This work is supported by the National Institutes of Health (NIH) grants R01DK093953 (X.L.), P30NS069271, BRFSG-2014-07 (X.L.). C.J. is partially supported by American Heart Associate pre-doctoral fellowship (14PRE20380168, to C.J.).

1. Membrane Sheet Preparation and Fixation
<ol>
	<li>Prepare membrane sheets labeled with iRFP-PAmCherry1-PHPLC&#948;1
	<ol>
		<li>Prepare the DNA plasmid encoding iRFP-PAmCherry1-PHPLC&#948;123 using standard molecular biology techniques.</li>
		<li>Culture INS-1 cells on #1.5 18 mm round coverslips pre-coated with 30 &#181;g/ml fibronectin to 50-70% confluency following standard INS-1 cell culture protocols38,39. Transfect the cells a day after 50 to 70% confluency is reached.</li>
		<li>Transfect cells with iRFP-PAmCherry1-PHPLC&#948;1 using liposome transfection reagent following manufacturer&#39;s protocols. After transfection, allow the cells to grow for 48 hr.</li>
		<li>On the day of the experiment, coat coverslips (on one-side) with ~0.5 - 1 ml of 500 &#181;g/ml Poly-D-Lysine (PDL; diluted in dH2O) for 1-2 hr. Then drain PDL by placing a tissue paper on the edge of the coverslip. Place the coverslips on a pre-chilled (4 &#176;C) metal plate for later use.</li>
		<li>Wash pre-transfected INS-1 cells growing on coverslips with ~0.5 - 1 ml ice-cold phosphate-buffered saline (PBS) containing 1 mM EGTA. Repeat the wash three times and drain PBS.</li>
		<li>Place the coverslips with cultured cells (cell-side facing down) on the PDL-coated coverslips on a pre-chilled metal plate with a pair of tweezers. Leave the plate in a refrigerator (4 &#176;C) for 7 - 10 min to allow cells to attach to the PDL-coated coverslips (Figure 2). 
		NOTE: The incubation time should be in the range of 7 - 10 min for better attachment of the cells to the PDL-coated surface. The refrigerator environment is dry and incubation should not be too long.</li>
		<li>Remove the metal plate from the refrigerator. Gently peel off the coverslip containing the pre-transfected cells using tweezers. This produces a thin layer of cell membrane sheet on the PDL-coated coverslip. Gently wash the membrane sheets with ~0.5 - 1 ml ice-cold PBS and then fix with ~0.5 - 1 ml ice-cold 4% paraformaldehyde (PFA) + 0.2% glutaraldehyde (GA) in PBS for 15 min at 4 &#176;C. 
		Caution: Paraformaldehyde and glutaraldehyde are toxic. Handle them in a fume hood with skin and eye protection.</li>
		<li>After fixation, image the membrane sheets immediately (see section 3) or store in ~0.5 - 1 ml PBS at 4 &#176;C. 
		NOTE: After fixing the membrane sheet, there will be no equilibrium binding of PH probes from cytosol to PI(4,5)P2. The bound PH probes will gradually dissociate from the membrane sheet and diffuse into the solution (although it might take days to weeks). Therefore, it is recommended to image the fixed samples right after sample preparation.</li>
	</ol>
	</li>
	<li>Prepare membrane sheets for PI(4,5)P2 specific antibody labeling
	<ol>
		<li>Culture INS-1 cells on #1.5, 18 mm round coverslips pre-coated with 30 &#181;g/ml fibronectin to 50%-70% confluence. Transfect cells with DNA plasmid the next day as described in step 1.1.3.</li>
		<li>Repeat steps from 1.1.4 to 1.1.7 as described above. 
		NOTE: Perform the following procedures at 4 &#176;C.</li>
		<li>Wash the coverslips containing fixed PM sheets three times with ~0.5 - 1 ml ice-cold PBS containing 50 mM NH4Cl. Quench the sheets with ~0.5 - 1 ml 0.1% sodium borohydride in PBS for 7 min, and wash with ~0.5 - 1 ml PBS (without 50 mM NH4Cl).</li>
		<li>Block the samples with ~0.5 - 1 ml blocking solution (PBS solution containing 5% (v/v) normal goat serum, 5% (v/v) bovine serum albumin and 50 mM NH4Cl) for 45 min. Then, incubate with ~0.5 - 1 ml primary PI(4,5)P2 antibody (1:300 dilution) in blocking solution for 1 hr. Wash three times (10 min each time) with ~0.5 - 1 ml PBS containing 50 mM NH4Cl.</li>
		<li>Incubate samples with ~0.5 - 1 ml secondary F(ab&#39;)2-goat-anti-mouse antibody conjugated with fluorophores (1:300) in blocking buffer for 1 hr. Wash three times with ~0.5 - 1 ml PBS.</li>
		<li>Post-fix samples with 4% PFA + 0.2% GA for 15 min, then wash samples three times with PBS (7 min each time). Proceed to Section 3 for imaging or store in ~0.5 ~ 1 ml PBS at 4 &#176;C for later use. 
		NOTE: Prepare samples at 4 &#176;C. Use 4% PFA + 0.2% GA fixative to preserve the physiological distribution of phosphoinositides in the PM. RT preparation or fixation with 4% PFA alone may cause significant artifacts (Figure 4).</li>
	</ol>
	</li>
</ol>
2. Cell Culture Preparation for Live-cell Imaging with mEOS3.1-PHPLC&#948;1
<ol>
	<li>Prepare the DNA plasmid encoding the mEOS3.1-PHPLC&#948;1 as described previously 23.</li>
	<li>Culture INS-1 cells on #1.5 18 mm round coverslips pre-coated with 30 &#181;g/ml fibronectin until they reach 50%-70% confluency following standard INS-1 cell culture protocols38,39.</li>
	<li>The following day, transfect INS-1 cells with the mEOS3.1-PHPLC&#948;1 DNA plasmid using liposome transfection reagent following manufacture&#39;s protocol. Incubate for 48 hr before imaging.</li>
</ol>
3. PALM Image Acquisition of Membrane Sheets and Live Cells
<ol>
	<li>PALM image acquisition of membrane sheets 
	NOTE: Here, a total internal reflection fluorescence (TIRF) microscope based SMLM system (100X oil, APO, NA = 1.49, WD 0.12 mm) 23 is used for all image acquisition.
	<ol>
		<li>Before imaging, dilute 1 &#181;l of fluorescent bead solution in 10 ml PBS + 50 mM MgCl2. Add 200 &#181;l diluted solution into the imaging chamber containing cell samples (from steps 1.1.8/1.2.6) for 10 min. Then, wash with PBS three times.</li>
		<li>Start the PALM imaging system. In the associated imaging software, select the &#34;iRFP channel&#34; button (642 nm laser excitation, 700/75 nm emission). Find the cell membrane expressing PH probes in the iRFP channel. 
		NOTE: The membrane sheet should have a fluorescent bead nearby. This is required for drift correction later.</li>
		<li>Use the &#34;Capture&#34; button to collect a conventional TIRF image of the cell membrane in iRFP channel as a reference for future image reconstruction. Set a normal TIRF angle (i.e., after reaching the critical angle, turn another 1.5 degrees) by typing in 2140 in the TIRF angle setting for imaging. Use this angle setting for all steps unless otherwise noted. 
