This manuscript was prepared with funding by the Division of Chemical Sciences, Geosciences, and Biosciences, 408 Office of Basic Energy Sciences of the US Department of Energy through Grant DE-SC0017035

1. Initial Materials
<ol>
	<li>Soak approximately 55 g of peas for 3 hours in 400 mL of distilled water, and then sow in a plastic tray (35 cm x 20 cm x 6 cm) in soil covered with thin layer of vermiculite.</li>
	<li>Grow the tray of peas at 20 &#176;C under 12/12 h light/dark (50 &#181;E/m2s) cycle for 9 to 15 days.</li>
	<li>Prepare protein substrate according to a preferred method. 
	Note: We have prepared protein substrates using a variety of methods, including 1) in vitro transcription from purified plasmids followed by translation using wheat germ extracts or rabbit reticulocyte lysates in the presence of [3H]-leucine or [35S]-methionine, 2) in vitro translation using a coupled transcription/translation kit such as the TnT kits from Promega, with radiolabeling as above, and 3) purification of overexpressed protein in E. coli. Radioactive in vitro translation products are generally quenched with 50 mM cold amino acid prior to use in transport reactions. Each of these methods typically requires some optimization for each new protein substrate. For an example of a coupled in vitro system, see Ling and Jarvis (2016)9.</li>
</ol>
2. Chloroplast Isolation and Quantification
Note: The first step in preparation of thylakoids is the isolation of intact chloroplasts10. All materials should be kept cold during preparation. Resuspension of chloroplasts should be handled gently, as breakage at this step can severely limit subsequent thylakoid yield.
<ol>
	<li>Prepare following solutions beforehand.
	<ol>
		<li>2x Grinding Buffer (2xGB): 100 mM K-HEPES pH 7.3, 660 mM sorbitol, 2 mM MgCl2, 2 mM MnCl2, 4 mM EDTA, 0.2% BSA.</li>
		<li>2x Import Buffer (2xIB): 100 mM K-Tricine or K-HEPES pH 8.0, 660 mM sorbitol, 8 mM MgCl2. 
		Note: Concentrations of MgCl2 ranging from 3 mM to 10 mM have been used without observable differences.</li>
	</ol>
	</li>
	<li>Prepare a continuous density gradient by centrifuging a mixture of 15 mL of Percoll and 15 mL of 2xGB at 30,900 g in a fixed angle rotor for 30 min at 4 &#176;C with the brake off.</li>
	<li>Harvest approximately 25 g of 9-15 day old peas and homogenize in 95 mL of 1xGB. Either a blender with sharpened blades or a Polytron have been used successfully. Filter this mixture through at least 2 layers of Miracloth in a funnel. 
	Note: Limiting the amount of stem tissue is not necessary but can make the homogenization process easier, thereby reducing chloroplast breakage that can occur with prolonged blending.</li>
	<li>Pellet at 3,000 g in a swinging bucket rotor for 5 min at 4 &#176;C, and gently resuspend in 1 mL of 1xGB. A paintbrush may be the most gentle resuspension technique.</li>
	<li>Carefully layer the green suspension on top of the Percoll gradient and centrifuge at 8,000 g in a swinging bucket rotor for 10 min at 4 &#176;C with the brake off.</li>
	<li>Carefully harvest the lower green band containing intact chloroplasts into a fresh tube. Spin the recovered intact chloroplasts at 1,800 g in a swinging bucket rotor for 5 min at 4 &#176;C, discard the supernatant and gently resuspend the pellet in 1xIB. Repeat this wash step once more, resuspending in 30 mL of 1xIB each time, with the final resuspension in 1 mL of 1xIB.</li>
	<li>To quantify chlorophyll (Chl) content, mix 10 &#181;L of fully resuspended chloroplasts with 5 mL of 80% acetone and filter through Whatman 1 filter paper (nominal thickness 180 &#181;m). Record the absorbance at 720 nm, 663 nm, and 645 nm in a spectrophotometer and calculate the Chl concentration using the following formula11: 
	[Chl] mg/mL = [40.2*(A663 &#8211; A720) + 101.4*(A645 &#8211; A720)]*0.1</li>
	<li>Adjust chloroplasts to 1 mg/mL Chl equivalents with 1xIB.</li>
</ol>
3. Isolation of Thylakoids
Note: Thylakoids are prepared by hypotonic lysis of intact chloroplasts. This is achieved by exposing the chloroplasts to a hypotonic buffer lacking sorbitol. Isolated thylakoids can be used for assaying any of the translocation pathways, but stromal extract (SE) must also be isolated during this preparation if either cpSec1 or cpSRP pathways are to be investigated.
<ol>
	<li>Prepare ahead of time the following solutions.
	<ol>
		<li>Hypotonic Lysis Buffer: 50 mM K-Tricine or K-HEPES pH 8.0, 8 mM MgCl2.</li>
		<li>2x Crude Stroma Buffer (for concentration of SE): 100 mM K-HEPES pH 8.0, 660 mM sorbitol, 8 mM MgCl2.</li>
		<li>Laemmli Sample Buffer (for SDS-PAGE, supplemented with EDTA): 125 mM Tris pH 6.8, 10% SDS, 20% glycerol, 0.05 mg/mL bromophenol blue, 10% &#946;-mercaptoethanol, 10 mM EDTA.</li>
