We thank the Herzik lab members for critically thinking and providing feedback on this manuscript and the video content. M.A.H.Jr. is supported by NIH R35 GM138206 and as a Searle Scholar. H.P.M.N is supported by the Molecular Biophysics Training Grant (NIH T32 GM008326). We would also like to thank Bill Anderson, Charles Bowman, and Dr. Gabriel Lander at the Scripps Research Institute for help designing, assembling, and testing the manual plunger shown in the video.

1. Prepare the manual plunging environment
NOTE: Estimated operating time: 5-30 minutes
<ol>
	<li>Locate the manual plunger in a 4 &#176;C cold room where a humidifier can be co-located to maintain the room close to 100% relative humidity (RH) (Figure 1A). 
	CAUTION: Please consult with the institution&#39;s Environmental Health and Safety guidelines for the safe location of the manual plunger and recommended operations.</li>
	<li>Prior to grid preparation, turn on the humidifier in the cold room to ensure the RH of the cold room is &#8805; 95 %. 
	NOTE: Grid preparation in low humidity can result in dehydration of thin films, alteration of buffer components due to evaporation, and a decrease in grid-to-grid reproducibility46. It is not recommended to freeze grids at &#60;80 % RH.</li>
	<li>Ensure the temperature of the cold room is at 4 &#176;C.</li>
	<li>Locate the manual plunger away from strong air currents (i.e., away from air conditioning unit vents) as they can lead to turbulence near grids and/or prominent ice accumulation on cold surfaces.</li>
</ol>
2. Prepare plunging materials and accessories
NOTE: Estimated operating time: 1-5 minutes
<ol>
	<li>Use clean scissors to cut blotting paper circles into 1-1.5 cm wide and ~9 cm long strips. Avoid touching the center of the blotting paper and discard the smaller end pieces. It is important to ensure that the blotting paper strips are dry, clean, and free of contaminants. Separate the strips and place them in a 100 mm Petri dish.</li>
	<li>Place a 22x22 mm square glass coverslip into a separate 60 mm glass Petri dish. This coverslip-containing glass Petri dish will be used to store, transfer, and glow-discharge grids. 
	NOTE: It is recommended to use an air-duster can to remove any visible debris from the slide prior to adding grids. An anti-static gun can also be used to remove any static electricity that accumulates.</li>
	<li>Assemble and label grid storage boxes.</li>
	<li>Acquire 4 to 6 clean and dry clamping tweezers and locate them to the manual plunger. Visually inspect each tweezer prior to plunging to ensure they are not damaged and are free of contaminants.</li>
</ol>
3. Prepare the cryogen dewar and manual plunger
NOTE: Estimated operating time: 5-15 minutes
<ol>
	<li>Install the platform base at the bottom of the plunging dewar. Place the ethane vessel dewar on top of the platform base, add the brass ethane vessel, and then install the spinning grid storage platform.
	<ol>
		<li>Once liquid nitrogen (LN2) is added to the plunging dewar, the height of the platform base can no longer be adjusted. Ensure that the grid base is installed properly and is level to limit grid and/or tweezer damage due to improper plunger height.</li>
	</ol>
	</li>
	<li>Prior to freezing, check the manual plunger and all ancillary equipment to ensure they are functioning properly to limit sample and/or grid loss.</li>
	<li>Prior to each freezing session, replace the tape on the manual plunger arm used to hold the tweezers. The high humidity of the room can deteriorate the tape adhesive and decrease the ability of the tape to hold the tweezers, increasing the likelihood of tweezer damage and/or grid loss.</li>
	<li>Adjust the lamp(s) near the manual plunger to ensure there is sufficient light to monitor sample wicking and ensure grid transfer is easily visualized to prevent grid damage and/or loss (see step 3.7). Use a ring lamp directly behind the plunger to visualize liquid movement and a flexible arm task light near the dewar to illuminate the frozen grids.</li>
	<li>Adjust the foot pedal tension to ensure the dewar plunging arm is securely retained in place while in the raised position and is fully released when the pedal is depressed. Perform several &#34;dry&#34; runs prior to sample application to ensure the plunger is working properly. 
	NOTE: Improper adjustment of the foot pedal tension will result in premature release of the plunging arm (i.e., tension is set too low) and grid loss or incomplete plunging of the grid into the ethane vessel (i.e., the tension is set too high).</li>
	<li>Place the plunging dewar at the base of the manual plunger directly below the plunging arm and secure it in place. Attach a pair of tweezers to the plunging arm using the attached tape. While holding the manual plunging arm, depress the foot pedal to carefully lower the plunging arm and adjust the travel of the plunging arm to ensure the grid will locate within the middle of the ethane vessel.</li>
	<li>Use the bump stop at the top of the plunging arm to determine the final position of the plunging arm when the foot pedal is fully depressed (Figure 1B). Adjust the bump stop height on the plunging arm to adjust the location of the grid in the ethane vessel (Figure 1C). 
	NOTE: Improperly setting the plunging arm height can lead to the grid and/or tweezer damage (e.g., plunging arm height is set too low) or inadequate vitrification (e.g., plunging arm height is set too high).</li>
	<li>Locate the dewar outside the cold room and proceed to preparing liquid ethane (step 4).</li>
</ol>
4. Prepare the cryogen
NOTE: Estimated operating time: 10-30 minutes
<ol>
	<li>Assess the ethane tank, regulator, tubing, and ethane dispensing tip for any signs of damage. Immediately report and rectify any signs of damage before proceeding. 
	CAUTION: Compressed ethane and ethane:propane gas mixes are flammable and can pose a serious threat to life and/or result in injury if improperly handled. Please consult an expert if unsure how to operate or handle compressed gas tanks. Please refer to the institution&#39;s Environmental Health and Safety guidelines when handling flammable compressed gases. In addition, liquified ethane is a powerful cryogen that can pose a serious threat to life and/or injury if not handled properly. Please refer to the institution&#39;s Environmental Health and Safety guidelines when handling cryogens.</li>