		NOTE: In the TIRF system described here, 3,500 is the vertical up angle, 2,200 is the TIRF critical angle, and 2140 is the normal TIRF angle, which is 1.5 degree more after TIRF critical angle. The narrow TIRF angle mentioned below in 3.2.3 is 2120, which is another 2 degree after reaching TIRF critical angle.</li>
		<li>Switch to PAmCherry1 channel by clicking the RFP channel button (561 nm excitation, 600/50 nm emission filter). Adjust the scroll bar in the &#34;AOTF&#34; pad all the way to the right to have full power illumination of 561 nm laser for 10-20 sec to bleach the background membrane fluorescence.</li>
		<li>Set the optimal camera setting (2x2 binning) in the &#34;Format&#34; tab and the fast acquisition protocol in &#34;ND sequence acquisition&#34; tab (typically 10,000-40,000 images at 20 Hz).</li>
		<li>Start acquisition of PAmCherry1 images (561 nm laser at full power, 50 msec/frame) with simultaneous 405 nm laser activation at a low level (0.1% - 1%) by clicking the &#34;Run now&#34; button. Adjust the intensity of 405 nm laser so that spatially isolated individual points in each frame are easily identifiable. 
		NOTE: The number of activatable PAmCherry1 molecules decreases gradually during acquisition. 405 nm laser intensity should be gradually increased to keep the optimal density of individual molecule signals in each frame.</li>
		<li>Continue acquiring images until no PAmCherry1 single molecule signal is activated.</li>
	</ol>
	</li>
	<li>PALM imaging in live cells
	<ol>
		<li>Before imaging, dilute fluorescent beads into the imaging chamber for 10 min as described in step 3.1.1. Then start PALM imaging by opening the associated imaging software. 
		NOTE: Use a magnetic quick-release imaging chamber for live-cell imaging. Maintain the center of the imaging field at 35 &#176;C with a temperature controller under constant perfusion with extracellular buffer (Extracellular Solution: 135 mM NaCl, 5.6 mM KCl, 2.6 mM CaCl2, 1.2 mM MgCl2, 3 mM glucose, and 20 mM HEPES; pH =7.3).</li>
		<li>Choose the GFP channel button (525/50 nm emission). Identify the cell membrane expressing fluorescent probes based on green fluorescent from mEOS3 under 488 nm laser excitation. Make sure that fluorescent beads nearby are also included during imaging as this is required later for offline drift correction.</li>
		<li>Click the &#34;Capture&#34; button to collect a TIRF image of the cell membrane in mEOS3 (green) channel as a reference image. Use a shallow evanescent wave excitation illumination (after reaching the critical angle, turn another 2 degrees) by typing in 2120 in the TIRF angle setting for live-cell imaging. 
		NOTE: This minimizes the fluorescence from the unbound mEos3-PH in the cytosol adjacent to the plasma membrane.</li>
		<li>Switch to the &#34;RFP channel&#34; button (561 nm excitation, 600/50 nm emission). Use the full power 561 nm laser to bleach background fluorescence of the membrane sheets for 10 ~ 20 sec with the scrollbar in the &#34;AOTF pad&#34; (see 3.1.4).</li>
		<li>Start image acquisition by clicking the &#34;Run Now&#34; button in the red channel (561 nm full power, set at 10 msec/frame in the &#34;camera&#34; setting tab) with simultaneous 405 nm laser activation. Adjust the 405 nm laser intensity to activate spatially separated points in each frame. 
		NOTE: As acquisition proceeds, un-converted mEOS3.1-PHPLC&#948;1 molecule number slowly decreases. Gradually increase the 405 nm laser power to optimize the single molecule signal. The imaging acquisition length depends on the experimental purpose. Acquire images continuously for 5 min under normal conditions. If a longer acquisition is required, collect multiple image stacks instead of a single, large image stack. The file size of each image stack should not exceed 4 GB or it will affect software analysis later.</li>
	</ol>
	</li>
</ol>
4. SMLM Image Processing and Reconstruction
<ol>
	<li>Transfer the image files (.tif image stacks) to an image analysis station. Launch the image reconstruction program (custom-written) in Matlab as described previously37 and load the image stack by clicking the &#34;File&#34; tab in the main menu, then &#34;open&#34;, then &#34;new file&#34;.</li>
	<li>Identify and localize individual molecular events from each frame. Set filtering intensity threshold with a threshold number (1-10) in the &#34;wavelet&#34;. Verify the optimal parameter settings for point detection visually before the reconstruction. Then go to the &#34;PALM&#34; tab and click &#34;one step process&#34; to start image reconstruction. 
	NOTE: Intensity threshold for point detection is arbitrary and depends on personal experience. Several trials may be required to generate an optimal detection threshold that neither picks up too many unqualified (dim) points nor filters out too many qualified (bright) points. Adjust other parameters to optimize data analysis. Here, neighborhood distance (fluorescence points in the neighboring frames within a distance are combined) is set as 65 nm (1/2 pixel width) and fitted as a single molecule. Gap frames (individual molecule events that occurred within these frames and neighborhood distance were combined and fitted as a single molecule event) is set as 26 frames (1.3 sec) for PAmCherry1 imaging40. Adjust these parameter according to the properties of single molecule probes and acquisition rate to avoid over-counting40 in SMLM. Apply drift correction with fluorescent beads during the reconstructions.
	<ol>
		<li>For imaging the fixed membrane sheets labeled by iRFP-PAmCherry1-PHPLC&#948;1, reconstruct the whole image stacks from the same membrane sheet into a single super-resolution image37.</li>
		<li>For live cell samples labeled by mEOS3.1-PHPLC&#948;1, separate the whole image stack into several smaller stacks of 1,000 frames so that 1,000-consecutive-frame stack is reconstructed as a single super-resolution image, which has a temporal resolution of 10 sec. In the end, combine all the time series images into the final time series stack23. 
		NOTE: In live-cell PALM imaging, a small number of activated probes may move or dissociate from PI(4,5)P2 in the PM before bleaching. To account for the oversampling of the probes, combine individual molecule signals in the neighboring frames within 130 nm (instead of 65 nm) into a single emission event during image analysis.</li>
	</ol>
	</li>
	<li>After obtaining the reconstructed images, carry out further image analysis with the custom-written program in Matlab to quantify molecule density, micro-domain density/size, and cluster analysis with pair-correlation41.</li>
</ol>

The authors have nothing to disclose.