	</ol>
	</li>
	<li>If SE recovery is not necessary, centrifuge the intact chloroplasts at 1,000 g in a swinging bucket rotor for 6 min at 4 &#176;C.
	<ol>
		<li>Discard the supernatant and resuspend to 1 mg/mL in Hypotonic Lysis Buffer. Incubate on ice in the dark for 10 min, with occasional mixing.</li>
		<li>Recover thylakoids by centrifuging at 3,200 g in swinging bucket rotor for 8 min at 4 &#176;C. Wash the thylakoids twice, resuspending with 1 to 2 mL of lysis buffer each time. Resuspend with 1 mL of 1xIB and requantify Chl as above in the chloroplast isolation protocol.</li>
	</ol>
	</li>
</ol>
4. Stromal Extract Recovery and Concentration
<ol>
	<li>If SE recovery is necessary, divide the intact chloroplasts into 600 &#181;L aliquots in 1.5 mL microcentrifuge tubes and centrifuge each tube at 1,000 g in swinging bucket rotor for 6 min at 4 &#176;C. 
	Note: This volume is convenient when using 1.5 mL microcentrifuge tubes, which helps to prevent disturbance of the eventual pellet for residual membranes.
	<ol>
		<li>Resuspend to 1 mg/mL Chl in Hypotonic Lysis Buffer and incubate on ice in the dark for 10 min, as in step 3.2.1.</li>
		<li>Centrifuge each tube at 3,200 x g in swinging bucket rotor for 8 min at 4 &#176;C and transfer the light green or yellow supernatant following chloroplast lysis to a new microcentrifuge tube with an equal volume of 2x Crude Stroma Buffer.</li>
		<li>Wash thylakoids with 2 volumes of lysis buffer (approximating 0.5 mg/mL) and collect by centrifugation at 3,200 g in swinging bucket rotor for 8 min at 4 &#176;C. Resuspend to 1 mg/mL Chl in 1xIB on ice.</li>
		<li>Centrifuge crude stroma at 42,000 g in a fixed angle rotor for 30 min at 4 &#176;C to remove residual membranes. Immunoblotting for outer and inner envelope proteins can be used to verify the purity of the supernatant.</li>
		<li>Collect 95% of the volume from each tube without disturbing the small yellow-green pellet. Note the volume taken from each tube.</li>
		<li>To prepare the concentrated stromal extract (SE), pool the collected supernatants and concentrate five-fold using a 4 mL 30 kDa MWCO concentrator. 
		Note: SE prepared in this manner is equivalent to stroma derived from chloroplasts at 2.5 mg/mL Chl. If necessary, SE can be concentrated ten-fold to 5 mg/mL Chl equivalents. SE will be golden in color and viscous. In the lab&#8217;s Legend RT centrifuge with swinging bucket rotor, this requires about 10 min per mL concentrated.</li>
	</ol>
	</li>
</ol>
5. Transport through the cpTat Pathway
Note: Unlike the cpSec1 or cpSRP, the cpTat pathway does not require soluble components or exogenously added energy sources; only the light-driven proton motive force is necessary3. Therefore, only isolated thylakoids and substrate protein are required for the assay. Typical substrates are intermediate forms of the 17 kDa (as seen in Figure 1) and 23 kDa subunits of the oxygen evolving complex, iOE17 and iOE23, respectively, but precursor forms, prOE17 and prOE23, can also be successfully transported. Precursor forms have the entire bipartite N-terminal targeting sequence, while intermediate forms have only the thylakoid targeting sequence.
<ol>
	<li>Prepare cpTat transport mix with 0.33 mg/mL Chl thylakoids, 5 mM ATP from a stock prepared in 1xIB, and 8 mM dithiothreitol (DTT) from a stock prepared in 1xIB, on ice. ATP is not strictly required for this reaction if conducted under illumination.</li>
	<li>Initiate transport by introducing 1:30 volume by volume substrate protein in the transport mix. If substrate protein is not prepared in 1xIB, prepare a 1:1 dilution with 2xIB first, then use 1:30&#160; volume by volume of the diluted substrate in the transport mix. 
	Note: Concentrations of substrate will vary based on the preparation method. Typically, in vitro preparations will allow for nanomolar to micromolar amounts, while overexpression will allow for micromolar to millimolar amounts. Detection methods must also be considered, as autoradiography and fluorography are more sensitive than immunoblotting.</li>
	<li>Illuminate the suspension in 80 - 100 &#181;E/m2s of photosynthetically active radiation (PAR) for 10 min at room temperature. If transport kinetics are required, pre-equilibrate both thylakoids and reaction mix to room temperature and illuminate for up to 30 min.</li>
	<li>Stop the transport reaction with an 8-fold dilution of ice-cold 1xIB and recover thylakoids by centrifugation at 3,200 g in microcentrifuge for 5 min at 4 &#176;C.</li>