	<li>Acquire sufficient LN2 in an appropriate LN2 handling dewar (i.e., 3-4 L is typical for grid preparation and storage). 
	CAUTION: LN2 is a cryogen that can pose a serious threat to life and/or injury if not handled properly.
	<ol>
		<li>Ensure all personal protective equipment are utilized to minimize the risk of injury. The vapor of LN2 is an asphyxiant and should be handled in well-ventilated areas. Please consult an expert if unsure how to operate or handle cryogenic vessels and cryogens. Please refer to the institution&#39;s Environmental Health and Safety guidelines when handling cryogens. For situations in which liquid nitrogen cannot be used in a cold room, we recommend plunge freezing in a cool and well-ventilated space.</li>
	</ol>
	</li>
	<li>Outside of the cold room, cool down the plunging dewar by pouring LN2 directly into the brass ethane vessel until the liquid nitrogen level reaches the top of the ethane vessel (i.e., just above the platform). Top off the LN2 outside the ethane vessel as needed. Proceed to the next step when the LN2 stops bubbling violently (approximately 5 minutes).
	<ol>
		<li>Add LN2 directly to the brass ethane vessel to sufficiently cool the vessel prior to condensing ethane gas. Failure to properly cool the brass ethane vessel will dramatically increase the time it takes to condense ethane.</li>
		<li>Once the dewar has reached LN2 temperature, avoid overfilling the dewar such that LN2 spills into the ethane vessel.</li>
	</ol>
	</li>
	<li>Ethane comes as a compressed gas and needs to be liquefied for use. The ethane tank utilizes a high-purity dual-stage regulator to control the gas flow. Connect tubing to the regulator outlet valve and use a 14-gauge flat metal dispensing tip connected at the end for dispensing ethane.</li>
	<li>Prior to opening the ethane main tank valve, make sure the pressure adjusting knob and outlet valve are closed all the way. Fully open the main tank valve and then open the outlet valve to ~50%. Slowly open the pressure adjusting knob until a slow gas flow is observed. Use the outlet valve to fine-tune the gas flow. 
	CAUTION: Always point the metal dispensing tip away from self when opening valves or making gas flow adjustments.</li>
	<li>Slowly start the gas flow and assess the flow rate by inserting the tip of the ethane gas line into a small beaker of deionized water. Adjust the gas flow until the flow rate moderately disturbs the water.
	<ol>
		<li>Adjust the gas flow rate to ensure proper ethane condensing occurs - too slow of a flow rate will cause the ethane gas to solidify in the dispensing tip and too fast of a flow rate will result in intense bubbling and prevent freezing.</li>
	</ol>
	</li>
	<li>Prior to inserting the tip of the ethane gas line into the brass ethane vessel, clean and wipe the dispensing tip with delicate task wipes to remove any water.</li>
	<li>In a smooth and quick motion, locate the gas dispensing tip at the bottom of the brass ethane vessel and begin moving the dispensing tip in a slow circle around the bottom of the ethane vessel. Solid ethane will form immediately but will quickly liquefy as more ethane gas is added/condensed.
	<ol>
		<li>Continue to move the metal ethane dispensing tip around at the bottom of the ethane vessel to liquefy the solid ethane. Fill up the ethane vessel to &#190; full of liquid ethane (2-3 threads from the top). Stop ethane gas flow by carefully removing the metal ethane dispensing tip from the brass ethane vessel and closing the outlet valve.</li>
	</ol>
	</li>
	<li>Top off the plunging dewar with LN2&#160;pouring gently on the side of the dewar to avoid LN2 addition to the brass ethane vessel, until the liquid level just touches the brass ethane vessel. Place the foam lid on the plunging dewar to facilitate ethane solidification.
	<ol>
		<li>LN2 must directly contact the brass ethane vessel to aid in the solidification of ethane. After approximately 5 minutes, the ethane within the brass vessel will become completely frozen solid. Add more LN2 until it just touches the ethane vessel and proceed to the next step.</li>
	</ol>
	</li>
	<li>If the ethane has not frozen solid, then the brass ethane vessel is not cold enough for the remaining steps. Add more LN2 until it just touches the ethane vessel and wait an additional 5 minutes. Ensure that the ethane within the brass vessel is completely frozen solid.</li>
	<li>Open the gas outlet valve to produce an ethane gas flow at a similar rate as determined in step 4.6. Vertically place the metal ethane dispensing tip into the solid ethane and continue to move the ethane dispensing tip in a circular motion to melt the solid ethane.
	<ol>
		<li>Continue to add ethane until it is level with the top of the brass ethane vessel. Slowly remove the tip from the ethane vessel and close the ethane tank outlet valve. Cover the dewar with the lid for ~1-4 minute(s) to let the ethane solidify around the edges of the brass ethane vessel. 
		NOTE: An ideal ethane vessel will have a 2-3 mm symmetric ring of solid ethane at the perimeter of the brass ethane vessel with liquid ethane in the center (Figure 1D and Figure 2).</li>
		<li>Ensure that the ethane be as cold as possible without solidifying to ensure proper vitrification of the biological specimen. Failure to properly prepare the liquid ethane can result in inadequate vitrification of the specimen, ice accumulation, and/or loss of specimen, each contributing to the deterioration of specimen quality for imaging.</li>
		<li>If a solid ring of ethane does not form after 2-3 minutes, add more LN2 to the dewar and cover for 2-5 more minutes.</li>
		<li>If the ethane is solidifying too quickly, then use a large pair of clean tweezers to gently warm the ethane vessel and/or solid ethane to prevent complete ethane solidification. Once the ethane and LN2 are stable, close all the ethane tank valves and locate the plunging dewar to the manual plunger. Secure the plunging dewar to the manual plunger. 
		CAUTION: Be extra careful when transferring the dewar as LN2 can spill into the ethane vessel and solidify the liquid ethane. If need be, a clean set of tweezers can be used to melt any solid ethane in the middle of the vessel.</li>
	</ol>
	</li>