For troubleshooting, two processes need extra attention: membrane sheet production and sample fixation. As described in the protocol, the incubation time of the coverslips in step 1.1.6 is important for membrane sheet production. Optimal incubation time under our experimental condition is 7-10 min (Figure 2). Longer than 10 min incubation will produce intact cells instead of the membrane sheets on PDL coverslips and shorter incubation will lead to less or no membrane sheets on the PDL-coated coverslips. As described in the protocol, the fixatives and temperature during fixation are critical for maintaining the PI(4,5)P2 distribution in the PM. Fixation at RT or use of 4%-PFA alone could distort the normal lipid distribution in the PM.
By applying PALM microscopy to membrane lipid research, we are able to observe the nanometer scale distribution of PI(4,5)P2, a key phosphoinositide that mediates many fundamental cellular activities. This spatial distribution of PI(4,5)P2 with limited concentration gradients in INS-1 cells provides a framework for rethinking lipid-protein interactions and local signaling events of PI(4,5)P2 in these cells. Moreover, the methods developed in this work can also be applied to other membrane phospholipid research with proper probes, thereby, offering novel tools to study phosphoinositides in biological processes.
The use of membrane sheets in this work bypasses two major concerns in phospholipid morphological studies: detergent treatment and potential signal contamination from the cytosol. Detergents often cause clustering and significant loss of PM phospholipid signal. The contamination of cytosolic signal is particularly problematic in the case of low abundance phosphoinositides on the PM23, such as PI(3,4,5)P3 and PI(3,4)P2. Membrane sheet samples are able to circumvent these problems without significantly disrupting structures associated with the plasma membrane, such as cortical actin meshwork and clathrin-coated pits42,43. The relative homogenous distribution of PI(4,5)P2 in the PM is in good agreement with other quick freezing EM studies using GST-PHPLC&#948;1 probes in the fibroblast membrane44.
It is important to note that improper sample processing conditions can generate misleading results. First, it is critical to perform the fixation steps at a lower temperature (4 &#176;C) and use the fixative GA for membrane sheet production. As shown in Figure 3, warm temperature and PFA fixation without GA is not sufficient to fix phosphoinositides in cell PM. This could distort the intact PI(4,5)P2 distribution and generate sharp clusters that are not observed in live cells under physiological conditions. Second, the use of PAmCherry1 as the SMLM probe, rather than other probes, is pivotal for quantitative PALM imaging. The benefit of PAmCherry1 application comes from its well-characterized single molecular photo-physical properties35,40,45, such as brightness, high photo-activation efficiency and most of all, very limited photo-blinking. These properties enable us to eliminate potential cluster artifacts from photo-blinking and quantitatively analyze the molecular density of membrane PI(4,5)P2.
This approach also has its limitations. First, the membrane sheet method used in this study may not fully mimic the physiological distribution of PI(4,5)P2 because the cell is disrupted before imaging. However, our live PALM imaging shows similar relatively homogeneous distribution of PI(4,5)P2, supporting the results observed with membrane sheet samples. Second, as we discussed in our previous work23, SMLM requires imaging expertise and extra attention to avoid imaging artifacts that might arise from different processes, including the probes used, sample preparation and fixation, image sampling and reconstruction. Lastly, though the PH domain based probes and antibodies have been widely used in phosphoinositide studies46,47 it remains possible that not all PI(4,5)P2 in the membrane can be detected by this approach. For example, PI(4,5)P2 bound by other endogenous proteins may not be accessible to PH probes or antibodies, and this may cause an underestimation of PI(4,5)P2 due to the space hindrance of probe themselves. An alternative way of labeling PI(4,5)P2 would be using Top-Fluor PI(4,5)P248, a pre-labeled PI(4,5)P2 analog with a modification on the tail of original PI(4,5)P2. However, it can be converted rapidly into other phosphoinositide subtypes by fast live cell metabolism since its inositol ring is the same as endogenous PI(4,5)P2. This raises the concern whether this pre-labeled PI(4,5)P2 analog in live cells can faithfully represent PI(4,5)P2 rather than its metabolic products. Therefore, despite some limitations, PH domain based probes are still among the best probes that have been widely used to monitor PI(4,5)P2 distribution and dynamics on the PM of cells.
The future application of this methodology can be extended to other phosphoinositide studies, such as PI(3,4,5)P3 and PI(3,4)P2. In summary, the novel SMLM approach used here opens new ways to study phosphoinositide in cells. Using PI(4,5)P2 as an example, we demonstrate the unique properties of PALM imaging in the morphological and quantitative study of cell membrane molecules, as well as its drawbacks. This approach can be adapted to other molecules of interests and will have wide applications in cell biology.