	<li>Remove residual substrate that has not been transported, resuspend the thylakoid pellet in 120 &#181;L of 1xIB and digest external protein by addition of 6 &#181;L of 2 mg/mL thermolysin and 10 mM CaCl2 in 1xIB.</li>
	<li>Incubate the protease reaction on ice for 40 min, and then quench the protease by doubling the volume with 25 mM EDTA prepared in 1xIB.</li>
	<li>Recover thylakoids by centrifuging at 3,200 g in a microcentrifuge for 5 min at 4 &#176;C. Wash recovered thylakoids in 120 &#956;L of 5 mM EDTA in 1xIB and transfer to a new tube.</li>
	<li>Centrifuge at 3,200 g in a microcentrifuge for 5 min at 4 &#176;C. Resuspend in an appropriate volume of Laemmli Sample Buffer supplemented with 10 mM EDTA. A volume of 40 &#181;L is usually enough to detect substrate on an SDS-PAGE gel and conserves sample for repeat gels when necessary.</li>
	<li>Place samples in a boiling water bath for 10 min and analyze by SDS-PAGE. Autoradiography, fluorography, or Western blotting of non-native or epitope-tagged proteins have been successfully used for detection of transported proteins.</li>
</ol>
6. Transport through the cpSec1 Pathway
Note: Transport through the cpSec1 translocon requires the stromal protein cpSecA112,13, which can be procured via overexpression in E. coli14,15 or recovered by concentrating stroma during thylakoid isolation. A typical substrate is the 33 kDa subunit of the oxygen evolving complex (prOE33), as seen in Figure 2.
<ol>
	<li>Prepare the cpSec1 transport mix with 0.33 mg/mL Chl thylakoids, 0.83 mg/mL Chl equivalent SE or 1.5 &#956;g of recombinant cpSecA1, and 5 mM ATP on ice, and incubate for 10 min. A typical transport reaction mixture here is 72 &#956;L, up from 60 &#956;L due to the SE addition.
	<ol>
		<li>If recombinant cpSecA1 will be used instead of SE, adjust purified cpSecA1 with an equal volume of 2xIB, then dilute to a convenient concentration to add to the transport reactions (e.g., 0.75 &#181;g/&#181;L). 
		Note: For long term storage, cpSecA1 is stored on ice in a controlled, refrigerated room after purification as freezing abolishes activity.</li>
	</ol>
	</li>
	<li>Initiate transport by introducing 1:10 volume by volume substrate protein to the transport mix. If substrate protein is not prepared in 1xIB, prepare a 1:1 dilution with 2xIB and add 1:10 volume by volume of the diluted protein to the transport mix.</li>
	<li>Incubate the reaction at room temperature for 10 min under 80 &#8211; 100 &#181;E/m2s PAR. Again, longer times may be necessary for kinetics or certain substrates.</li>
	<li>After light treatment, dilute 8-fold with ice-cold 1xIB and centrifuge reactions at 3200 g in microcentrifuge for 5 min at 4 &#176;C.</li>
	<li>Treat with thermolysin and quench with EDTA as above in Steps 5.5 through 5.7.</li>
	<li>Centrifuge at 3,200 g in microcentrifuge for 5 min at 4 &#176;C and resuspend the pellet in an appropriate volume of Laemmli Sample Buffer supplemented with 10 mM EDTA. Place in boiling water bath for 10 min prior to loading on SDS-PAGE gel.</li>
</ol>
7. Insertion through the cpSRP Pathway
Note: The cpSRP-mediated integration of light harvesting complex proteins (LHCP) seen in Figure 3 requires cpSRP54, cpSRP43, and cpFtsY16. These components are supplied to the transport reaction through concentrated stromal extract, as described for the cpSec1 transport protocol.
<ol>
	<li>Prepare the cpSRP transport mix with 0.33 mg/mL Chl thylakoids, 0.83 mg/mL Chl equivalent SE, and 5 mM ATP on ice and incubate for 10 min.</li>
	<li>Initiate transport by introducing 1:10 volume by volume substrate protein to the transport mix. If substrate protein is not prepared in 1xIB, prepare a 1:1 dilution with 2xIB and add 1:10 volume by volume of the diluted protein to the transport mix.</li>
	<li>Incubate reaction at room temperature for 10 min in 80 &#8211; 100 &#181;E/m2s PAR.</li>
	<li>After light treatment, dilute 8-fold with ice-cold 1xIB and centrifuge reactions at 3,200 g in microcentrifuge for 5 min at 4 &#176;C. Discard supernatant and resuspend the pellet in 120 &#181;L of 1xIB.</li>
	<li>Treat with thermolysin as above in sections 5.5 through 5.7. Thermolysin digestion is necessary here to assess successful membrane integration. Wash recovered thylakoids in 120 &#956;L of 5 mM EDTA in 1xIB and transfer to a new tube.</li>
	<li>Centrifuge at 3,200 g in microcentrifuge for 5 min at 4 &#176;C and resuspend the pellet again in an appropriate volume of 2x Laemmli buffer supplemented with 10 mM EDTA. Place in boiling water bath for 10 min prior to analysis by SDS-PAGE. 
	Note: Integration of mature LHCP (mLHCP) is assessed by the appearance of a protease-protected degradation product (mLHCP-D) approximately 1.5-2 kDa smaller than the uncleaved mLHCP17.</li>
</ol>