	<li>Test the location of the ethane dewar with a pair of empty tweezers to ensure the tweezer tip locates at the center of the ethane vessel and there is sufficient space for the grid and tweezer tip inside the liquid ethane (Figure 1D).
	<ol>
		<li>If the solid ethane ring is too thick for easy grid handling, then use a pair of room temperature, clean tweezers to melt the solid ethane and create more freezing area at the center of the ethane vessel.</li>
	</ol>
	</li>
</ol>
5. Prepare EM grids
NOTE: Estimated operating time: 1-5 minutes
<ol>
	<li>Add the grid storage box(es) to the dewar, unscrew the grid storage box lid(s), and make sure each lid can freely rotate to a new grid slot.</li>
	<li>Carefully transfer grids from the grid storage box to the edge of the square glass coverslip with ~30-40% of the grid off the slide edge. Ensure that the grid foil is facing up. Ensure grids are covered when not in use. Placing the grids over the edge of the square glass coverslip provides ease of grid handling and decreases the chance of bending or damaging the grid during transfer. 
	NOTE: 4-6 grids are typically prepared at a time.</li>
	<li>Render grids hydrophilic using a glow discharger or plasma cleaner. 
	NOTE: Please refer to the recommended guidelines for grid cleaning provided by the glow discharger/plasma cleaner manufacturer.
	<ol>
		<li>Use the grids within 10 minutes of plasma cleaning as the grids lose hydrophilicity and grid-to-grid reproducibility decreases after this time.</li>
	</ol>
	</li>
</ol>
6. Prepare cryoEM specimen by plunge freezing
NOTE: Estimated operating time: &#62;10 minutes (~1-3 min per grid)
<ol>
	<li>Use a clean and dry clamping tweezer to pick up a cleaned grid, slide the plastic clamp down to fix the grid in place, and gently tap the tweezers to ensure the grid is properly secured.
	<ol>
		<li>Handle grids by the outer ring to prevent damage to the grid foil.</li>
	</ol>
	</li>
	<li>Apply 1 to 5 &#181;L of sample to the prepared side (e.g., front or foil side) of the grid. 
	NOTE: The optimal volume and blotting time depends on the sample and needs to be optimized for each sample; larger volumes and more viscous samples require longer blotting times.</li>
	<li>Secure the tweezer-grid-sample assembly to the manual plunging arm by wrapping tape around the tweezer handle.
	<ol>
		<li>Face the sample towards the user for traditional front blotting. If the sample requires back blotting, then locate the sample away from the user.</li>
	</ol>
	</li>
	<li>Hold a clean, dry, cut piece of blotting paper between the thumb and index finger of each hand.
	<ol>
		<li>Only handle the blotting papers from the edges and never touch the center as oils and other contaminants from hands/gloves can alter grid quality.</li>
	</ol>
	</li>
	<li>Rest hands on the edge of the plunging dewar to establish a stable position. Locate the blotting paper parallel to the grid surface approximately 1 cm away from the grid surface.
	<ol>
		<li>Use the middle section of the blotting paper to allow for complete fluid mobility and even wicking across the grid surface.</li>
	</ol>
	</li>
	<li>Gently slide and rotate the thumb and ring fingers towards each other to bend blotting paper toward the grid to initiate blotting. Maintain contact between the blotting paper and the grid surface during the entire blotting process.
	<ol>
		<li>Directly contact the blotting paper to the grid surface and maintain consistent contact across the grid surface.</li>
		<li>Gently bending the blotting paper decreases bending of the grid and/or damage to the grid surface, and results in more consistent ice across the grid (Figure 3A).</li>
	</ol>
	</li>
	<li>Observe the mobile liquid front and once it stops progressing into the blotting paper begin counting for 4 to 6 seconds. 
	NOTE: Counting can occur once the blotting paper contacts the grid surface but lower grid-to-grid reproducibility can occur. The total blot time will depend on the grid type, foil type, sample concentration, and sample type (e.g., soluble versus membrane versus filamentous proteins). For more viscous samples longer blot times (e.g.., 5 to 7 seconds) will be required.
	<ol>
		<li>Important: Develop a reliable and consistent counting scheme to greatly enhance reproducibility during the freezing process.</li>
	</ol>
	</li>
	<li>Move the left, right thumb and index fingers in opposite directions to remove the blotting paper in a &#34;snapping motion&#34; away from the grid surface. Immediately depress the foot pedal to release the plunging arm and plunge the grid into liquid ethane.
	<ol>
		<li>Simultaneously remove the blotting paper and press the foot pedal to plunge the grid into the ethane as soon as possible for best freezing results. The longer the time between blotting paper removal and plunging, the more evaporation of thin films will occur and decrease grid-to-grid reproducibility.</li>
	</ol>
	</li>
	<li>Use one hand to stabilize the clamping tweezers, unwind tape carefully from around the tweezers and manual plunging arm.
	<ol>
		<li>Always maintain contact with the tweezer to prevent movement of the tweezer-grid and limit grid damage that occur from knocking the grid against the solid ethane.</li>
	</ol>
	</li>
	<li>Once clamping tweezers are free from the manual plunging arm, maintain the tweezer in one hand resting on top of the plunging dewar, ensure the grid remains in the liquid ethane. Carefully slide the plastic clamp away from the grid so the grid can be transferred. Maintain pressure on the tweezers to retain the grid.
	<ol>
		<li>With one swift motion, quickly transfer the grid from the ethane vessel into the LN2 reservoir. Carefully place the grid in the grid storage box. 
		NOTE: Some ethane may solidify on the grid surface. Opening the tweezer slightly will break the ethane and allow for the grid to be dropped into the grid box.</li>
	</ol>
	</li>
	<li>Wrap the tip of the tweezers in a delicate task wipe to prevent frost accumulation. Set aside until the tweezers have returned to room temperature.
	<ol>
		<li>Have 4 to 6 tweezers on hand for ease of use. Each tweezer will be used for sample freezing and warmed before subsequent use.</li>
	</ol>
	</li>
	<li>Repeat steps 6.1-6.11 for each grid.</li>
	<li>Once freezing has culminated, securely close the grid box and transfer to a proper storage location.</li>
	<li>Carefully dispose of the liquid ethane and LN2 and store all materials in a dry location.</li>
</ol>

