production of the SEDs orthologues in E. coli was highly variable with respect to the expression levels and integrity of the GFP fusion proteins. The experiment identified a subset for further investigation.

Green Fluorescent Protein-based Expression Screening of Membrane Proteins in Escherichia coli

A streamlined approach to screening for the expression of recombinant membrane proteins in Escherichia coli based on fusion to green fluorescent protein is presented.

The production of recombinant membrane proteins for structural and functional studies remains technically challenging due to low levels of expression and ...

Single-channel Analysis and Calcium Imaging in the Podocytes of the Freshly Isolated Glomeruli

Podocytes (renal glomerular epithelial cells) are known to regulate glomerular permeability and maintain glomerular structure; a key role for these cells in the pathogenesis of various renal diseases has been established since podocyte injury leads to proteinuria and foot process effacement. It was previously reported that various endogenous agents may cause a dramatic overload in intracellular Ca2+ concentration in podocytes, presumably leading to albuminuria, and this likely occurs via calcium-conducting ion channels. Therefore, it appeared important to study calcium handling in the podocytes both under normal conditions and in various pathological states. However, available experimental approaches have remained somewhat limited to cultured and transfected cells. Although they represent a good basic model for such studies, they are essentially extracted from the native environment of the glomerulus. Here we describe the methodology of studying podocytes as a part of the freshly isolated whole glomerulus. This preparation retains the functional potential of the podocytes, which are still attached to the capillaries; therefore, podocytes remain in the environment that conserves the major parts of the glomeruli filtration apparatus. The present manuscript elaborates on two experimental approaches that allow 1) real-time detection of calcium concentration changes with the help of ratiometric confocal fluorescence microscopy, and 2) the recording of the single ion channels activity in the podocytes of the freshly isolated glomeruli. These methodologies utilize the advantages of the native environment of the glomerulus that enable researchers to resolve acute changes in the intracellular calcium handling in response to applications of various agents, measure basal concentration of calcium within the cells (for instance, to evaluate disease progression), and assess and manipulate calcium conductance at the level of single ion channels.

Changes in the intracellular calcium levels in the podocytes are one of the most important means to control the filtration function of glomeruli. Here we explain a high-throughput approach that allows detection of real-time calcium handling and single ion channels activity in the podocytes of the freshly isolated glomeruli.

Podocytes (renal glomerular epithelial cells) are known to regulate glomerular permeability and maintain glomerular structure; a key role for these cells ...

Enrichment of Extracellular Matrix Proteins from Tissues and Digestion into Peptides for Mass Spectrometry Analysis

The extracellular matrix (ECM) is a complex meshwork of cross-linked proteins that provides biophysical and biochemical cues that are major regulators of cell proliferation, survival, migration, etc. The ECM plays important roles in development and in diverse pathologies including cardio-vascular and musculo-skeletal diseases, fibrosis, and cancer. Thus, characterizing the composition of ECMs of normal and diseased tissues could lead to the identification of novel prognostic and diagnostic biomarkers and potential novel therapeutic targets. However, the very nature of ECM proteins (large in size, cross-linked and covalently bound, heavily glycosylated) has rendered biochemical analyses of ECMs challenging. To overcome this challenge, we developed a method to enrich ECMs from fresh or frozen tissues and tumors that takes advantage of the insolubility of ECM proteins. We describe here in detail the decellularization procedure that consists of sequential incubations in buffers of different pH and salt and detergent concentrations and that results in 1) the extraction of intracellular (cytosolic, nuclear, membrane and cytoskeletal) proteins and 2) the enrichment of ECM proteins. We then describe how to deglycosylate and digest ECM-enriched protein preparations into peptides for subsequent analysis by mass spectrometry.

This protocol describes a procedure for enriching ECM proteins from tissues or tumors and deglycosylating and digesting the ECM-enriched preparations into peptides to analyze their protein composition by mass spectrometry.

The extracellular matrix (ECM) is a complex meshwork of cross-linked proteins that provides biophysical and biochemical cues that are major regulators of ...

Cycloheximide Chase Analysis of Protein Degradation in Saccharomyces cerevisiae

Regulation of protein abundance is crucial to virtually every cellular process. Protein abundance reflects the integration of the rates of protein synthesis and protein degradation. Many assays reporting on protein abundance (e.g., single-time point western blotting, flow cytometry, fluorescence microscopy, or growth-based reporter assays) do not allow discrimination of the relative effects of translation and proteolysis on protein levels. This article describes the use of cycloheximide chase followed by western blotting to specifically analyze protein degradation in the model unicellular eukaryote, Saccharomyces cerevisiae (budding yeast). In this procedure, yeast cells are incubated in the presence of the translational inhibitor cycloheximide. Aliquots of cells are collected immediately after and at specific time points following addition of cycloheximide. Cells are lysed, and the lysates are separated by polyacrylamide gel electrophoresis for western blot analysis of protein abundance at each time point. The cycloheximide chase procedure permits visualization of the degradation kinetics of the steady state population of a variety of cellular proteins. The procedure may be used to investigate the genetic requirements for and environmental influences on protein degradation.