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The authors have nothing to disclose.

Chloroplast and Thylakoid isolation
Excessive breakage can result in poor chloroplast isolation and thus poor thylakoid yield after separation in the gradient. It is best to homogenize the harvested tissue gently by ensuring that all material is submerged before blending and pulsing in 15 s cycles until fully homogenized. If necessary, use multiple shorter rounds of blending with less tissue in each round.
Refrigerating all materials that come into contact with harvest...

Nearly all of the proteinaceous machinery responsible for proper chloroplast function must be translocated from the cytosol1. At the chloroplast envelopes, protein substrates are imported through the translocon of the outer membrane (TOC) and the translocon of the inner membrane (TIC)2. Further targeting to the thylakoid membrane and lumen occurs through the twin arginine translocation (cpTat)3, the secretory (cpSec1)4, the signal recognition particle (cpSRP)5, and the spontaneous insertion pathways6. A method for the high-yield isolation of physiologically active chloroplasts and thylakoid membranes is necessary to measure the energetics and kinetics of a translocation event, to understand the diverse transport mechanisms in each pathway, and to localize a particular protein substrate of interest to any of the six distinct compartments of the chloroplast.
The isolation of membranes from the chloroplast offers better experimental control over environmental factors (such as salt and substrate concentrations, the presence of ATP/GTP, and pH conditions) that affect the measurement of transport energetics and kinetics. This in vitro environment lends itself to the exploration of mechanistic details of translocation for the same reasons. In addition, while predictive software for localization of chloroplast proteins has improved7,8, in vitro transport assays provide a quicker method for confirmation over microscopy-based fluorescent assays that require a genetically encoded fluorescent tag, plant transformation and/or specific antibodies. Here, we present protocols for chloroplast and thylakoid isolations from peas (Pisum sativum), as well as for transport assays optimized for each of the energy-dependent thylakoid translocation pathways.

<table border="0" cellpadding="0" cellspacing="0" style="width:1936px;" width="1936">
	<tbody>
		<tr height="21">
			<td height="21" style="height:21px;width:324px;">Pisum sativum seeds</td>
			<td style="width:252px;">Seedway LLC, Hall, NY</td>
			<td style="width:292px;">8686 - Little Marvel</td>
			<td style="width:1068px;"></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;">Miracloth</td>
			<td>Calbiochem, Gibbstown, NJ</td>
			<td>475855-1</td>
			<td></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;">80% Acetone</td>
			<td>Sigma, Saint Louis, MO</td>
			<td>67-64-1</td>
			<td></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;">Blender with sharpened blades</td>
			<td>Waring Commercial</td>
			<td>BB155S</td>
			<td></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;">Polytron 10-35</td>
			<td>Fischer Sci</td>
			<td>13-874-617</td>
			<td></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;">Percoll</td>
			<td>Sigma, Saint Louis, MO</td>
			<td>GE17-0891-01</td>
			<td></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;">Beckman J2-MC with JA 20 rotor</td>
			<td>Beckman-Coulter</td>
			<td>8043-30-1180</td>
			<td></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;">Sorvall RC-5B with HB-4 rotor</td>
			<td>Sorvall</td>
			<td>8327-30-1016</td>
			<td></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;">100 mM dithiothreitol (DTT) in 1xIB</td>
			<td>Sigma, Saint Louis, MO</td>
			<td>12/3/83</td>
			<td>Can be frozen in aliquots for future use</td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;">200 mM MgATP in 1xIB</td>
			<td>Sigma, Saint Louis, MO</td>
			<td>74804-12-9</td>
			<td>Can be frozen in aliquots for future use</td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;">Thermolysin in 1xIB (2mg/mL)</td>
			<td>Sigma, Saint Louis, MO</td>
			<td>9073-78-3</td>
			<td>Can be frozen in aliquots for future use</td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;">HEPES</td>
			<td>Sigma, Saint Louis, MO</td>
			<td>H3375</td>
			<td></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;">K-Tricine</td>
			<td>Sigma, Saint Louis, MO</td>
			<td>T0377</td>
			<td></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;">Sorbitol</td>
			<td>Sigma, Saint Louis, MO</td>
			<td>50-70-4</td>
			<td></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;">Magnesium Chloride</td>
			<td>Sigma, Saint Louis, MO</td>
			<td>7791-18-6</td>
			<td></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;">Manganese Chloride</td>
			<td>Sigma, Saint Louis, MO</td>
			<td>13446-34-9</td>
			<td></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;">EDTA</td>
			<td>Sigma, Saint Louis, MO</td>
			<td>60-00-4</td>
			<td></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;">BSA</td>
			<td>Sigma, Saint Louis, MO</td>
			<td>9048-46-8</td>
			<td></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;">Tris</td>
			<td>Sigma, Saint Louis, MO</td>
			<td>77-86-1</td>
			<td></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;">SDS</td>
			<td>Sigma, Saint Louis, MO</td>
			<td>151-21-3</td>
			<td></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;">Glycerol</td>
			<td>Sigma, Saint Louis, MO</td>
			<td>56-81-5</td>
			<td></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;">Bromophenol Blue</td>
			<td>Sigma, Saint Louis, MO</td>
			<td>115-39-9</td>
			<td></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;">B-Mercaptoethanol</td>
			<td>Sigma, Saint Louis, MO</td>
			<td>60-24-2</td>
			<td></td>
		</tr>
	</tbody>
</table>

isolation of physiologically active thylakoids and their use in energy-dependent protein transport assays