We have nothing to disclose.

The vitrification of biological specimens for imaging by single-particle cryogenic electron microscopy (cryoEM) remains a critically important step for successful structure determination. The manual blot-and-plunge method described in this protocol represents a cost-effective, reliable, and robust method for quickly freezing biological samples in thin films of vitreous ice for cryoEM imaging. Using the methods outlined in the manuscript, researchers will be able to assemble and operate the manual plunger, prepare cryogen...

Single-particle cryogenic electron microscopy (cryoEM) is a powerful structural technique that can be used to solve structures of dynamic biological specimens to near-atomic resolution1,2,3,4. Indeed, recent advances in direct electron detector technologies4,5,6,7,8,9,10, improvements in electron sources4,11,12,13,14, and electromagnetic lens stability15, coupled with the continued development of data acquisition16,17 and analysis software packages18,19, have enabled researchers to now routinely determine structures of well-behaved specimens to 3 &#197; resolution or better4,11,13,14,20,21,22,23. Despite these improved imaging and data processing capabilities, cryoEM grid preparation remains the largest impediment for successful high-resolution structure determination and often serves as a considerable bottleneck in the EM workflow24,25,26,27.
CryoEM relies on the imaging of biological samples in aqueous solutions that are frozen to form a thin film of &#34;glass-like&#34; ice - a process known as vitrification - that preserves the native biochemical state. Vitrification of biological samples for cryoEM dates back over 40 years28,29,30 and many techniques and equipment that have been developed for this process rely on the originally detailed blot-and-plunge method31,32,33,34,35, whereby a small volume of sample (e.g., 1-5 &#181;L) is applied to a specialized EM grid before the excess solution is removed using physical interaction of the grid with blotting paper. The timing of this process is usually empirically determined for each specimen as a critical component of freezing samples is the thickness of the vitreous ice film - if the ice is too thick then imaging quality deteriorates dramatically due to increased scattering of the electron beam while ice that is too thin can restrict protein orientations and/or exclude particles from the center of the grid foil holes36. This reliance on the perfect ice thickness for single-particle cryoEM has led to a wide array of techniques and equipment that can freeze samples, including robotics37,38, microfluidics42, and ultrasonic or spraying devices27,39,40,41,42,43,44. In recent years, some of the most popular sample preparation devices rely on the use of robotics for automated freezing of samples using the blot-and-plunge technique45. While these devices are designed to reproducibly create proper ice thickness for imaging, they often remain too expensive for individual labs to purchase and operate and are generally found within cryoEM facilities at hourly rates for usage. In recent years, the original manual blot-and-plunge technique has come back into increased use3,47,48,49,50,51,52. Indeed, a manually operated blot-and-plunge device can achieve high-quality cryoEM grids at a fraction of the cost of robotic counterparts.&#160;Furthermore, manual blotting also offers more users control over blotting as researchers can adjust the type of blotting (i.e., back-blotting of the grid, front-blotting of the grid, etc.), and blotting time based on each individual sample and research questions.
In this article, we provide details on how to effectively freeze biological samples using a traditional manual blot-and-plunge vitrification device coupled with a custom-designed dewar platform53. Best practices, including preparation of the cryogen, grid handling, sample application, and blotting, as well as common pitfalls and recommendations on how to overcome these hurdles are provided. Advice on how to increase ice thickness reproducibility between grid preparations and how to modify sample blotting based on biological specimen type are discussed. Given the low cost associated with the purchase and operation of the manual plunger described in this manuscript, labs across the globe can prepare biological specimens for cryoEM in a cost-effective and reproducible manner.

