We thank Dr. Kristen Verhey (University of Michigan, Ann Arbor) and Dr. Gregory Pazour (University of Massachusetts Medical School) for providing some plasmids. The project was supported by grants from the National Institutes of Health (NIH GM097037, GM116204 and GM122552 to W.Y.).

1. NIH-3T3 cell preparation for SPEED microscopy from stock
<ol>
	<li>1.5 weeks in advance of the experiment, recover a fresh culture of NIH-3T3 cells from a frozen stock by thawing at 37 &#176;C and transferring the cells to a 25 cm2 cell culture flask with 3 mL of Dulbecco&#39;s Modified Eagle&#39;s Medium (DMEM) supplemented with 110 mg/mL sodium pyruvate, 2 mM glutamine, 10% fetal bovine serum, and 1% penicillin/streptomycin.</li>
	<li>Incubate the cells at 37 &#176;C in a 5% CO2 incubator.</li>
	<li>Split cells at 80% confluency, about every two days, at least three times before experimental day to ensure homogeneity of cell cycle. Trypsinize cells with 0.25% trypsin for 2 min at 37 &#176;C, aspirate trypsin and replace it with 2 mL of medium. Pipette the medium repeatedly to break up cell clusters, remove the desired number of cells and bring total volume of media back up to 3 mL. 
	NOTE: NIH-3T3 were previously genetically engineered to express NPHP-4, a protein that localizes to the TZ26, fused at the C terminus to mCherry. mCherry is a fluorophore which can be excited with 561 nm illumination to quantitatively localize the TZ selectivity barrier and orient the primary cilia.</li>
	<li>Two days before the experiment, plate the cells into a 35 mm glass bottom dish at 60-70% confluency with 1.5 mL of the same medium as step 1.1 and return the cells to the incubator.</li>
	<li>One day before the experiment, chemically transfect the cells with the desired plasmid. Mix 500 - 1000 ng of the desired plasmid (see the Note below) in a 1:2.5 ratio with transfection reagent in 0.25 mL of reduced serum media without antibiotics for 30 min. Aspirate media from the 35 mm glass bottom dish and replace it with the 0.25 mL plasmid/transfection reagent mix plus an extra 1.25 mL of reduced serum media without antibiotics. Reduced serum media serves the purpose facilitating a successful transfection, inducing primary cilia growth, as well as keeping the cells alive long enough to perform experiment. Return cells to the incubator for the experiment on the following day. 
	NOTE: When performing single-molecule tracking of IFT20, a plasmid containing a genetically-modified IFT20 fused at its C terminus to GFP is used25. When performing single-molecule tracking of SSTR3, a plasmid containing a genetically-modified SSTR3 fused at its N terminus to an acceptor peptide (AP) domain and C terminus to GFP is used22. In addition to the SSTR3 construct, a plasmid containing the biotin ligase BirA must be co-expressed and the transfection media must be supplemented with 10 &#181;M biotin. BirA then attaches biotin to the AP domain of newly synthesized AP-SSTR3-GFP molecules at the level of the ER. Alexa647 conjugated to three of the four biotin-binding sites on streptavidin, on average, may then be supplemented to the media prior to imaging to fluorescently label the AP-SSTR3-GFP molecules on the external surface of the cell22,27. GFP and AlexaFluor647 are used in this method; however, other fluorescent probes can be used if they have similarly high photo-stability and quantum yield.</li>
	<li>If using the externally-labeled SSTR3 construct, remove the media from the glass bottom dish 1 h before experiment, wash the cell 5 times with 1 mL of phosphate-buffered saline (PBS), and add 1 mL of reduced serum media supplemented with 1 &#181;M Alexa647 conjugated streptavidin.</li>
	<li>No more than 15 min before the experiment, remove media from the glass bottom dish and wash the transfected and labeled cells 5 times with 1 mL of PBS.</li>
	<li>Place 1 mL of imaging buffer (20 mM HEPES, 110 mM KOAc, 5 mM NaOAc, 2 mM MgOAc, 1 mM EGTA, pH 7.3) in the glass bottom dish. 
	NOTE: In the imaging buffer, cells are viable for no longer than 3 h. Therefore, only 2 h of experiments are performed on each dish.</li>