Chloroplasts are the organelles in green plants responsible for carrying out numerous essential metabolic pathways, most notably photosynthesis. Within the chloroplasts, the thylakoid membrane system houses all the photosynthetic pigments, reaction center complexes, and most of the electron carriers, and is responsible for light-dependent ATP synthesis. Over 90% of chloroplast proteins are encoded in the nucleus, translated in the cytosol, and subsequently imported into the chloroplast. Further protein transport into or across the thylakoid membrane utilizes one of four translocation pathways. Here, we describe a high-yield method for isolation of transport-competent thylakoids from peas (Pisum sativum), along with transport assays through the three energy-dependent cpTat, cpSec1, and cpSRP-mediated pathways. These methods enable experiments relating to thylakoid protein localization, transport energetics, and the mechanisms of protein translocation across biological membranes.

To gauge amount of substrate successfully transported, it is useful to include one or more &#34;percent input&#34; lanes. For the data presented below, 10% of the final transport reaction without thylakoids was used. This &#34;percent input&#34; also helps to visualize the size of the precursor substrate. The percentage represents a known, defined amount of substrate with which to compare transported substrate against and can be scaled up or down as necessary using initially prepared prot...

Watch this Scientific Journal Video about Isolation of Physiologically Active Thylakoids and Their Use in Energy-Dependent Protein Transport Assays at JoVE.com

Isolation of Physiologically Active Thylakoids and Their Use in Energy-Dependent Protein Transport Assays

We present protocols herein for high-yield isolation of physiologically active thylakoids and protein transport assays for the chloroplast twin arginine translocation (cpTat), secretory (cpSec1), and signal recognition particle (cpSRP) pathways.

Chloroplasts are the organelles in green plants responsible for carrying out numerous essential metabolic pathways, most notably photosynthesis. Within ...

isolation-physiologically-active-thylakoids-their-use-energy

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Biochemistry

10.7K Views.  University of California - Davis. We present protocols herein for high-yield isolation of physiologically active thylakoids and protein transport assays for the chloroplast twin arginine translocation (cpTat), secretory (cpSec1), and signal recognition particle (cpSRP) pathways.

Video: Isolation of Physiologically Active Thylakoids and Their Use in Energy-Dependent Protein Transport Assays

Synthesis of 1,2-Azaborines and the Preparation of Their Protein Complexes with T4 Lysozyme Mutants

We describe a general synthesis of 1,2-azaborines using standard air-free techniques and protein complex preparation with T4 lysozyme mutants by vapor diffusion. Oxygen- and moisture-sensitive compounds are prepared and isolated under an inert atmosphere (N2) using either a vacuum gas manifold or a glove box. As an example of azaborine synthesis, we demonstrate the synthesis and purification of the volatile N-H-B-ethyl-1,2-azaborine by a five-step sequence involving distillation and column chromatography for the isolation of products. T4 lysozyme mutants L99A and L99A/M102Q are expressed with Escherichia coli RR1 strain. Standard protocols for chemical cell lysis followed by purification using carboxymethyl ion exchange column affords protein of sufficiently high purity for crystallization. Protein crystallization is performed in various concentrations of precipitant at different pH ranges using the hanging drop vapor diffusion method. Complex preparation with the small molecules is carried out by vapor diffusion method under an inert atmosphere. X-ray diffraction analysis of the crystal complex provides unambiguous structural evidence of binding interactions between the protein binding site and 1,2-azaborines.

A protocol for the synthesis of 1,2-azaborines and the preparation of their protein complexes with T4 lysozyme mutants is presented.

We describe a general synthesis of 1,2-azaborines using standard air-free techniques and protein complex preparation with T4 lysozyme mutants by vapor ...

Analyzing Supercomplexes of the Mitochondrial Electron Transport Chain with Native Electrophoresis, In-gel Assays, and Electroelution

The mitochondrial electron transport chain (ETC) transduces the energy derived from the breakdown of various fuels into the bioenergetic currency of the cell, ATP. The ETC is composed of 5 massive protein complexes, which also assemble into supercomplexes called respirasomes (C-I, C-III, and C-IV) and synthasomes (C-V) that increase the efficiency of electron transport and ATP production. Various methods have been used for over 50 years to measure ETC function, but these protocols do not provide information on the assembly of individual complexes and supercomplexes. This protocol describes the technique of native gel polyacrylamide gel electrophoresis (PAGE), a method that was modified more than 20 years ago to study ETC complex structure. Native electrophoresis permits the separation of ETC complexes into their active forms, and these complexes can then be studied using immunoblotting, in-gel assays (IGA), and purification by electroelution. By combining the results of native gel PAGE with those of other mitochondrial assays, it is possible to obtain a completer picture of ETC activity, its dynamic assembly and disassembly, and how this regulates mitochondrial structure and function. This work will also discuss limitations of these techniques. In summary, the technique of native PAGE, followed by immunoblotting, IGA, and electroelution, presented below, is a powerful way to investigate the functionality and composition of mitochondrial ETC supercomplexes.

This protocol describes the separation of functional mitochondrial electron transport chain complexes (Cx) I-V and supercomplexes thereof using native electrophoresis to reveal information about their assembly and structure. The native gel can be subjected to immunoblotting, in-gel assays, and purification by electroelution to further characterize individual complexes.