Phosphoinositides contribute to a small portion of total membrane lipids, but play critical roles in a variety of cellular processes. They include seven members derived from reversible phosphorylation or dephosphorylation of the inositol rings on the 3rd, 4th and 5th positions1. Phosphatidylinositol 4-phosphate (PI4P) and phosphatidylinositol 4,5-bisphosphate (PI(4,5)P2) are two major phosphoinositides that function relatively independently as the determinant lipids of cell plasma membrane (PM) 2,3. Phosphatidylinositol (3,4,5)-trisphosphate (PIP3) is much less abundant than PI4P and PI(4,5)P2, but it has unique functions in different cellular processes including cancer4 and diabetes5. These lipids have complex molecular interactions with their effectors and many other proteins. Therefore, it is crucial to understand the spatial organization of these phosphoinositides in the PM at the nanometer scale.
Mounting evidence has shown that protein complexes or molecule clusters in the confined PM areas can serve as signaling hotspots6. For example, syntaxin 1a, a key protein that regulates membrane fusion7-9, displays cluster organization in the PM. Distinct from the consensus view of the cluster organization of syntaxin 1a, the spatial distribution of phosphoinositides in the PM is controversial. PI(4,5)P2 distribution patterns range from uniform10-12, large patches13,14, to dense clusters14-18, depending on cell types and experimental methods used. The spatial organization of PI(4,5)P2 at higher resolution is also inconsistent. A study using stimulated-emission-depletion (STED) microscopy 19 has revealed a large number of dense PI(4,5)P2 nano-clusters (~73 nm in diameter) in the PM sheets of PC-12 cells 20. This result is different from studies using quick freezing electron microscopy (EM)21,22, an approach that preserves the intact PM structure of live cells much better than chemical fixation. The latter showed distinct pools of PI(4,5)P2; relatively concentrated PI(4,5)P2 in caveolae and coated pits as well as uniform distribution on the flat PM region. Moreover, nanoscale PI(4,5)P2 organization in membrane sheets may differ in live and fixed cells. Our recent work investigated this issue in both fixed and live INS-1 cells using single-molecule localization microscopy (SMLM)23.
SMLM is based on stochastically switching on only a small subset of fluorophores at any given time so that individual fluorophores can be localized with high precision. Many super-resolution imaging approaches have been developed using similar principles to surpass the diffraction limit of conventional light microscopy, such as photoactivation localization microscopy (PALM)24, fluorescence photoactivation localization microscopy (FPALM)25, stochastic optical reconstruction microscopy (STORM)26,27 and direct STORM (dSTORM)28. With photo-switchable or photoactivatable fluorophores (dyes or fluorescent proteins), SMLM techniques allow scientists to image biological structures at nanometer resolution24,29,30 with video-rate in living cells31,32.
Using PI(4,5)P2 as an example, we introduced the SMLM approach to study the nanoscale distribution of phosphoinositides on the PM. The PH domain of PLC&#948;1 (Phospholipase C &#948;1) that specifically binds to PI(4,5)P2 is a well-established probe for imaging PI(4,5)P2 sub-cellular distribution and dynamics33,34 in the PM. We have genetically tagged this domain with two fluorescent proteins, PAmCherry135 and iRFP36 to produce a dual-color fusion protein (iRFP-PAmCherry1-PHPLC&#948;1) (Figure 1A-B). PAmCherry1 serves as the photoactivatable probe of PH domain for PALM and iRFP serves as a general indicator to identify transfected cells before PALM acquisition. We apply this dual-color fluorescent probe for SMLM imaging in the fixed membrane sheets. For live PALM imaging, we tagged mEOS337 instead of PAmCherry1 to the PHPLC&#948;1 domain to generate the mEOS3.1-PHPLC&#948;1 probe for its better photon efficiency and brightness (Figure 1C-D).
SMLM imaging with these novel probes in the PM of insulin-secreting INS-1 cells38 has uncovered homogeneous labeling of PI(4,5)P2 in the majority of the PM regions as well as concentrated PI(4,5)P2 microdomains that are sparsely intermixed in the flat PM and some filopodia-like structures23. The nanoscale distribution of PI(4,5)P2 provides a structural base for rethinking how it functions in living cells.

<table border="0" cellpadding="0" cellspacing="0" width="791">
	<colgroup>
		<col />
		<col />
		<col />
		<col />
	</colgroup>
	<tbody>
		<tr height="21">
			<td height="21" style="height:21px;width:216px;">Microscope</td>
			<td style="width:199px;">Nikon</td>
			<td style="width:184px;">Ti-U</td>
			<td style="width:193px;"></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:216px;">sCMOS camera</td>
			<td style="width:199px;">Andor</td>
			<td style="width:184px;">Neo</td>
			<td></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:216px;">Spinning disk</td>
			<td style="width:199px;">Yokogawa</td>
			<td style="width:184px;">CSU X-1, 10,000 rpm&#160;</td>
			<td></td>
		</tr>
		<tr height="147">
			<td height="147" style="height:147px;width:216px;">&#160;High Power Monolithic Laser Combiner SP with 405, 488, 561 and 642 nm lasers.</td>
			<td style="width:199px;">Agilent</td>
			<td style="width:184px;">MLC400</td>
			<td style="width:193px;">laser original powers &#38; powers at the end of optical fiber) 
			405nm: 15 mW &#38; 13 mW; 
			488nm: 45 mW &#38; 42 mW; 
			561nm: 45 mW &#38; 40 mW; 
			640nm: 35 mW &#38; 16 mW.</td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:216px;">100X Objective</td>
			<td style="width:199px;">Nikon</td>
			<td style="width:184px;"></td>
			<td>APO 100X Oil, NA 1.49, WD 0.12mm&#160;</td>
		</tr>
		<tr height="42">
			<td height="42" style="height:42px;width:216px;">Nikon acquisition and analysis software(NIS Element)</td>
			<td style="width:199px;">Nikon</td>
			<td style="width:184px;"></td>
			<td></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:216px;">Matlab</td>
			<td style="width:199px;">MathWorks</td>
			<td style="width:184px;"></td>
			<td></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:216px;">Coverslip</td>
			<td style="width:199px;">Warner</td>
			<td style="width:184px;">64-0714</td>
			<td>Round 18mm coverslip, #1.5&#160;</td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:216px;">Fibronectin</td>
			<td style="width:199px;">Millipore</td>
			<td style="width:184px;">FC010-5MG</td>
			<td></td>
		</tr>
		<tr height="41">
			<td height="41" style="height:41px;width:216px;">Lipofectamin 3000(transfection reagent)</td>
			<td style="width:199px;">Invitrogen</td>
			<td style="width:184px;">L3000-008</td>
			<td></td>
		</tr>
		<tr height="41">
			<td height="41" style="height:41px;width:216px;">Glutaraldehyde</td>
			<td style="width:199px;">Electron Microscopy Science</td>
			<td style="width:184px;">#16120</td>
			<td></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:216px;">PI(4,5)P2 1st antibody</td>
			<td>Santa Cruz</td>
			<td>sc-53412</td>
			<td></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;">secondary antibody&#160; F(ab&#8217;)2-goat-anti-mouse Alexa Fluor 647</td>
			<td style="width:199px;">Invitrogen</td>
			<td>A-21237</td>
			<td></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:216px;">Tetraspeck beads</td>
			<td style="width:199px;">Invitrogen</td>
			<td style="width:184px;">T7279</td>
			<td></td>
		</tr>
		<tr height="41">
			<td height="41" style="height:41px;width:216px;">magnetic quick release imaging chamber&#160;</td>
			<td style="width:199px;">Warner Instruments</td>
			<td style="width:184px;">Cat#641994</td>
			<td></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;">temperature controller</td>
			<td style="width:199px;">Warner Instruments</td>
			<td>TC-344C</td>
			<td></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:216px;">Poly-D-Lysine</td>
			<td style="width:199px;">Sigma</td>
			<td style="width:184px;">P6407</td>
			<td></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:216px;">Phosphate buffer saline</td>
			<td style="width:199px;">Sigma</td>
			<td style="width:184px;">P4417-100TAB</td>
			<td></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:216px;">EGTA</td>
			<td style="width:199px;">Sigma</td>
			<td align="right" style="width:184px;">3780</td>
			<td></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:216px;">NH4Cl</td>
			<td style="width:199px;">Sigma</td>
			<td style="width:184px;">A0171</td>
			<td></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:216px;">Goat serum</td>
			<td style="width:199px;">Sigma</td>
			<td style="width:184px;">G9023</td>
			<td></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:216px;">bovine serum albumin</td>
			<td style="width:199px;">Sigma</td>
			<td style="width:184px;">A7906</td>
			<td></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:216px;">NaCl</td>
			<td style="width:199px;">Sigma</td>
			<td style="width:184px;">S5886</td>
			<td></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:216px;">KCl</td>
			<td style="width:199px;">Sigma</td>
			<td style="width:184px;">P5405</td>
			<td></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:216px;">CaCl2*2H2O</td>
			<td style="width:199px;">Sigma</td>
			<td align="right" style="width:184px;">223506</td>
			<td></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:216px;">MgCl2*6H2O</td>
			<td style="width:199px;">Sigma</td>
			<td style="width:184px;">M9272</td>
			<td></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:216px;">Glucose</td>
			<td style="width:199px;">Sigma</td>
			<td style="width:184px;">G7021</td>
			<td></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:216px;">HEPES</td>
			<td style="width:199px;">Sigma</td>
			<td style="width:184px;">H4034</td>
			<td></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:216px;">Paraformaldyhyde</td>
			<td style="width:199px;">Sigma</td>
			<td style="width:184px;">P6148</td>
			<td></td>
		</tr>
	</tbody>
</table>