</ol>
2. SPEED microscopy
Note: The SPEED microscopy setup includes an inverted fluorescence microscope equipped with a 1.4-NA 100&#215; oil-immersion apochromatic objective, a 35 mW 633 nm He-Ne laser, 50 mW solid state 488-nm and 561-nm lasers, an on-chip multiplication gain charge-coupled-device camera and a microscope software package for data acquisition and processing (Figure 1). For individual channel imaging, GFP, mCherry, and Alexa647 are excited by 488 nm, 561 nm, or 633 nm lasers, respectively. For single molecule tracking, single point illumination is used to track individual fluorescently-labeled molecules. For epifluorescence imaging, a concave lens is placed in the laser illumination path to expand the beam into a uniform field of illumination. The fluorescence emissions are collected by the same objective, filtered by a dichroic filter (405/488/561/635) and an emission filter (405/488/561/635), and imaged with the above CCD camera operating at 500 Hz for single molecule tracking or 2 Hz for epifluorescence imaging.
<ol>
	<li>Affix the glass bottom plate to the stage of the microscope and locate a cell that is properly expressing the desired constructs. Once a suitable cell has been found, align the NPHP4-mCherry spot at the base of the primary cilia with the location on the imaging plane that corresponds to the laser&#39;s single point illumination.</li>
	<li>Capture an epifluorescence image of NPHP4-mCherry and either IFT20-GFP or AP-SSTR3-GFP using the &#34;Snap&#34; function in the &#34;Camera&#34; tab of the &#34;Focus Controls&#34; window if using the digital microscopy software package (see Table of Materials). 
	NOTE: These images will act as a reference for the subsequent single molecule locations.</li>
	<li>Once the reference images are obtained, locally reduce the concentration of labeled single molecules. Photo-bleach the TZ with 1 mW laser illumination for 20 s or until the fluorescence intensity is close to that of background fluorescence. 
	NOTE: When the precise concentration can be controlled, 0.1-1 nM labeled single molecules are used.</li>
	<li>To prepare for single molecule tracking, reduce the laser illumination power to ~0.15 mW for single molecules labeled with GFP or ~0.5 mW for molecules labeled with Alexa647.</li>
	<li>As soon as the laser power and imaging parameters are set, maximum gain and intensification and 2 ms frame rate, for single molecule imaging, engage the appropriate illumination laser and record non-photobleached, labeled single molecules as they are transported through the photobleached region of the TZ by clicking the &#34;Stream&#34; button in the &#34;Camera&#34; tab of the &#34;Focus Controls&#34; window. 
	NOTE: No more than 2 min of video should be captured to minimize the effects of ciliary drift to a negligible level.</li>
	<li>After capturing the single molecule video, process the videos using a 2D Gaussian fitting algorithm, such as Glimpse by the Gelles Lab, which precisely localizes the centroid of each single molecule&#39;s excitation PSF in an encompassing area of interest (AOI).</li>
	<li>Select all single molecule locations with precision &#60;10 nm and correct the center of cilia based on distribution of single molecule locations fitted with a 2D Gaussian function. 
	NOTE: By using 2D to 3D transformation algorithm, the 3D transport routes of IFT20-GFP and AP-SSTR3 routes are clearly shown on ciliary axonemal or ciliary membrane, respectively.</li>
</ol>
3. 2D to 3D Transformation
<ol>
	<li>Once several thousand localizations for transiting molecules (signal to noise ratio &#62; 11) in the cilium are collected, select the long axis of the cilium as the X-dimension. Make a Y dimension histogram of the locations and obtain the bin sums in 10 nm increments. 
	NOTE: The 2D to 3D transformation may be evaluated by hand or any software or programming language. The authors have successfully implemented the transformation in both Matlab and Python 2.7.</li>
</ol>