Cycloheximide Chase Analysis of Protein Degradation in Saccharomyces cerevisiae

Protein abundance reflects the rates of both protein synthesis and protein degradation. This article describes the use of cycloheximide chase followed by western blotting to analyze protein degradation in the model unicellular eukaryote, Saccharomyces cerevisiae (budding yeast).

Regulation of protein abundance is crucial to virtually every cellular process. Protein abundance reflects the integration of the rates of protein ...

Comparison of Tobacco Host Cell Protein Removal Methods by Blanching Intact Plants or by Heat Treatment of Extracts

Plants not only provide food, feed and raw materials for humans, but have also been developed as an economical production system for biopharmaceutical proteins, such as antibodies, vaccine candidates and enzymes. These must be purified from the plant biomass but chromatography steps are hindered by the high concentrations of host cell proteins (HCPs) in plant extracts. However, most HCPs irreversibly aggregate at temperatures above 60 &#176;C facilitating subsequent purification of the target protein. Here, three methods are presented to achieve the heat precipitation of tobacco HCPs in either intact leaves or extracts. The blanching of intact leaves can easily be incorporated into existing processes but may have a negative impact on subsequent filtration steps. The opposite is true for heat precipitation of leaf extracts in a stirred vessel, which can improve the performance of downstream operations albeit with major changes in process equipment design, such as homogenizer geometry. Finally, a heat exchanger setup is well characterized in terms of heat transfer conditions and easy to scale, but cleaning can be difficult and there may be a negative impact on filter capacity. The design-of-experiments approach can be used to identify the most relevant process parameters affecting HCP removal and product recovery. This facilitates the application of each method in other expression platforms and the identification of the most suitable method for a given purification strategy.

Three heat precipitation methods are presented that effectively remove more than 90% of host cell proteins (HCPs) from tobacco extracts prior to any other purification step. The plant HCPs irreversibly aggregate at temperatures above 60 &#176;C.

Plants not only provide food, feed and raw materials for humans, but have also been developed as an economical production system for biopharmaceutical ...

Light Sheet Fluorescence Microscopy of Plant Roots Growing on the Surface of a Gel

One of the key questions in understanding plant development is how single cells behave in a larger context of the tissue. Therefore, it requires the observation of the whole organ with a high spatial- as well as temporal resolution over prolonged periods of time, which may cause photo-toxic effects. This protocol shows a plant sample preparation method for light-sheet microscopy, which is characterized by mounting the plant vertically on the surface of a gel. The plant is mounted in such a way that the roots are submerged in a liquid medium while the leaves remain in the air. In order to ensure photosynthetic activity of the plant, a custom-made lighting system illuminates the leaves. To keep the roots in darkness the water surface is covered with sheets of black plastic foil. This method allows long-term imaging of plant organ development in standardized conditions.

This protocol shows a plant sample preparation method for light-sheet microscopy. The setup is characterized by mounting the plant vertically on the surface of a gel and letting it grow in controlled bright conditions. This allows long-term observation of plant organ development in standardized conditions.

One of the key questions in understanding plant development is how single cells behave in a larger context of the tissue. Therefore, it requires the ...

Analysis of Cell Suspensions Isolated from Solid Tissues by Spectral Flow Cytometry

Flow cytometry has been used for the past 40 years to define and analyze the phenotype of lymphoid and other hematopoietic cells. Initially restricted to the analysis of a few fluorochromes, currently there are dozens of different fluorescent dyes, and up to 14-18 different dyes can be combined at a time. However, several limitations still impair the analytical capabilities. Because of the multiplicity of fluorescent probes, data analysis has become increasingly complex due to the need of large, multi-parametric compensation matrices. Moreover, mutant mouse models carrying fluorescent proteins to detect and trace specific cell types in different tissues have become available, so the analysis (by flow cytometry) of auto-fluorescent cell suspensions obtained from solid organs is required. Spectral flow cytometry, which distinguishes the shapes of emission spectra along a wide range of continuous wavelengths, addresses some of these problems. The data is analyzed with an algorithm that replaces compensation matrices and treats auto-fluorescence as an independent parameter. Thus, spectral flow cytometry should be capable of discriminating fluorochromes with similar emission peaks and can provide a multi-parametric analysis without compensation requirements.
This protocol describes the spectral flow cytometry analysis, allowing for a 21-parameter (19 fluorescent probes) characterization and the management of an auto-fluorescent signal, providing high resolution in minor population detection. The results presented here show that spectral flow cytometry presents advantages in the analysis of cell populations from tissues difficult to characterize in conventional flow cytometry, such as the heart and the intestine. Spectral flow cytometry thus demonstrates the multi-parametric analytical capacity of high-performing conventional flow cytometry without the requirement for compensation and enables auto-fluorescence management.

This article describes spectral cytometry, a new approach in flow cytometry that uses the shapes of emission spectra to distinguish fluorochromes. An algorithm replaces compensations and can treat auto-fluorescence as an independent parameter. This new approach allows for the proper analysis of cells isolated from solid organs.

Flow cytometry has been used for the past 40 years to define and analyze the phenotype of lymphoid and other hematopoietic cells. Initially restricted to ...