<table><tbody><tr><td>4 slot grid storage box</td><td>Ted Pella</td><td>160-40</td><td></td></tr><tr><td>14 gauge flat metal dispensing tip</td><td>Amazon</td><td>B07M7YWWLT</td><td></td></tr><tr><td>22x22 mm square glass coverslip</td><td>Sigma</td><td>C9802-1PAK</td><td></td></tr><tr><td>60 mm glass Petri dish to store grids</td><td>Fisher</td><td>08-747A</td><td></td></tr><tr><td>100 mm glass Petri dish to store Whatman paper</td><td>Fisher</td><td>08-747D</td><td></td></tr><tr><td>150 mm glass Petri dish to store Whatman paper</td><td>Fisher</td><td>08-747F</td><td></td></tr><tr><td>250 mL beaker</td><td>Fisher</td><td>02-555-25B</td><td></td></tr><tr><td>Blue styrofoam dewar</td><td>Spear Lab</td><td>FD-500</td><td></td></tr><tr><td>Brass ethane vessel</td><td>Lasco</td><td>17-4075</td><td></td></tr><tr><td>Clamping tweezers</td><td>Ted Pella</td><td>38825</td><td></td></tr><tr><td>Delicate task wipes</td><td>Fisher</td><td>06-666</td><td></td></tr><tr><td>Dual-stage regulator with control valve</td><td>Airgas</td><td>Y12N245D580-AG</td><td></td></tr><tr><td>Dewer grid base</td><td>UCSD</td><td></td><td></td></tr><tr><td>Ethane platform</td><td>UCSD</td><td></td><td></td></tr><tr><td>Ethane propane tank</td><td>Praxair</td><td>ET PR50ZU-G</td><td>ethane (50%) : propane (50%) in a high-pressure tank</td></tr><tr><td>Ethane tank</td><td>Praxair</td><td>UN1035</td><td>ethane (100%)</td></tr><tr><td>Flexible arm task light</td><td>Amscope</td><td>LED-11CR</td><td></td></tr><tr><td>Grids (UltrAufoil R 1.2/1.3 300 mesh)</td><td>Electron Microscopy Sciences</td><td>Q325AR1.3</td><td></td></tr><tr><td>Humidifier</td><td>Target</td><td>719438</td><td></td></tr><tr><td>Hygrometer</td><td>ThermoPro</td><td>B01H1R0K68</td><td></td></tr><tr><td>Lab coat</td><td>UCSD</td><td></td><td></td></tr><tr><td>Liquid Nitrogen dewar</td><td>Worthington</td><td>LD4</td><td></td></tr><tr><td>Liquid Nitrogen gloves</td><td>Fisher</td><td>19-059-925</td><td></td></tr><tr><td>Manual plunger stand (black stand + foot pedal)</td><td>UCSD</td><td></td><td></td></tr><tr><td>Mark 5 (plunging platform)</td><td>UCSD</td><td></td><td></td></tr><tr><td>Nitrile gloves</td><td>VWR</td><td>82026-424</td><td></td></tr><tr><td>P20 pipette</td><td>Eppendorf</td><td>13-690-029</td><td></td></tr><tr><td>PCR tubes</td><td>Eppendorf</td><td>E0030124286</td><td></td></tr><tr><td>Pipette tips</td><td>ibis scientific</td><td>63300005</td><td></td></tr><tr><td>Ring lamp</td><td>Amazon</td><td>B07HMR4H8G</td><td></td></tr><tr><td>Safety glasses</td><td>UCSD</td><td></td><td></td></tr><tr><td>Scissors</td><td>Amazon</td><td>Fiskars 01-004761J</td><td></td></tr><tr><td>Screw driver</td><td>Ironside</td><td>354711</td><td></td></tr><tr><td>Tape</td><td>Fisher</td><td>15-901-10R</td><td></td></tr><tr><td>Tweezer to transfer grid box</td><td>Amazon</td><td>LTS-3</td><td></td></tr><tr><td>Tygon tubing</td><td>Fisher</td><td>14-171-130</td><td></td></tr><tr><td>Whatman blotting paper</td><td>Fisher</td><td>1001-090</td><td></td></tr></tbody></table>

manual blot-and-plunge freezing of biological specimens for single-particle cryogenic electron microscopy

Imaging biological specimens with electrons for high-resolution structure determination by single-particle cryogenic electron microscopy (cryoEM) requires a thin layer of vitreous ice containing the biomolecules of interest. Despite numerous technological advances in recent years that have propelled single-particle cryoEM to the forefront of structural biology, the methods by which specimens are vitrified for high-resolution imaging often remain the rate-limiting step. Although numerous recent efforts have provided means to overcome hurdles frequently encountered during specimen vitrification, including the development of novel sample supports and innovative vitrification instrumentation, the traditional manually operated plunger remains a staple in the cryoEM community due to the low cost to purchase and ease of operation. Here, we provide detailed methods for using a standard, guillotine-style manually operated blot-and-plunge device for the vitrification of biological specimens for high-resolution imaging by single-particle cryoEM. Additionally, commonly encountered issues and troubleshooting recommendations for when a standard preparation fails to yield a suitable specimen are also described.