The mitochondrial electron transport chain (ETC) transduces the energy derived from the breakdown of various fuels into the bioenergetic currency of the ...

Biochemical and Structural Characterization of the Carbohydrate Transport Substrate-binding-protein SP0092

Development of new antimicrobials and vaccines for Streptococcus pneumoniae (pneumococcus) are necessary to halt the rapid rise in multiple resistant strains. Carbohydrate substrate binding proteins (SBPs) represent viable targets for the development of protein-based vaccines and new antimicrobials because of their extracellular localization and the centrality of carbohydrate import for pneumococcal metabolism, respectively. Described here is a rationalized integrated protocol to carry out a comprehensive characterization of SP0092, which can be extended to other carbohydrate SBPs from the pneumococcus and other bacteria. This procedure can aid the structure-based design of inhibitors for this class of proteins. Presented in the first part of this manuscript are protocols for biochemical analysis by thermal shift assay, multi angle light scattering (MALS), and size exclusion chromatography (SEC), which optimize the stability and homogeneity of the sample directed to crystallization trials and so enhance the probability of success. The second part of this procedure describes the characterization of the SBP crystals using a tunable wavelength anomalous diffraction synchrotron beamline, and data collection protocols for measuring data that can be used to resolve the crystallized protein structure.

A streamlined protocol for performing an extensive biochemical and structural characterization of a carbohydrate substrate binding protein from Streptococcus pneumoniae is presented.

Development of new antimicrobials and vaccines for Streptococcus pneumoniae (pneumococcus) are necessary to halt the rapid rise in multiple resistant ...

Isolation and Respiratory Measurements of Mitochondria from Arabidopsis thaliana

Mitochondria are essential organelles involved in numerous metabolic pathways in plants, most notably the production of adenosine triphosphate (ATP) from the oxidation of reduced compounds such as nicotinamide adenine dinucleotide (NADH) and flavin adenine dinucleotide (FADH2). The complete annotation of the Arabidopsis thaliana genome has established it as the most widely used plant model system, and thus the need to purify mitochondria from a variety of organs (leaf, root, or flower) is necessary to fully utilize the tools that are now available for Arabidopsis to study mitochondrial biology. Mitochondria are isolated by homogenization of the tissue using a variety of approaches, followed by a series of differential centrifugation steps producing a crude mitochondrial pellet that is further purified using continuous colloidal density gradient centrifugation. The colloidal density material is subsequently removed by multiple centrifugation steps. Starting from 100 g of fresh leaf tissue, 2 - 3 mg of mitochondria can be routinely obtained. Respiratory experiments on these mitochondria display typical rates of 100 - 250 nmol O2 min-1 mg total mitochondrial protein-1 (NADH-dependent rate) with the ability to use various substrates and inhibitors to determine which substrates are being oxidized and the capacity of the alternative and cytochrome terminal oxidases. This protocol describes an isolation method of mitochondria from Arabidopsis thaliana leaves using continuous colloidal density gradients and an efficient respiratory measurements of purified plant mitochondria.

Isolation and Respiratory Measurements of Mitochondria from Arabidopsis thaliana

As mitochondria are only a small percentage of the plant cell, they need to be purified for a range of studies. Mitochondria can be isolated from a variety of plant organs by homogenization, followed by differential and density gradient centrifugation to obtain a highly purified mitochondrial fraction.

Mitochondria are essential organelles involved in numerous metabolic pathways in plants, most notably the production of adenosine triphosphate (ATP) from ...

Split-BioID &#8212; Proteomic Analysis of Context-specific Protein Complexes in Their Native Cellular Environment

To complement existing affinity purification (AP) approaches for the identification of protein-protein interactions (PPI), enzymes have been introduced that allow the proximity-dependent labeling of proteins in living cells. One such enzyme, BirA* (used in the BioID approach), mediates the biotinylation of proteins within a range of approximately 10 nm. Hence, when fused to a protein of interest and expressed in cells, it allows the labeling of proximal proteins in their native environment. As opposed to AP that relies on the purification of assembled protein complexes, BioID detects proteins that have been marked within cells no matter whether they are still interacting with the protein of interest when they are isolated. Since it biotinylates proximal proteins, one can moreover capitalize on the exceptional affinity of streptavidin for biotin to very efficiently isolate them. While BioID performs better than AP for identifying transient or weak interactions, both AP- and BioID-mass spectrometry approaches provide an overview of all possible interactions a given protein may have. However, they do not provide information on the context of each identified PPI. Indeed, most proteins are typically part of several complexes, corresponding to distinct maturation steps or different functional units. To address this common limitation of both methods, we have engineered a protein-fragments complementation assay based on the BirA* enzyme. In this assay, two inactive fragments of BirA* can reassemble into an active enzyme when brought in close proximity by two interacting proteins to which they are fused. The resulting split-BioID assay thus allows the labeling of proteins that assemble around a pair of interacting proteins. Provided these two only interact in a given context, split-BioID then allows the analysis of specific context-dependent functional units in their native cellular environment. Here, we provide a step-by-step protocol to test and apply split-BioID to a pair of interacting proteins.