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The authors declare no conflicts of interest.

This protocol describes the application of SPEED microscopy to the primary cilium, a cellular signaling organelle that is highly reliant on efficient protein transport. SPEED microscopy can provide high resolution (&#60; 10 nm) locations for fluorescently-labeled molecules as they pass through the single point illumination centered on the TZ. Previously it has been applied to study the protein trafficking through the NPC6,7,8. H...

Since stated by Ernst Abbe in 1873, the resolution of conventional light microscopy has been believed to be limited to approximately 200 nm due to light diffraction from the objective1,2. Currently, super-resolution light microscopy techniques break this limitation and allow the capture of dynamic images with sub-diffraction (&#60; 200 nm) resolution. The techniques generally fall into two broad categories: stimulated emission depletion (STED) microscopy based approaches, which generate sub-diffraction illumination volume due to nonlinear optical response of fluorophores in samples3; and photoactivated light microscopy (PALM) and stochastic optical reconstruction microscopy (STORM)-based super-resolution techniques, which utilize mathematical functions to localize the centroids of fluorophores and then reconstitute these centroids to form super-resolution images4,5. Currently, due to the relatively uncomplicated optical setup, PALM and STORM are extensively employed by only activating a small subset of fluorophores in each frame of a long video of a biological preparation. This allows for the more accurate localization by 2D Gaussian fitting of the fluorescent spot, termed the point spread function (PSF), of fluorescently-labeled proteins in each frame of the video. The 2D location of each fluorescently-labeled molecule can then be superimposed on a single imaging plane to produce a super-resolution image of the biological preparation1,2. While these single-molecule localization, super-resolution approaches to microscopy certainly revolutionized how imaging of biological samples was performed, there are still challenges to be overcome. For example, STORM and PALM can achieve their best spatial resolutions after fixation of biological samples and thus present a static representation of the fluorescently-labeled proteins, which is a similar limitation of electron microscopy. Additionally, to achieve high spatial resolution for each fluorescently-labeled protein in live cells, samples must be imaged at very long framerates which are unable to capture protein dynamics. Therefore, it is necessary to overcome these main technical hurdles.
To obtain a high spatiotemporal resolution that is well-suited for detecting fast-moving proteins or RNAs in live cells, we have developed super-resolution SPEED microscopy in our laboratory (Figure 1)6,7,8. Several major technical advances in SPEED microscopy have previously enabled us to successfully track nucleocytoplasmic transport of small molecules, proteins, mRNA and virus through native nuclear pore complexes (NPCs)6,7,8. Briefly, the following features of SPEED microscopy will be used to track fast-moving macromolecules through sub-micrometer rotationally symmetrical structures in live cells, such as NPCs and primary cilia: (1) An inclined or a vertical illumination PSF enables the excitation of single molecules within a small diffraction-limit volume in the focal plane (Figure 1); (2) The inclined PSF can greatly avoid out-of-focus fluorescence and thus improve the signal-to-noise ratio. (3) The optical density of 100-500 kW/ cm2 in the illumination PSF allows thousands of photons to be collected from single fluorophores with fast detection speeds (&#62; 500 Hz). (4) The fast detection speed also greatly reduces the single-molecule spatial localization error (&#60; 10 nm) in determining the spatial trajectories of moving fluorescent molecules in live cells, because molecular diffusion is one of major factors causing imperfections of single-molecule localization for moving molecules. (5) Well-established 2D to 3D transformation algorithms enable us to provide 3D spatial probability density maps of transport routes for molecules in the NPC or the primary cilium. It is noteworthy that our conversion process between the Cartesian and the cylindrical coordination system is used to generate a 3D spatial probability density map rather than 3D single-molecule tracking (Figure 2). Previously, electron microscopy data have revealed that the NPC9,10 and the primary cilium11 both have a rotationally symmetrical structure. In principle, randomly diffusing molecules moving through the NPC or primary cilium should also have rotationally symmetrical distributions. As shown in Figure 2, a high number of randomly diffusing molecules inside the cylinder would generate rotationally symmetrical distributions at the cross-section view as that in the NPC, further resulting in an approximately uniform spatial distribution within each very small sub-region between two neighboring rings (Figure 2E). This uniform distribution leads that the spatial distribution along &#952; dimension in the cylindrical system is constant. Then the 3D coordinates (R, X, &#952;) can be simplified to be the 2D coordinates (R, X, constant). Actually, our conversion process between the Cartesian and the cylindrical systems is from 2D (X, Y) to 2D (R, X, constant). The constant &#952;, refers to the spatial density p in Figure 2E, is calculated by using the equation A<img alt="Equation 1" src="/files/ftp_upload/56475/56475eq1.jpg" />.
Ultimately, single-molecule tracking has broad application in biological research, thus, it is natural that a plethora of techniques will be developed to fill specific biological niches12,13,14. Such is the case with SPEED microscopy. Previously, when coupled with a 3D transformation algorithm, this technique was developed to resolve 3D transport routes of transiting molecules through the NPCs, a sub-diffraction-sized and rotationally symmetric biological structure6. In this paper, primary cilia are shown to be excellent model organelles as well. Primary cilia are cylindrical, antenna-like organelles (~125 nm radius) that project from the surface of most mammalian cells15,16,17. They are responsible for receiving external signals and transmitting an intracellular response typically associated with growth and metabolism15,16. Therefore, flux of structural proteins, recycling of transmembrane receptors, and transmission of intracellular messengers are vital responsibilities of primary cilia. At the juncture between the primary cilia and the cell body is a critical selectivity barrier, called the transition zone or TZ, through which all this protein transport must occur11,18,19,20. In addition to the gating function of the TZ, at least two transport processes, intraflagellar transport and passive diffusion, are thought to be responsible for the movement of protein through this region16,21,22. From a human health standpoint, the loss of primary cilia and subsequent deregulation of downstream signaling is characteristic of many cancers. In addition, many genetic diseases, such as Bardet-Biedl syndrome and polycystic kidney disease, are associated with defective protein transport23. Both the sub-diffraction limit size and the complex process of selective protein transport through the TZ make the primary cilia a prime target for this technique. In this methods paper, we will demonstrate the tracking of a ciliary transmembrane protein, somatostatin receptor 3 (SSTR3)24, labeled externally with Alexa Fluor 647 and a component of IFT, IFT2025, labeled with a fused GFP molecule.