Successful execution of the blot-and-plunge protocol described here will result in a thin, uniform layer of vitreous ice that is free of any hexagonal ice, contaminants, and large gradients of unusable ice which can be observed under the electron microscope (Figure 3). Inconsistent contact of the blotting paper with the grid surface, prematurely removing the blotting paper, or moving the blotting paper during grid contact can decrease the quality of the vitreous ice and lead to inconsistent ...

Watch this Scientific Journal Video about Manual Blot-and-Plunge Freezing of Biological Specimens for Single-Particle Cryogenic Electron Microscopy at JoVE.com

Manual Blot-and-Plunge Freezing of Biological Specimens for Single-Particle Cryogenic Electron Microscopy

This manuscript outlines the blot-and-plunge method to manually freeze biological specimens for single-particle cryogenic electron microscopy.

Imaging biological specimens with electrons for high-resolution structure determination by single-particle cryogenic electron microscopy (cryoEM) requires ...

manual-blot-plunge-freezing-biological-specimens-for-single-particle

Research

JoVE Journal

Biochemistry

6.2K Views.  University of California, San Diego. This manuscript outlines the blot-and-plunge method to manually freeze biological specimens for single-particle cryogenic electron microscopy.

Video: Manual Blot-and-Plunge Freezing of Biological Specimens for Single-Particle Cryogenic Electron Microscopy

Single Particle Cryo-Electron Microscopy: From Sample to Structure

Cryo-electron microscopy (cryoEM) is a powerful technique for structure determination of macromolecular complexes, via single particle analysis (SPA). The overall process involves i) vitrifying the specimen in a thin film supported on a cryoEM grid; ii) screening the specimen to assess particle distribution and ice quality; iii) if the grid is suitable, collecting a single particle dataset for analysis; and iv) image processing to yield an EM density map. In this protocol, an overview for each of these steps is provided, with a focus on the variables which a user can modify during the workflow and the troubleshooting of common issues. With remote microscope operation becoming standard in many facilities, variations on imaging protocols to assist users in efficient operation and imaging when physical access to the microscope is limited will be described.

Structure determination of macromolecular complexes using cryoEM has become routine for certain classes of proteins and complexes. Here, this pipeline is summarized (sample preparation, screening, data acquisition and processing) and readers are directed towards further detailed resources and variables that may be altered in the case of more challenging specimens.

Cryo-electron microscopy (cryoEM) is a powerful technique for structure determination of macromolecular complexes, via single particle analysis (SPA). The ...

Electron Cryotomography of Bacterial Cells

While much is already known about the basic metabolism of bacterial cells, many fundamental questions are still surprisingly unanswered, including for instance how they generate and maintain specific cell shapes, establish polarity, segregate their genomes, and divide. In order to understand these phenomena, imaging technologies are needed that bridge the resolution gap between fluorescence light microscopy and higher-resolution methods such as X-ray crystallography and NMR spectroscopy.
Electron cryotomography (ECT) is an emerging technology that does just this, allowing the ultrastructure of cells to be visualized in a near-native state, in three dimensions (3D), with "macromolecular" resolution (~4nm).1, 2 In ECT, cells are imaged in a vitreous, "frozen-hydrated" state in a cryo transmission electron microscope (cryoTEM) at low temperature (&lt; -180&deg;C). For slender cells (up to ~500 nm in thickness3), intact cells are plunge-frozen within media across EM grids in cryogens such as ethane or ethane/propane mixtures. Thicker cells and biofilms can also be imaged in a vitreous state by first "high-pressure freezing" and then, "cryo-sectioning" them. A series of two-dimensional projection images are then collected through the sample as it is incrementally tilted along one or two axes. A three-dimensional reconstruction, or "tomogram" can then be calculated from the images. While ECT requires expensive instrumentation, in recent years, it has been used in a few labs to reveal the structures of various external appendages, the structures of different cell envelopes, the positions and structures of cytoskeletal filaments, and the locations and architectures of large macromolecular assemblies such as flagellar motors, internal compartments and chemoreceptor arrays.1, 2
In this video article we illustrate how to image cells with ECT, including the processes of sample preparation, data collection, tomogram reconstruction, and interpretation of the results through segmentation and in some cases correlation with light microscopy.

We illustrate here how to use electron cryotomography (ECT) to study the ultrastructure of bacterial cells in near-native states, to "macromolecular" (~4 nm) resolution.

While much is already known about the basic metabolism of bacterial cells, many fundamental questions are still surprisingly unanswered, including for ...