single-molecule super-resolution imaging of phosphatidylinositol 4,5-bisphosphate in the plasma membrane with novel fluorescent probes

Phosphoinositides in the cell membrane are signaling lipids with multiple cellular functions. Phosphatidylinositol 4,5-bisphosphate (PI(4,5)P2) is a determinant phosphoinositide of the plasma membrane (PM), and it is required to modulate ion channels, actin dynamics, exocytosis, endocytosis, intracellular signaling, and many other cellular processes. However, the spatial organization of PI(4,5)P2 in the PM is controversial, and its nanoscale distribution is poorly understood due to the technical limitations of research approaches. Here by utilizing single molecule localization microscopy and the Pleckstrin Homology (PH) domain based dual color fluorescent probes, we describe a novel method to visualize the nanoscale distribution of PI(4,5)P2 in the PM in fixed membrane sheets as well as live cells.

The localization uncertainty (&#963;) of our super-resolution system is 14.73 nm23. Direct comparisons between TIRF and PALM images demonstrated a significant improvement of spatial resolution. Figure 3A-B shows the representative PI(4,5)P2 TIRF images labeled with PI(4,5)P2 antibody and iRFP-PAmCherry1-PHPLC&#948;1 in typical membrane sheets and live cells. The images with conventional TIRF microscopy in membrane sheets are remarkably similar to those in intact live cells labeled with the enhanced green fluorescence protein (EGFP) tagged PH domains (EGFP-PHPLC&#948;1) (Figure 3C). All samples showed an even distribution of probes. In contrast, non-optimal fixation of the samples resulted in sharp dense PI(4,5)P2 clusters and a decrease in signal intensity (Figure 4). Under optimal fixation conditions, the super-resolution images of PI(4,5)P2 in fixed cells (Figure 5) revealed a homogenous distribution of probes in a significant portion of the PM with only limited concentration gradients. Some membrane patches enriched with PI(4,5)P2 probes were sparsely distributed and had various sizes. Live cell PALM images display a similar spatial distribution as fixed cells (Figure 6). Detailed analysis of PI(4,5)P2 signals over time results in fast dynamics in local areas, without significant changes of their abundance in broad areas.
<img alt="Figure 1" src="/files/ftp_upload/54466/54466fig1.jpg" /> 
Figure 1. Scheme for fluorescent probes used in this study. (A-B) iRFP-PAmCherry1-PHPLC&#948;1 probe used in the fixed membrane sheet experiments. During conventional TIRF imaging (A), a 640 nm laser is used to excite the iRFP (Ex: 692 nm; Em: 713 nm). TIRF image taken in this condition serves as a TIRF reference image for the super-resolution imaging obtained by PALM imaging (B). A 405 nm laser is used to photo-activate the PAmCherry1 fluorophore and a 561 nm laser is used to excite PAmCherry1 (Ex: 564 nm; Em: 595 nm) for PALM imaging. (C-D) mEos3.1-PHPLC&#948;1 probe used in the live cell experiments. (C) During conventional TIRF imaging, a 488 nm laser is used to excite mEOS3.1 (Ex: 506 nm; Em: 519 nm). (D) After photoconversion by a 405 nm laser, mEos3.1 turns into the red form (Ex: 573 nm; Em: 584 nm) and a 561 nm laser is used for PALM acquisitions. <a href="https://cloudflare-jove-com.remotexs.ntu.edu.sg/files/ftp_upload/54466/54466fig1large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 2" src="/files/ftp_upload/54466/54466fig2.jpg" /> 
Figure 2. Scheme for membrane sheet preparation from INS-1 cells. (A) Place the coverslip with cultured cells facing down onto a PDL-coated coverslip and wait for 7 ~ 10 min at 4 &#176;C to allow cell attachment to the PDL-coated coverslip. (B) Peel off the top coverslip with tweezers and fix the membrane sheet attached to the PDL pre-coated coverslip. (C) Image the samples with TIRFM and PALM. <a href="https://cloudflare-jove-com.remotexs.ntu.edu.sg/files/ftp_upload/54466/54466fig2large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 3" src="/files/ftp_upload/54466/54466fig3.jpg" /> 
Figure 3. PI(4,5)P2 spatial organization is similar between membrane sheets and intact live cells under conventional TIRF microscope. (A) A typical TIRF image of membrane sheets fixed at 4 &#176;C with 4% PFA and 0.2% GA. PI(4,5)P2 was labeled with PI(4,5)P2 specific antibody. (B) A membrane sheet from the INS-1 cell expressing iRFP-PAmCherry1-PHPLC&#948;1. (C) TIRF image of two intact live cells expressing EGFP-PHPLC&#948;1 at different levels. Scale bars: (A): 3 &#181;m; (B) and (C): 5 &#181;m. <a href="https://cloudflare-jove-com.remotexs.ntu.edu.sg/files/ftp_upload/54466/54466fig3large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 4" src="/files/ftp_upload/54466/54466fig4.jpg" /> 
Figure 4. PI(4,5)P2 spatial organization in membrane sheets is sensitive to common fixation conditions. (A) Membrane sheets fixed at 37 &#176;C with 4% PFA alone and labeled with PI(4,5)P2 specific antibody (as in Figure 3A). (B) Membrane sheet fixed at RT&#160;with PFA alone and labeled with PI(4,5)P2 specific antibody. Note that the dense clusters of PI(4,5)P2 probes are clearly visible under TIRF microscope, in contrast to the much more even fluorescence images shown in Figure 3A. Scale bars: A-B: 3 &#181;m. <a href="https://cloudflare-jove-com.remotexs.ntu.edu.sg/files/ftp_upload/54466/54466fig4large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 5" src="/files/ftp_upload/54466/54466fig5.jpg" /> 
Figure 5. PALM imaging of PI(4,5)P2 probes reveals their nanometer scale distribution in an INS-1 cell PM. (A) iRFP TIRF image of a membrane sheet from an INS-1 cell expressing iRFP-PAmCherry1-PHPLC&#948;1. (B) Corresponding PALM image of PM in the same region based on PAmCherry1 signal reconstruction. Note the homogeneous PI(4,5)P2 spatial distribution in major PM regions and several PI(4,5)P2 microdomains. (C) An enlarged view of the boxed region in (B). Arrows indicate sparsely distributed PM microdomains enriched with PI(4,5)P2 probes. Scale bars: A and B: 3 &#181;m; C: 500 nm. <a href="https://cloudflare-jove-com.remotexs.ntu.edu.sg/files/ftp_upload/54466/54466fig5large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 6" src="/files/ftp_upload/54466/54466fig6.jpg" /> 
Figure 6. PALM imaging in live INS-1 cells. (A) TIRF image of PI(4,5)P2 in a live INS-1 cell expressing mEos3.1-PHPLC&#948;1. The image was rapidly acquired in the green channel before PALM acquisition (35 &#176;C). (B) Sequential live-cell PALM images at 10 sec interval. Insets show the intensity profiles of the local PI(4,5)P2 density along the same straight line 1 position at different times in (B) and (C). Note their large local intensity changes within 10 sec. (D) Time course of the average intensity changes of PI(4,5)P2 in the large area (box2, 3x3 &#181;m) and small circles (3, 4, and 5, 500 nm diameter) in (B) during 5 min of PALM imaging (frame/10 sec). Note the rapid intensity fluctuations of local PI(4,5)P2 probes (circle 3, 4 and 5) compared to very small changes in the broad area (box 2). (E) Enlarged PALM images of the box2 region in (B) at indicated times. Arrows indicate PI(4,5)P2 enriched membrane patches under physiological conditions. Scale bars: C: 3 &#181;m; E: 500 nm. <a href="https://cloudflare-jove-com.remotexs.ntu.edu.sg/files/ftp_upload/54466/54466fig6large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>