<table border="0" cellpadding="0" cellspacing="0" style="width:619px;" width="618">
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		<col />
		<col />
		<col />
	</colgroup>
	<tbody>
		<tr height="47">
			<td height="47" style="height:47px;width:123px;">25 cm2 tissue culture dish</td>
			<td style="width:204px;">Corning</td>
			<td style="width:101px;">VV-01936-00</td>
			<td style="width:191px;"></td>
		</tr>
		<tr height="43">
			<td height="43" style="height:43px;width:123px;">Penicillin/streptomycin</td>
			<td style="width:204px;">ThermoFisher</td>
			<td style="width:101px;">15140122</td>
			<td style="width:191px;"></td>
		</tr>
		<tr height="43">
			<td height="43" style="height:43px;width:123px;">Fetal bovine serum</td>
			<td style="width:204px;">ThermoFisher</td>
			<td style="width:101px;">10438018</td>
			<td style="width:191px;"></td>
		</tr>
		<tr height="22">
			<td height="22" style="height:22px;width:123px;">DMEM</td>
			<td style="width:204px;">ThermoFisher</td>
			<td style="width:101px;">10566-016</td>
			<td style="width:191px;"></td>
		</tr>
		<tr height="22">
			<td height="22" style="height:22px;width:123px;">OPTIMEM</td>
			<td style="width:204px;">ThermoFisher</td>
			<td style="width:101px;">31985062</td>
			<td style="width:191px;"></td>
		</tr>
		<tr height="22">
			<td height="22" style="height:22px;width:123px;">Trypsin</td>
			<td style="width:204px;">ThermoFisher</td>
			<td style="width:101px;">25300054</td>
			<td style="width:191px;"></td>
		</tr>
		<tr height="43">
			<td height="43" style="height:43px;width:123px;">Phosphate buffered saline</td>
			<td style="width:204px;">Sigma-Aldrich</td>
			<td style="width:101px;">P3813-1PAK</td>
			<td style="width:191px;"></td>
		</tr>
		<tr height="22">
			<td height="22" style="height:22px;width:123px;">Transit LT1</td>
			<td style="width:204px;">Mirus</td>
			<td style="width:101px;">MIR 2300</td>
			<td style="width:191px;"></td>
		</tr>
		<tr height="43">
			<td height="43" style="height:43px;width:123px;">35 mm glass bottom dish</td>
			<td style="width:204px;">MatTek</td>
			<td style="width:101px;">P35GCOL-0-14-C</td>
			<td style="width:191px;"></td>
		</tr>
		<tr height="64">
			<td height="64" style="height:64px;width:123px;">AlexaFluor 647-conjugated streptavidin</td>
			<td style="width:204px;">ThermoFisher</td>
			<td style="width:101px;">S21374</td>
			<td style="width:191px;"></td>
		</tr>
		<tr height="22">
			<td height="22" style="height:22px;width:123px;">Biotin</td>
			<td style="width:204px;">Sigma-Aldrich</td>
			<td style="width:101px;">B4501-100MG</td>
			<td style="width:191px;"></td>
		</tr>
		<tr height="43">
			<td height="43" style="height:43px;width:123px;">633 nm He-Ne laser</td>
			<td style="width:204px;">Melles Griot</td>
			<td style="width:101px;">25-LHP-928-249</td>
			<td style="width:191px;"></td>
		</tr>
		<tr height="43">
			<td height="43" style="height:43px;width:123px;">561 nm solid state laser</td>
			<td style="width:204px;">Coherent</td>
			<td style="width:101px;">OBIS 561-50 LS</td>
			<td style="width:191px;"></td>
		</tr>
		<tr height="43">
			<td height="43" style="height:43px;width:123px;">488 nm solid state laser</td>
			<td style="width:204px;">Coherent</td>
			<td style="width:101px;">1185053</td>
			<td style="width:191px;"></td>
		</tr>
		<tr height="64">
			<td height="64" style="height:64px;width:123px;">Inverted fluorescence microscope</td>
			<td style="width:204px;">Olympus</td>
			<td style="width:101px;">IX81</td>
			<td style="width:191px;"></td>
		</tr>
		<tr height="85">
			<td height="85" style="height:85px;width:123px;">1.4-NA 100&#215; oil-immersion apochromatic objective</td>
			<td style="width:204px;">Olympus</td>
			<td style="width:101px;">UPLSAPO 100&#215;</td>
			<td style="width:191px;"></td>
		</tr>
		<tr height="106">
			<td height="106" style="height:106px;width:123px;">On-chip multiplication gain charge-coupled-device camera</td>
			<td style="width:204px;">Roper Scientific</td>
			<td style="width:101px;">Cascade 128+</td>
			<td style="width:191px;"></td>
		</tr>
		<tr height="64">
			<td height="64" style="height:64px;width:123px;">Dichroic filter</td>
			<td style="width:204px;">Semrock</td>
			<td style="width:101px;">Di01- R405/488/561/635-25x36</td>
			<td style="width:191px;"></td>
		</tr>
		<tr height="64">
			<td height="64" style="height:64px;width:123px;">Emission filter</td>
			<td style="width:204px;">Semrock</td>
			<td style="width:101px;">NF01-405/488/561/635-25X5.0</td>
			<td style="width:191px;"></td>
		</tr>
		<tr height="22">
			<td height="22" style="height:22px;width:123px;">Slidebook 6.0</td>
			<td>Intelligent Imaging Innovations</td>
			<td></td>
			<td style="width:191px;">digital microscopy software</td>
		</tr>
	</tbody>
</table>

application of high-speed super-resolution speed microscopy in live primary cilium