We provide a step-by-step protocol for split-BioID, a protein fragments-complementation assay based on the proximity-labeling technique BioID. Activated on the interaction of two given proteins, it allows the proteomics analysis of context-dependent protein complexes in their native cellular environment. The method is simple, cost-effective and only requires standard laboratory equipment.

To complement existing affinity purification (AP) approaches for the identification of protein-protein interactions (PPI), enzymes have been introduced ...

Use of Recombinant Fusion Proteins in a Fluorescent Protease Assay Platform and Their In-gel Renaturation

Proteases are intensively studied enzymes due to their essential roles in several biological pathways of living organisms and in pathogenesis; therefore, they are important drug targets. We have developed a magnetic-agarose-bead-based assay platform for the investigation of proteolytic activity, which is based on the use of recombinant fusion protein substrates. In order to demonstrate the use of this assay system, a protocol is presented on the example of human immunodeficiency virus type 1 (HIV-1) protease. The introduced assay platform can be utilized efficiently in the biochemical characterization of proteases, including enzyme activity measurements in mutagenesis, kinetic, inhibition, or specificity studies, and it may be suitable for high-throughput substrate screening or may be adapted to other proteolytic enzymes.
In this assay system, the applied substrates contain N-terminal hexahistidine (His6) and maltose-binding protein (MBP) tags, cleavage sites for tobacco etch virus (TEV) and HIV-1 proteases, and a C-terminal fluorescent protein. The substrates can be efficiently produced in Escherichia coli cells and easily purified using nickel (Ni)-chelate-coated beads. During the assay, the proteolytic cleavage of bead-attached substrates leads to the release of fluorescent cleavage fragments, which can be measured by fluorimetry. Additionally, cleavage reactions can be analyzed by sodium dodecyl sulfate-polyacrylamide gel electrophoresis (SDS-PAGE). A protocol for the in-gel renaturation of assay components is also described, as partial renaturation of fluorescent proteins enables their detection based on molecular weight and fluorescence.

Here, we present the detailed procedure of a recently developed protease assay platform utilizing N-terminal hexahistidine/maltose-binding protein and fluorescent protein-fused recombinant substrates attached to the surface of nickel-nitrilotriacetic acid magnetic agarose beads. A subsequent in-gel analysis of the assay samples separated by sodium dodecyl sulfate-polyacrylamide gel electrophoresis is also presented.

Proteases are intensively studied enzymes due to their essential roles in several biological pathways of living organisms and in pathogenesis; therefore, ...

Analysis of Protein Folding, Transport, and Degradation in Living Cells by Radioactive Pulse Chase

Radioactive pulse-chase labeling is a powerful tool for studying the conformational maturation, the transport to their functional cellular location, and the degradation of target proteins in live cells. By using short (pulse) radiolabeling times (&lt;30 min) and tightly controlled chase times, it is possible to label only a small fraction of the total protein pool and follow its folding. When combined with nonreducing/reducing SDS-polyacrylamide gel electrophoresis (SDS-PAGE) and immunoprecipitation with (conformation-specific) antibodies, folding processes can be examined in great detail. This system has been used to analyze the folding of proteins with a huge variation in properties such as soluble proteins, single and multi-pass transmembrane proteins, heavily N- and O-glycosylated proteins, and proteins with and without extensive disulfide bonding. Pulse-chase methods are the basis of kinetic studies into a range of additional features, including co- and posttranslational modifications, oligomerization, and polymerization, essentially allowing the analysis of a protein from birth to death. Pulse-chase studies on protein folding are complementary with other biochemical and biophysical methods for studying proteins in vitro by providing increased temporal resolution and physiological information. The methods as described within this paper are adapted easily to study the folding of almost any protein that can be expressed in mammalian or insect-cell systems.

Here we describe a protocol for a general pulse-chase method that allows the kinetic analysis of folding, transport, and degradation of proteins to be followed in live cells.

Radioactive pulse-chase labeling is a powerful tool for studying the conformational maturation, the transport to their functional cellular location, and ...

In Vitro Ubiquitination and Deubiquitination Assays of Nucleosomal Histones

Ubiquitination is a post-translational modification that plays important roles in various signaling pathways and is notably involved in the coordination of chromatin function and DNA-associated processes. This modification involves a sequential action of several enzymes including E1 ubiquitin-activating, E2 ubiquitin-conjugating and E3 ubiquitin-ligase and is reversed by deubiquitinases (DUBs). Ubiquitination induces degradation of proteins or alteration of protein function including modulation of enzymatic activity, protein-protein interaction and subcellular localization. A critical step in demonstrating protein ubiquitination or deubiquitination is to perform in vitro reactions with purified components. Effective ubiquitination and deubiquitination reactions could be greatly impacted by the different components used, enzyme co-factors, buffer conditions, and the nature of the substrate.&#160; Here, we provide step-by-step protocols for conducting ubiquitination and deubiquitination reactions. We illustrate these reactions using minimal components of the mouse Polycomb Repressive Complex 1 (PRC1), BMI1, and RING1B, an E3 ubiquitin ligase that monoubiquitinates histone H2A on lysine 119. Deubiquitination of nucleosomal H2A is performed using a minimal Polycomb Repressive Deubiquitinase (PR-DUB) complex formed by the human deubiquitinase BAP1 and the DEUBiquitinase ADaptor (DEUBAD) domain of its co-factor ASXL2. These ubiquitination/deubiquitination assays can be conducted in the context of either recombinant nucleosomes reconstituted with bacteria-purified proteins or native nucleosomes purified from mammalian cells. We highlight the intricacies that can have a significant impact on these reactions and we propose that the general principles of these protocols can be swiftly adapted to other E3 ubiquitin ligases and deubiquitinases.