Watch this Scientific Journal Video about Single-molecule Super-resolution Imaging of Phosphatidylinositol 4,5-bisphosphate in the Plasma Membrane with Novel Fluorescent Probes at JoVE.com

Single-molecule Super-resolution Imaging of Phosphatidylinositol 4,5-bisphosphate in the Plasma Membrane with Novel Fluorescent Probes

PI(4,5)P2 regulates various cellular functions, but its nanoscale organization in the cell plasma membrane is poorly understood. By labeling PI(4,5)P2 with a dual-color fluorescent probe fused to the Pleckstrin Homology domain, we describe a novel approach to study the PI(4,5)P2 spatial distribution in the plasma membrane at the nanometer scale.

Phosphoinositides in the cell membrane are signaling lipids with multiple cellular functions. Phosphatidylinositol 4,5-bisphosphate (PI(4,5)P2) is a ...

single-molecule-super-resolution-imaging-phosphatidylinositol-45

Nanyang Technological University

Research

JoVE Journal

Biochemistry

9.4K Views.  University of Wisconsin-Madison. PI(4,5)P2 regulates various cellular functions, but its nanoscale organization in the cell plasma membrane is poorly understood. By labeling PI(4,5)P2 with a dual-color fluorescent probe fused to the Pleckstrin Homology domain, we describe a novel approach to study the PI(4,5)P2 spatial distribution in the plasma membrane at the nanometer scale.

Video: Single-molecule Super-resolution Imaging of Phosphatidylinositol 4,5-bisphosphate in the Plasma Membrane with Novel Fluorescent Probes

High Precision FRET at Single-molecule Level for Biomolecule Structure Determination

A protocol on how to perform high-precision interdye distance measurements using F&#246;rster resonance energy transfer (FRET) at the single-molecule level in multiparameter fluorescence detection (MFD) mode is presented here. MFD maximizes the usage of all &#34;dimensions&#34; of fluorescence to reduce photophysical and experimental artifacts and allows for the measurement of interdye distance with an accuracy up to ~1 &#197; in rigid biomolecules. This method was used to identify three conformational states of the ligand-binding domain of the N-methyl-D-aspartate (NMDA) receptor to explain the activation of the receptor upon ligand binding. When comparing the known crystallographic structures with experimental measurements, they agreed within less than 3 &#197; for more dynamic biomolecules. Gathering a set of distance restraints that covers the entire dimensionality of the biomolecules would make it possible to provide a structural model of dynamic biomolecules.

A protocol for high-precision FRET experiments at the single molecule level is presented here. Additionally, this methodology can be used to identify three conformational states in the ligand-binding domain of the N-methyl-D-aspartate (NMDA) receptor. Determining precise distances is the first step towards building structural models based on FRET experiments.

A protocol on how to perform high-precision interdye distance measurements using F&#246;rster resonance energy transfer (FRET) at the single-molecule ...