The primary cilium is a microtubule-based protrusion on the surface of many eukaryotic cells and contains a unique complement of proteins that function critically in cell motility and signaling. Since cilia are incapable of synthesizing their own protein, nearly 200 unique ciliary proteins need to be trafficked between the cytosol and primary cilia. However, it is still a technical challenge to map three-dimensional (3D) locations of transport pathways for these proteins in live primary cilia due to the limitations of currently existing techniques. To conquer the challenge, recently we have developed and employed a high-speed virtual 3D super-resolution microscopy, termed single-point edge-excitation sub-diffraction (SPEED) microscopy, to determine the 3D spatial location of transport pathways for both cytosolic and membrane proteins in primary cilia of live cells. In this article, we will demonstrate the detailed setup of SPEED microscopy, the preparation of cells expressing fluorescence-protein-labeled ciliary proteins, the real-time single-molecule tracking of individual proteins in live cilium and the achievement of 3D spatial probability density maps of transport routes for ciliary proteins.

This section demonstrates the data obtained from performing SPEED microscopy at the TZ of primary cilia to study the transport route of SSTR3 connected by a ~15 nm external linker to Alexa647 (Figure 3A). It serves the dual purpose of verifying the 3D transformation algorithm. Alexa647 should only label the external surface of the primary cilium and therefore, the 3D transport route should reveal a high-density transport route at that locatio...

Watch this Scientific Journal Video about Application of High-speed Super-resolution SPEED Microscopy in Live Primary Cilium at JoVE.com

Application of High-speed Super-resolution SPEED Microscopy in Live Primary Cilium

Recently we mapped the three-dimensional (3D) spatial locations of transport routes for various proteins translocating inside primary cilia in live cells. Here this paper details the experimental setup, the process of biological samples and the data analyses for the 3D super-resolution fluorescence imaging approach newly applied in live primary cilia.

The primary cilium is a microtubule-based protrusion on the surface of many eukaryotic cells and contains a unique complement of proteins that function ...

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8.2K 조회수.  Temple University. Recently we mapped the three-dimensional (3D) spatial locations of transport routes for various proteins translocating inside primary cilia in live cells. Here this paper details the experimental setup, the process of biological samples and the data analyses for the 3D super-resolution fluorescence imaging approach newly applied in live primary cilia.

비디오: Application of High-speed Super-resolution SPEED Microscopy in Live Primary Cilium

High Speed Droplet-based Delivery System for Passive Pumping in Microfluidic Devices

A novel microfluidic system has been developed that uses the phenomenon of passive pumping along with a user controlled droplet based fluid delivery system. Passive pumping is the phenomenon by which surface tension induced pressure differences drive fluid movement in closed channels. The automated fluid delivery system consists of a set of voltage controlled valves with micro-nozzles connected to a fluid reservoir and a control system. These voltage controlled valves offer a volumetrically precise way to deliver fluid droplets to the inlet of a microfluidic device in a high frequency manner. Based on the  dimensions demonstrated in the current study example, the system is capable of flowing 4 milliliters per minute (through a 2.2mm by 260um cross-sectional channel). Based on these same channel dimensions, fluid exchange of a point inside the channel can be achieved in as little as eight milliseconds. It is observed that there is interplay between momentum of the system (imparted by a combination of the droplets created by the valves and the fluid velocity in the channel), and the surface tension of the liquid. Where momentum provides velocity to the fluid flow (or vice-versa), equilibration of surface tension at the inlet provides a sudden stop to any flow. This sudden stop allows the user to control the flow characteristics of the channel and opens the door for a variety of biological applications, ranging anywhere from reagent delivery to drug-cell studies. It is also observed that when nozzles are aimed at the inlet at shallow angles, the droplet momentum can cause additional interesting fluid phenomena, such as mixing of multiple droplets in the inlet.

A novel microfluidic system has been developed using the phenomenon of passive pumping and a user controlled fluid delivery system. This microfluidic system has the potential to be used in a wide variety of biological applications given its low cost, ease of use, volumetric precision, high speed, repeatability and automation.

Microfluidic 장치에 수동 펌핑을위한 고속 비말 기반 전달 시스템

A novel microfluidic system has been developed that uses the phenomenon of passive pumping along with a user controlled droplet based fluid delivery ...