Ubiquitination is a post-translational modification that plays important roles in cellular processes and is tightly coordinated by deubiquitination. Defects in both reactions underlie human pathologies. We provide protocols for conducting ubiquitination and deubiquitination reaction in vitro using purified components.

Ubiquitination is a post-translational modification that plays important roles in various signaling pathways and is notably involved in the coordination ...

Application of Biolayer Interferometry (BLI) for Studying Protein-Protein Interactions in Transcription

A transcription factor&#160;(TF) is a protein that regulates gene expression by interacting with the RNA polymerase, another TF, and/or template DNA. GrgA is a novel transcription activator found specifically in the obligate intracellular bacterial pathogen Chlamydia. Protein pulldown assays using affinity beads have revealed that GrgA binds two &#963; factors, namely &#963;66 and &#963;28, which recognize different sets of promoters for genes whose products are differentially required at developmental stages. We have used BLI to confirm and further characterize the interactions. BLI demonstrates several advantages over pulldown: 1) It reveals real-time association and dissociation between binding partners, 2) It generates quantitative kinetic parameters, and 3) It can detect bindings that pulldown assays often fail to detect. These characteristics have enabled us to deduce the physiological roles of GrgA in gene expression regulation in Chlamydia, and possible detailed interaction mechanisms. We envision that this relatively affordable technology can be extremely useful for studying transcription and other biological processes.

Application of Biolayer Interferometry BLI for Studying Protein-Protein Interactions in Transcription

Interactions of transcription factors (TFs) with the RNA polymerase are usually studied using pulldown assays. We apply a Biolayer Interferometry (BLI) technology to characterize the interaction of GrgA with the chlamydial RNA polymerase. Compared to pulldown assays, BLI detects real-time association and dissociation, offers higher sensitivity, and is highly quantitative.

A transcription factor&#160;(TF) is a protein that regulates gene expression by interacting with the RNA polymerase, another TF, and/or template DNA. GrgA ...

Use of Microscale Thermophoresis to Measure Protein-Lipid Interactions

The ability to determine the binding affinity of lipids to proteins is an essential part of understanding protein-lipid interactions in membrane trafficking, signal transduction and cytoskeletal remodeling. Classic tools for measuring such interactions include surface plasmon resonance (SPR) and isothermal titration calorimetry (ITC). While powerful tools, these approaches have setbacks. ITC requires large amounts of purified protein as well as lipids, which can be costly and difficult to produce. Furthermore, ITC as well as SPR are very time consuming, which could add significantly to the cost of performing these experiments. One way to bypass these restrictions is to use the relatively new technique of microscale thermophoresis (MST). MST is fast and cost effective using small amounts of sample to obtain a saturation curve for a given binding event. There currently are two types of MST systems available. One type of MST requires labeling with a fluorophore in the blue or red spectrum. The second system relies on the intrinsic fluorescence of aromatic amino acids in the UV range. Both systems detect the movement of molecules in response to localized induction of heat from an infrared laser. Each approach has its advantages and disadvantages. Label-free MST can use untagged native proteins; however, many analytes, including pharmaceuticals, fluoresce in the UV range, which can interfere with determination of accurate KD values. In comparison, labeled MST allows for a greater diversity of measurable pairwise interactions utilizing fluorescently labeled probes attached to ligands with measurable absorbances in the visible range as opposed to UV, limiting the potential for interfering signals from analytes.

Microscale thermophoresis obtains binding constants quickly at low material cost. Either labeled or label free microscale thermophoresis is commercially available; however, label free thermophoresis is not capable of the diversity of interaction measurements that can be performed using fluorescent labels. We provide a protocol for labeled thermophoresis measurements.

Isolation of Physiologically Active Thylakoids and Their Use in Energy-Dependent Protein Transport Assays

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Rozdziały w tym wideo

Synthesis of 1,2-Azaborines and the Preparation of Their Protein Complexes with T4 Lysozyme Mutants

Analyzing Supercomplexes of the Mitochondrial Electron Transport Chain with Native Electrophoresis, In-gel Assays, and Electroelution

Biochemical and Structural Characterization of the Carbohydrate Transport Substrate-binding-protein SP0092

Isolation and Respiratory Measurements of Mitochondria from Arabidopsis thaliana

Split-BioID — Proteomic Analysis of Context-specific Protein Complexes in Their Native Cellular Environment

Use of Recombinant Fusion Proteins in a Fluorescent Protease Assay Platform and Their In-gel Renaturation

Analysis of Protein Folding, Transport, and Degradation in Living Cells by Radioactive Pulse Chase

In Vitro Ubiquitination and Deubiquitination Assays of Nucleosomal Histones

Application of Biolayer Interferometry (BLI) for Studying Protein-Protein Interactions in Transcription

Use of Microscale Thermophoresis to Measure Protein-Lipid Interactions