Single-molecule Manipulation of G-quadruplexes by Magnetic Tweezers

Non-canonical nucleic acid secondary structure G-quadruplexes (G4) are involved in diverse cellular processes, such as DNA replication, transcription, RNA processing, and telomere elongation. During these processes, various proteins bind and resolve G4 structures to perform their function. As the function of G4 often depends on the stability of its folded structure, it is important to investigate how G4 binding proteins regulate the stability of G4. This work presents a method to manipulate single G4 molecules using magnetic tweezers, which enables studies of the regulation of G4 binding proteins on a single G4 molecule in real time. In general, this method is suitable for a wide scope of applications in studies for proteins/ligands interactions and regulations on various DNA or RNA secondary structures.

A single-molecule magnetic tweezers platform to manipulate G-quadruplexes is reported, which allows for the study of G4 stability and regulation by various proteins.

Non-canonical nucleic acid secondary structure G-quadruplexes (G4) are involved in diverse cellular processes, such as DNA replication, transcription, RNA ...

Measuring Trans-Plasma Membrane Electron Transport by C2C12 Myotubes

Trans-plasma membrane electron transport (tPMET) plays a role in protection of cells from intracellular reductive stress as well as protection from damage by extracellular oxidants. This process of transporting electrons from intracellular reductants to extracellular oxidants is not well defined. Here we present spectrophotometric assays by C2C12 myotubes to monitor tPMET utilizing the extracellular electron acceptors: water-soluble tetrazolium salt-1 (WST-1) and 2,6-dichlorophenolindophenol (DPIP or DCIP). Through reduction of these electron acceptors, we are able to monitor this process in a real-time analysis. With the addition of enzymes such as ascorbate oxidase (AO) and superoxide dismutase (SOD) to the assays, we can determine which portion of tPMET is due to ascorbate export or superoxide production, respectively. While WST-1 was shown to produce stable results with low background, DPIP was able to be re-oxidized after the addition of AO and SOD, which was demonstrated with spectrophotometric analysis. This method demonstrates a real-time, multi-well, quick spectrophotometric assay with advantages over other methods used to monitor tPMET, such as ferricyanide (FeCN) and ferricytochrome c reduction.

The goal of this protocol is to spectrophotometrically monitor trans-plasma membrane electron transport utilizing extracellular electron acceptors and to analyze enzymatic interactions that may occur with these extracellular electron acceptors.

Trans-plasma membrane electron transport (tPMET) plays a role in protection of cells from intracellular reductive stress as well as protection from damage ...

Covalent Immobilization of Proteins for the Single Molecule Force Spectroscopy

In recent years, atomic force microscopy (AFM) based single molecule force spectroscopy (SMFS) extended our understanding of molecular properties and functions. It gave us the opportunity to explore a multiplicity of biophysical mechanisms, e.g., how bacterial adhesins bind to host surface receptors in more detail. Among other factors, the success of SMFS experiments depends on the functional and native immobilization of the biomolecules of interest on solid surfaces and AFM tips. Here, we describe a straightforward protocol for the covalent coupling of proteins to silicon surfaces using silane-PEG-carboxyls and the well-established N-hydroxysuccinimid/1-ethyl-3-(3-dimethyl-aminopropyl)carbodiimid (EDC/NHS) chemistry in order to explore the interaction of pilus-1 adhesin RrgA from the Gram-positive bacterium Streptococcus pneumoniae (S. pneumoniae) with the extracellular matrix protein fibronectin (Fn). Our results show that the surface functionalization leads to a homogenous distribution of Fn on the glass surface and to an appropriate concentration of RrgA on the AFM cantilever tip, apparent by the target value of up to 20% of interaction events during SMFS measurements and revealed that RrgA binds to Fn with a mean force of 52 pN. The protocol can be adjusted to couple via site specific free thiol groups. This results in a predefined protein or molecule orientation and is suitable for other biophysical applications besides the SMFS.

This protocol describes the covalent immobilization of proteins with a heterobifunctional silane coupling agent to silicon-oxide surfaces designed for the atomic force microscopy based single molecule force spectroscopy which is exemplified by the interaction of RrgA (pilus-1 tip adhesin of S. pneumoniae) with fibronectin.

In recent years, atomic force microscopy (AFM) based single molecule force spectroscopy (SMFS) extended our understanding of molecular properties and ...

Proteome-wide Quantification of Labeling Homogeneity at the Single Molecule Level

Cell proteomes are often characterized using electrophoresis assays, where all species of proteins in the cells are non-specifically labeled with a fluorescent dye and are spotted by a photodetector following their separation. Single molecule fluorescence imaging can provide ultrasensitive protein detection with its ability for visualizing individual fluorescent molecules. However, the application of this powerful imaging method to electrophoresis assays is hampered by the lack of ways to characterize the homogeneity of fluorescent labeling of each protein species across the proteome. Here, we developed a method to evaluate the labeling homogeneity across the proteome based on a single molecule fluorescence imaging assay. In our measurement using a HeLa cell sample, the proportion of proteins labeled with at least one dye, which we termed &#8216;labeling occupancy&#8217; (LO), was determined to range from 50% to 90%, supporting the high potential of the application of single molecule imaging to sensitive and precise proteome analysis.

Here, we present a protocol to assess the labeling homogeneity for each protein species in a complex protein sample at the single molecule level.

Cell proteomes are often characterized using electrophoresis assays, where all species of proteins in the cells are non-specifically labeled with a ...

Interactions with and Membrane Permeabilization of Brain Mitochondria by Amyloid Fibrils

A growing body of evidence indicates that membrane permeabilization, including internal membranes such as mitochondria, is a common feature and primary mechanism of amyloid aggregate-induced toxicity in neurodegenerative diseases. However, most reports describing the mechanisms of membrane disruption are based on phospholipid model systems, and studies directly targeting events occurring at the level of biological membranes are rare. Described here is a model for studying the mechanisms of amyloid toxicity at the membrane level. For mitochondrial isolation, density gradient medium is used to obtain preparations with minimal myelin contamination. After mitochondrial membrane integrity confirmation, the interaction of amyloid fibrils arising from &#945;-synuclein, bovine insulin, and hen egg white lysozyme (HEWL) with rat brain mitochondria, as an in vitro biological model, is investigated. The results demonstrate that treatment of brain mitochondria with fibrillar assemblies can cause different degrees of membrane permeabilization and ROS content enhancement. This indicates structure-dependent interactions between amyloid fibrils and mitochondrial membrane. It is suggested that biophysical properties of amyloid fibrils and their specific binding to mitochondrial membranes may provide explanations for some of these observations.

Provided here is a protocol for investigating the interactions between native form, prefibrillar, and mature amyloid fibrils of different peptides and proteins with mitochondria isolated from different tissues and various areas of the brain.