연구

생물학

Super-resolution Imaging of the Bacterial Division Machinery

Bacterial cell division requires the coordinated assembly of more than ten essential proteins at midcell1,2. Central to this process is the formation of a ring-like suprastructure (Z-ring) by the FtsZ protein at the division plan3,4. The Z-ring consists of multiple single-stranded FtsZ protofilaments, and understanding the arrangement of the protofilaments inside the Z-ring will provide insight into the mechanism of Z-ring assembly and its function as a force generator5,6. This information has remained elusive due to current limitations in conventional fluorescence microscopy and electron microscopy. Conventional fluorescence microscopy is unable to provide a high-resolution image of the Z-ring due to the diffraction limit of light (~200 nm). Electron cryotomographic imaging has detected scattered FtsZ protofilaments in small C. crescentus cells7, but is difficult to apply to larger cells such as E. coli or B. subtilis. Here we describe the application of a super-resolution fluorescence microscopy method, Photoactivated Localization Microscopy (PALM), to quantitatively characterize the structural organization of the E. coli Z-ring8.
	PALM imaging offers both high spatial resolution (~35 nm) and specific labeling to enable unambiguous identification of target proteins. We labeled FtsZ with the photoactivatable fluorescent protein mEos2, which switches from green fluorescence (excitation = 488 nm) to red fluorescence (excitation = 561 nm) upon activation at 405 nm9. During a PALM experiment, single FtsZ-mEos2 molecules are stochastically activated and the corresponding centroid positions of the single molecules are determined with &lt;20 nm precision. A super-resolution image of the Z-ring is then reconstructed by superimposing the centroid positions of all detected FtsZ-mEos2 molecules.
	Using this method, we found that the Z-ring has a fixed width of ~100 nm and is composed of a loose bundle of FtsZ protofilaments that overlap with each other in three dimensions. These data provide a springboard for further investigations of the cell cycle dependent changes of the Z-ring10 and can be applied to other proteins of interest.

We describe a super-resolution imaging method to probe the structural organization of the bacterial FtsZ-ring, an essential apparatus for cell division. This method is based on quantitative analyses of photoactivated localization microscopy (PALM) images and can be applied to other bacterial cytoskeletal proteins.

세균 본부 기계의 슈퍼 해상도 이미징

Bacterial cell division requires the coordinated  assembly of more than ten essential proteins at midcell1,2. Central  to this process is the formation of ...

Test Samples for Optimizing STORM Super-Resolution Microscopy

STORM is a recently developed super-resolution microscopy technique with up to 10 times better resolution than standard fluorescence microscopy techniques. However, as the image is acquired in a very different way than normal, by building up an image molecule-by-molecule, there are some significant challenges for users in trying to optimize their image acquisition. In order to aid this process and gain more insight into how STORM works we present the preparation of 3 test samples and the methodology of acquiring and processing STORM super-resolution images with typical resolutions of between 30-50 nm. By combining the test samples with the use of the freely available rainSTORM processing software it is possible to obtain a great deal of information about image quality and resolution. Using these metrics it is then possible to optimize the imaging procedure from the optics, to sample preparation, dye choice, buffer conditions, and image acquisition settings. We also show examples of some common problems that result in poor image quality, such as lateral drift, where the sample moves during image acquisition and density related problems resulting in the 'mislocalization' phenomenon.

We describe the preparation of three test samples and how they can be used to optimize and assess the performance of STORM microscopes. Using these examples we show how to acquire raw data and then process it to acquire super-resolution images in cells of approximately 30-50 nm resolution.

최적화 STORM 슈퍼 해상도 현미경에 대한 테스트 샘플

STORM is a recently developed super-resolution microscopy technique with up to 10 times better resolution than standard fluorescence microscopy ...

Visualization of G3BP Stress Granules Dynamics in Live Primary Cells

SGs can be visualized in cells by immunostaining of specific protein components or polyA+ mRNAs. SGs are highly dynamic and the study of their assembly and fate is important to understand the cellular response to stress. The deficiency in key factors of SGs like G3BP (RasGAP SH3 domain Binding Protein) leads to developmental defects in mice&#160;and alterations of the Central Nervous System. To study the dynamics of SGs in cells from an organism, one can culture primary cells and follow the localization of a transfected tagged component of SGs. We describe time-lapse experiment to observe G3BP1-containing SGs in Mouse Embryonic Fibroblasts (MEFs). This technique can also be used to study G3BP-containing SGs in live neurons, which is crucial as it was recently shown that these SGs are formed at the onset of neurodegenerative diseases like Alzheimer&#39;s disease. This approach can be adapted to any other cellular body and granule protein component, and performed with transgenic animals, allowing the live study of granules dynamics for example in the absence of a specific factor of these granules.

Stress granules (SGs) are cytoplasmic RNA granules containing stalled ribonucleoprotein particles (RNPs), and important in cellular response to various stresses. Dynamics of SGs can be followed in live cells by visualizing the localization of a tagged component of SGs in transfected primary cells after stress.