Biology

The Peel-Blot Technique: A Cryo-EM Sample Preparation Method to Separate Single Layers From Multi-Layered or Concentrated Biological Samples

The peel-blot cryo-EM grid preparation technique is a significantly modified back-injection method with the objective of achieving a reduction in layers of multi-layered samples. This removal of layers prior to plunge freezing can aid in reducing sample thickness to a level suitable for cryo-EM data collection, improving sample flatness, and facilitating image processing. The peel-blot technique allows for the separation of multilamellar membranes into single layers, of layered 2D crystals into individual crystals, and of stacked, sheet-like structures of soluble proteins to likewise be separated into single layers. The high sample thickness of these types of samples frequently poses insurmountable problems for cryo-EM data collection and cryo-EM image processing, especially when the microscope stage must be tilted for data collection. Furthermore, grids of high concentrations of any of these samples can be prepared for efficient data collection since sample concentration prior to grid preparation can be increased and the peel-blot technique adjusted to result in a dense distribution of single-layered specimen.

The peel-blot technique is a cryo-EM grid preparation method that allows for the separation of multilayered and concentrated biological samples into single layers to reduce thickness, increase sample concentration, and facilitate image processing.

The peel-blot cryo-EM grid preparation technique is a significantly modified back-injection method with the objective of achieving a reduction in layers ...

Nano-fEM: Protein Localization Using Photo-activated Localization Microscopy and Electron Microscopy

Mapping the distribution of proteins is essential for understanding the function of proteins in a cell. Fluorescence microscopy is extensively used for protein localization, but subcellular context is often absent in fluorescence images. Immuno-electron microscopy, on the other hand, can localize proteins, but the technique is limited by a lack of compatible antibodies, poor preservation of morphology and because most antigens are not exposed to the specimen surface. Correlative approaches can acquire the fluorescence image from a whole cell first, either from immuno-fluorescence or genetically tagged proteins. The sample is then fixed and embedded for electron microscopy, and the images are correlated 1-3. However, the low-resolution fluorescence image and the lack of fiducial markers preclude the precise localization of proteins. 
Alternatively, fluorescence imaging can be done after preserving the specimen in plastic. In this approach, the block is sectioned, and fluorescence images and electron micrographs of the same section are correlated 4-7. However, the diffraction limit of light in the correlated image obscures the locations of individual molecules, and the fluorescence often extends beyond the boundary of the cell. 
Nano-resolution fluorescence electron microscopy (nano-fEM) is designed to localize proteins at nano-scale by imaging the same sections using photo-activated localization microscopy (PALM) and electron microscopy. PALM overcomes the diffraction limit by imaging individual fluorescent proteins and subsequently mapping the centroid of each fluorescent spot 8-10. 
We outline the nano-fEM technique in five steps. First, the sample is fixed and embedded using conditions that preserve the fluorescence of tagged proteins. Second, the resin blocks are sectioned into ultrathin segments (70-80 nm) that are mounted on a cover glass. Third, fluorescence is imaged in these sections using the Zeiss PALM microscope. Fourth, electron dense structures are imaged in these same sections using a scanning electron microscope. Fifth, the fluorescence and electron micrographs are aligned using gold particles as fiducial markers. In summary, the subcellular localization of fluorescently tagged proteins can be determined at nanometer resolution in approximately one week.

We describe a method to localize fluorescently tagged proteins in electron micrographs. Fluorescence is first localized using photo-activated localization microscopy on ultrathin sections. These images are then aligned to electron micrographs of the same section.

Mapping the distribution of proteins is essential for understanding the function of proteins in a cell. Fluorescence microscopy is extensively used for ...

Cryo-electron Microscopy Specimen Preparation By Means Of a Focused Ion Beam

Here we present a protocol used to prepare cryo-TEM samples of Aspergillus niger spores, but which can easily be adapted for any number of microorganisms or solutions. We make use of a custom built cryo-transfer station and a modified cryo-SEM preparation chamber2. The spores are taken from a culture, plunge-frozen in a liquid nitrogen slush and observed in the cryo-SEM to select a region of interest. A thin lamella is then extracted using the FIB, attached to a TEM grid and subsequently thinned to electron transparency. The grid is transferred to a cryo-TEM holder and into a TEM for high resolution studies. Thanks to the introduction of a cooled nanomanipulator tip and a cryo-transfer station, this protocol is a straightforward adaptation to cryogenic temperature of the routinely used FIB preparation of TEM samples. As such it has the advantages of requiring a small amount of modifications to existing instruments, setups and procedures; it is easy to implement; it has a broad range of applications, in principle the same as for cryo-TEM sample preparation. One limitation is that it requires skillful handling of the specimens at critical steps to avoid or minimize contaminations.

Cryo Electron Microscopes, either Scanning (SEM) or Transmission (TEM), are widely used for characterization of biological samples or other materials with a high water content1. A SEM/Focused Ion Beam (FIB) is used to identify features of interest in samples and extract a thin, electron-transparent lamella for transfer to a cryo-TEM.

Here we present a protocol used to prepare cryo-TEM samples of Aspergillus niger spores, but which can easily be adapted for any number of microorganisms ...

Plunge Freezing: A Tool for the Ultrastructural and Immunolocalization Studies of Suspension Cells in Transmission Electron Microscopy

Transmission Electron Microscopy (TEM) is an extraordinary tool for studying cell ultrastructure, in order to localize proteins and visualize macromolecular complexes at very high resolution. However, to get as close as possible to the native state, perfect sample preservation is required. Conventional electron microscopy (EM) fixation with aldehydes, for instance, does not provide good ultrastructural preservation. The slow penetration of fixatives induces cell reorganization and loss of various cell components. Therefore, conventional EM fixation does not allow for an instantaneous stabilization and preservation of structures and antigenicity. The best choice for examining intracellular events is to use cryofixation followed by the freeze-substitution fixation method that keeps cells in their native state. High-pressure freezing/freeze-substitution, which preserves the integrity of cellular ultrastructure, is the most commonly used method, but requires expensive equipment. Here, an easy-to-use and low-cost freeze fixation method followed by freeze-substitution for suspension cell cultures is presented.