A growing body of evidence indicates that membrane permeabilization, including internal membranes such as mitochondria, is a common feature and primary ...

Production of Dynein and Kinesin Motor Ensembles on DNA Origami Nanostructures for Single Molecule Observation

Cytoskeletal motors are responsible for a wide variety of functions in eukaryotic cells, including mitosis, cargo transport, cellular motility, and others. Many of these functions require motors to operate in ensembles. Despite a wealth of knowledge about the mechanisms of individual cytoskeletal motors, comparatively less is known about the mechanisms and emergent behaviors of motor ensembles, examples of which include changes to ensemble processivity and velocity with changing motor number, location, and configuration. Structural DNA nanotechnology, and the specific technique of DNA origami, enables the molecular construction of well-defined architectures of motor ensembles. The shape of cargo structures as well as the type, number and placement of motors on the structure can all be controlled. Here, we provide detailed protocols for producing these ensembles and observing them using total internal reflection fluorescence microscopy. Although these techniques have been specifically applied for cytoskeletal motors, the methods are generalizable to other proteins that assemble in complexes to accomplish their tasks. Overall, the DNA origami method for creating well-defined ensembles of motor proteins provides a powerful tool for dissecting the mechanisms that lead to emergent motile behavior.

The goal of this protocol is to form ensembles of molecular motors on DNA origami nanostructures and observe the ensemble motility using total internal reflection fluorescence microscopy.

Cytoskeletal motors are responsible for a wide variety of functions in eukaryotic cells, including mitosis, cargo transport, cellular motility, and ...

Conventional BODIPY Conjugates for Live-Cell Super-Resolution Microscopy and Single-Molecule Tracking

Single molecule localization microscopy (SMLM) techniques overcome the optical diffraction limit of conventional fluorescence microscopy and can resolve intracellular structures and the dynamics of biomolecules with ~20 nm precision. A prerequisite for SMLM are fluorophores that transition from a dark to a fluorescent state in order to avoid spatio-temporal overlap of their point spread functions in each of the thousands of data acquisition frames. BODIPYs are well-established dyes with numerous conjugates used in conventional microscopy. The transient formation of red-shifted BODIPY ground-state dimers (DII) results in bright single molecule emission enabling single molecule localization microscopy (SMLM). Here we present a simple but versatile protocol for SMLM with conventional BODIPY conjugates in living yeast and mammalian cells. This procedure can be used to acquire super-resolution images and to track single BODIPY-DII states to extract spatio-temporal information of BODIPY conjugates. We apply this procedure to resolve lipid droplets (LDs), fatty acids, and lysosomes in living yeast and mammalian cells at the nanoscopic length scale. Furthermore, we demonstrate the multi-color imaging capability with BODIPY dyes when used in conjunction with other fluorescent&#160;probes. Our representative results show the differential spatial distribution and mobility of BODIPY-fatty acids and neutral lipids in yeast under fed and fasted conditions. This optimized protocol for SMLM can be used with hundreds of commercially available BODIPY conjugates and is a useful resource to study biological processes at the nanoscale far beyond the applications of this work.&#160;

Conventional BODIPY conjugates can be used for live-cell single-molecule localization microscopy (SMLM) through exploitation of their transiently forming, red-shifted ground state dimers. We present an optimized SMLM protocol to track and resolve subcellular neutral lipids and fatty acids in living mammalian and yeast cells at the nanoscopic length scale.

Single molecule localization microscopy (SMLM) techniques overcome the optical diffraction limit of conventional fluorescence microscopy and can resolve ...

An In Vitro Single-Molecule Imaging Assay for the Analysis of Cap-Dependent Translation Kinetics

Cap-dependent protein synthesis is the predominant translation pathway in eukaryotic cells. While various biochemical and genetic approaches have allowed extensive studies of cap-dependent translation and its regulation, high resolution kinetic characterization of this translation pathway is still lacking. Recently, we developed an in vitro assay to measure cap-dependent translation kinetics with single-molecule resolution. The assay is based on fluorescently labeled antibody binding to nascent epitope-tagged polypeptide. By imaging the binding and dissociation of antibodies to and from nascent peptide&#8211;ribosome&#8211;mRNA complexes, the translation progression on individual mRNAs can be tracked. Here, we present a protocol for establishing this assay, including mRNA and PEGylated slide preparations, real-time imaging of translation, and analysis of single molecule trajectories. This assay enables tracking of individual cap-dependent translation events and resolves key translation kinetics, such as initiation and elongation rates. The assay can be widely applied to distinct translation systems and should broadly benefit in vitro studies of cap-dependent translation kinetics and translational control mechanisms.

An In Vitro Single-Molecule Imaging Assay for the Analysis of Cap-Dependent Translation Kinetics

Tracking individual translation events allows for high-resolution kinetic studies of cap-dependent translation mechanisms. Here we demonstrate an in vitro single-molecule assay based on imaging interactions between fluorescently labeled antibodies and epitope-tagged nascent peptides. This method enables single-molecule characterization of initiation and peptide elongation kinetics during active in vitro cap-dependent translation.

Cap-dependent protein synthesis is the predominant translation pathway in eukaryotic cells. While various biochemical and genetic approaches have allowed ...

Single-Molecule Imaging of EWS-FLI1 Condensates Assembling on DNA

The fusion genes resulting from chromosomal translocation have been found in many solid tumors or leukemia. EWS-FLI1, which belongs to the FUS/EWS/TAF15 (FET) family of fusion oncoproteins, is one of the most frequently involved fusion genes in Ewing sarcoma. These FET family fusion proteins typically harbor a low-complexity domain (LCD) of FET protein at their N-terminus and a DNA-binding domain (DBD) at their C-terminus. EWS-FLI1 has been confirmed to form biomolecular condensates at its target binding loci due to LCD-LCD and LCD-DBD interactions, and these condensates can recruit RNA polymerase II to enhance gene transcription. However, how these condensates are assembled at their binding sites remains unclear. Recently, a single-molecule biophysics method-DNA Curtains-was applied to visualize these assembling processes of EWS-FLI1 condensates. Here, the detailed experimental protocol and data analysis approaches are discussed for the application of DNA Curtains in studying the biomolecular condensates assembling on target DNA.

Here, we describe the use of the single-molecule imaging method, DNA Curtains, to study the biophysical mechanism of EWS-FLI1 condensates assembling on DNA.

The fusion genes resulting from chromosomal translocation have been found in many solid tumors or leukemia. EWS-FLI1, which belongs to the FUS/EWS/TAF15 ...