라이브 일차 전지에 G3BP 스트레스 과립 역학의 시각화

SGs can be visualized in cells by immunostaining of specific protein components or polyA+ mRNAs. SGs are highly dynamic and the study of their assembly ...

Sample Preparation for Single Virion Atomic Force Microscopy and Super-resolution Fluorescence Imaging

Immobilization of virions to glass surfaces is a critical step in single virion imaging. Here we present a technique&#160;adopted from single molecule imaging assays which allows adhesion of single virions to glass surfaces with specificity. This preparation is based on grafting the surface of the glass with a mixture of PLL-g-PEG and PLL-g-PEG-Biotin, adding a layer of avidin, and finally creating virion anchors through attachment of biotinylated virus specific antibodies. We have applied this technique across a range of experiments including atomic force microscopy (AFM) and super-resolution fluorescence imaging. This sample preparation method results in a control adhesion of the virions to the surface.

The attachment of virions to a surface is a requirement for single virion imaging by Super-resolution fluorescence imaging or atomic force microscopy (AFM). Here we demonstrate a sample preparation method for controlled adhesion of virions to glass surfaces suitable for use in AFM and super-resolution fluorescence imaging.

단일 비리온 원자력 현미경 검사및 초분해성 형광 이미징을 위한 샘플 준비

Immobilization of virions to glass surfaces is a critical step in single virion imaging. Here we present a technique&#160;adopted from single molecule ...

Super-resolution Imaging of the Cytokinetic Z Ring in Live Bacteria Using Fast 3D-Structured Illumination Microscopy (f3D-SIM)

Imaging of biological samples using fluorescence microscopy has advanced substantially with new technologies to overcome the resolution barrier of the diffraction of light allowing super-resolution of live samples. There are currently three main types of super-resolution techniques &#8211; stimulated emission depletion (STED), single-molecule localization microscopy (including techniques such as PALM, STORM, and GDSIM), and structured illumination microscopy (SIM). While STED and single-molecule localization techniques show the largest increases in resolution, they have been slower to offer increased speeds of image acquisition. Three-dimensional SIM (3D-SIM) is a wide-field fluorescence microscopy technique that offers a number of advantages over both single-molecule localization and STED. Resolution is improved, with typical lateral and axial resolutions of 110 and 280 nm, respectively and depth of sampling of up to 30 &#181;m from the coverslip, allowing for imaging of whole cells. Recent advancements (fast 3D-SIM) in the technology increasing the capture rate of raw images allows for fast capture of biological processes occurring in seconds, while significantly reducing photo-toxicity and photobleaching. Here we describe the use of one such method to image bacterial cells harboring the fluorescently-labelled cytokinetic FtsZ protein to show how cells are analyzed and the type of unique information that this technique can provide.

Super-resolution Imaging of the Cytokinetic Z Ring in Live Bacteria Using Fast 3D-Structured Illumination Microscopy f3D-SIM

Spatiotemporal information about dynamic proteins inside live cells is crucial for understanding biology. A type of super-resolution microscopy called fast 3D-structured illumination microscopy (f3D-SIM) reveals unique information about the cytokinetic Z ring in bacteria: both its bead-like appearance and the rapid dynamics of FtsZ within the ring.

고속 3D 구조 조명 현미경을 사용하여 라이브 박테리아의 Cytokinetic Z 반지의 슈퍼 해상도 이미징 (F3D-SIM)

Imaging of biological samples using fluorescence microscopy has advanced substantially with new technologies to overcome the resolution barrier of the ...

Three-dimensional Super Resolution Microscopy of F-actin Filaments by Interferometric PhotoActivated Localization Microscopy (iPALM)

Fluorescence microscopy enables direct visualization of specific biomolecules within cells. However, for conventional fluorescence microscopy, the spatial resolution is restricted by diffraction to ~ 200 nm within the image plane and &#62; 500 nm along the optical axis. As a result, fluorescence microscopy has long been severely limited in the observation of ultrastructural features within cells. The recent development of super resolution microscopy methods has overcome this limitation. In particular, the advent of photoswitchable fluorophores enables localization-based super resolution microscopy, which provides resolving power approaching the molecular-length scale. Here, we describe the application of a three-dimensional super resolution microscopy method based on single-molecule localization microscopy and multiphase interferometry, called interferometric PhotoActivated Localization Microscopy (iPALM). This method provides nearly isotropic resolution on the order of 20 nm in all three dimensions. Protocols for visualizing the filamentous actin cytoskeleton, including specimen preparation and operation of the iPALM instrument, are described here. These protocols are also readily adaptable and instructive for the study of other ultrastructural features in cells.

Three-dimensional Super Resolution Microscopy of F-actin Filaments by Interferometric PhotoActivated Localization Microscopy iPALM

We present a protocol for the application of interferometric PhotoActivated Localization Microscopy (iPALM), a 3-dimensional single-molecule localization super resolution microscopy method, to the imaging of the actin cytoskeleton in adherent mammalian cells. This approach allows light-based visualization of nanoscale structural features that would otherwise remain unresolved by conventional diffraction-limited optical microscopy.

입체 슈퍼의 간섭 광 활성화 현지화 현미경으로 F-액틴 필라멘트의 해상도 현미경 (iPALM)

Fluorescence microscopy enables direct visualization of specific biomolecules within cells. However, for conventional fluorescence microscopy, the spatial ...

Open-source Single-particle Analysis for Super-resolution Microscopy with VirusMapper

Super-resolution fluorescence microscopy is currently revolutionizing cell biology research. Its capacity to break the resolution limit of around 300 nm allows for the routine imaging of nanoscale biological complexes and processes. This increase in resolution also means that methods popular in electron microscopy, such as single-particle analysis, can readily be applied to super-resolution fluorescence microscopy. By combining this analytical approach with super-resolution optical imaging, it becomes possible to take advantage of the molecule-specific labeling capacity of fluorescence microscopy to generate structural maps of molecular elements within a metastable structure. To this end, we have developed a novel algorithm &#8212; VirusMapper &#8212; packaged as an easy-to-use, high-performance, and high-throughput ImageJ plugin. This article presents an in-depth guide to this software, showcasing its ability to uncover novel structural features in biological molecular complexes. Here, we present how to assemble compatible data and provide a step-by-step protocol on how to use this algorithm to apply single-particle analysis to super-resolution images.

This manuscript uses the Fiji-based open-source software package VirusMapper to apply single-particle analysis to super-resolution microscopy images in order to generate precise models of nanoscale structure.

VirusMapper 슈퍼 해상도 현미경을위한 오픈 소스 단일 입자 분석

Super-resolution fluorescence microscopy is currently revolutionizing cell biology research. Its capacity to break the resolution limit of around 300 nm ...

Ground State Depletion Super-resolution Imaging in Mammalian Cells

Advances in fluorescent microscopy and cell biology are intimately correlated, with the enhanced ability to visualize cellular events often leading to dramatic leaps in our understanding of how cells function. The development and availability of super-resolution microscopy has considerably extended the limits of optical resolution from ~250-20 nm. Biologists are no longer limited to describing molecular interactions in terms of colocalization within a diffraction limited area, rather it is now possible to visualize the dynamic interactions of individual molecules. Here, we outline a protocol for the visualization and quantification of cellular proteins by ground-state depletion microscopy&#160;for fixed cell imaging. We provide examples from two different membrane proteins, an element of the endoplasmic reticulum translocon, sec61&#946;, and a plasma membrane-localized voltage-gated L-type Ca2+ channel (CaV1.2). Discussed are the specific microscope parameters, fixation methods, photo-switching buffer formulation, and pitfalls and challenges of image processing.

This article outlines a protocol for the detection of one or more plasma and/or intracellular membrane proteins using Ground State Depletion (GSD) super-resolution microscopy in mammalian cells. Here, we discuss the benefits and considerations of using such approaches for the visualization and quantification of cellular proteins.

포유류 세포에 있는 바닥 상태 고갈 슈퍼 해상도 영상

Advances in fluorescent microscopy and cell biology are intimately correlated, with the enhanced ability to visualize cellular events often leading to ...

Examination of Mitotic and Meiotic Fission Yeast Nuclear Dynamics by Fluorescence Live-cell Microscopy

Live-cell imaging is a microscopy technique used to examine cell and protein dynamics in living cells. This imaging method is not toxic, generally does not interfere with cell physiology, and requires minimal experimental handling. The low levels of technical interference enable researchers to study cells across multiple cycles of mitosis and to observe meiosis from beginning to end. Using fluorescent tags such as Green Fluorescent Protein (GFP) and Red Fluorescent Protein (RFP), researchers can analyze different factors whose functions are important for processes like transcription, DNA replication, cohesion, and segregation. Coupled with data analysis using Fiji (a free, optimized ImageJ version), live-cell imaging offers various ways of assessing protein movement, localization, stability, and timing, as well as nuclear dynamics and chromosome segregation. However, as is the case with other microscopy methods, live-cell imaging is limited by the intrinsic properties of light, which put a limit to the resolution power at high magnifications, and is also sensitive to photobleaching or phototoxicity at high wavelength frequencies. However, with some care, investigators can bypass these physical limitations by carefully choosing the right conditions, strains, and fluorescent markers to allow for the appropriate visualization of mitotic and meiotic events.

Here, we present live-cell imaging which is a non-toxic microscopy method that allows researchers to study protein behavior and nuclear dynamics in living fission yeast cells during mitosis and meiosis.

형광 라이브 세포 현미경 검사법에 의한 미토틱 및 Meiotic 핵분열 효모 핵 역학의 검사

Live-cell imaging is a microscopy technique used to examine cell and protein dynamics in living cells. This imaging method is not toxic, generally does ...