This manuscript describes an easy-to-use and low-cost cryofixation method for visualizing suspension cells by transmission electron microscopy.

Transmission Electron Microscopy (TEM) is an extraordinary tool for studying cell ultrastructure, in order to localize proteins and visualize ...

Flash-and-Freeze: A Novel Technique to Capture Membrane Dynamics with Electron Microscopy

Cells constantly change their membrane architecture and protein distribution, but it is extremely difficult to visualize these events at a temporal and spatial resolution on the order of ms and nm, respectively. We have developed a time-resolved electron microscopy technique, &#34;flash-and-freeze,&#34; that induces cellular events with optogenetics and visualizes the resulting membrane dynamics by freezing cells at defined time points after stimulation. To demonstrate this technique, we expressed channelrhodopsin, a light-sensitive cation channel, in mouse hippocampal neurons. A flash of light stimulates neuronal activity and induces neurotransmitter release from synaptic terminals through the fusion of synaptic vesicles. The optogenetic stimulation of neurons is coupled with high-pressure freezing to follow morphological changes during synaptic transmission. Using a commercial instrument, we captured the fusion of synaptic vesicles and the recovery of the synaptic vesicle membrane. To visualize the sequence of events, large datasets were generated and analyzed blindly, since morphological changes were followed in different cells over time. Nevertheless, flash-and-freeze allows the visualization of membrane dynamics in electron micrographs with ms temporal resolution.

We developed a novel technique in electron microscopy, &#34;flash-and-freeze,&#34; that enables the visualization of membrane dynamics with ms temporal resolution. This technique combines the optogenetic stimulation of neurons with high-pressure freezing. Here, we demonstrate the procedures and describe the protocols in detail.

Cells constantly change their membrane architecture and protein distribution, but it is extremely difficult to visualize these events at a temporal and ...

Miniaturized Sample Preparation for Transmission Electron Microscopy

Due to recent technological progress, cryo-electron microscopy (cryo-EM) is rapidly becoming a standard method for the structural analysis of protein complexes to atomic resolution. However, protein isolation techniques and sample preparation methods for EM remain a bottleneck. A relatively small number (100,000 to a few million) of individual protein particles need to be imaged for the high-resolution analysis of proteins by the single particle EM approach, making miniaturized sample handling techniques and microfluidic principles feasible.
A miniaturized, paper-blotting-free EM grid preparation method for sample pre-conditioning, EM grid priming and post processing that only consumes nanoliter-volumes of sample is presented. The method uses a dispensing system with sub-nanoliter precision to control liquid uptake and EM grid priming, a platform to control the grid temperature thereby determining the relative humidity above the EM grid, and a pick-and-plunge-mechanism for sample vitrification. For cryo-EM, an EM grid is placed on the temperature-controlled stage and the sample is aspirated into a capillary. The capillary tip is positioned in proximity to the grid surface, the grid is loaded with the sample and excess is re-aspirated into the microcapillary. Subsequently, the sample film is stabilized and slightly thinned by controlled water evaporation regulated by the offset of the platform temperature relative to the dew-point. At a given point the pick-and-plunge mechanism is triggered, rapidly transferring the primed EM grid into liquid ethane for sample vitrification. Alternatively, sample-conditioning methods are available to prepare nanoliter-sized sample volumes for negative stain (NS) EM.
The methodologies greatly reduce sample consumption and avoid approaches potentially harmful to proteins, such as the filter paper blotting used in conventional methods. Furthermore, the minuscule amount of sample required allows novel experimental strategies, such as fast sample conditioning, combination with single-cell lysis for &#34;visual proteomics,&#34; or &#34;lossless&#34; total sample preparation for quantitative analysis of complex samples.

An instrument and methods for the preparation of nanoliter-sized sample volumes for transmission electron microscopy is presented. No paper-blotting steps are required, thus avoiding the detrimental consequences this can have for proteins, significantly reducing sample loss and enabling the analysis of single cell lysate for visual proteomics.

Due to recent technological progress, cryo-electron microscopy (cryo-EM) is rapidly becoming a standard method for the structural analysis of protein ...

Biological Sample Preparation by High-pressure Freezing, Microwave-assisted Contrast Enhancement, and Minimal Resin Embedding for Volume Imaging

The described sample preparation technique is designed to combine the best quality of ultrastructural preservation with the most suitable contrast for the imaging modality in a focused ion beam scanning electron microscope (FIB-SEM), which is used to obtain stacks of sequential images for 3D reconstruction and modelling. High-pressure freezing (HPF) allows close to native structural preservation, but the subsequent freeze substitution often does not provide sufficient contrast, especially for a bigger specimen, which is needed for high-quality imaging in the SEM required for 3D reconstruction. Therefore, in this protocol, after the freeze substitution, additional contrasting steps are carried out at room temperature. Although these steps are performed in a microwave, it is also possible to follow traditional bench processing, which requires longer incubation times.The subsequent embedding in minimal amounts of resin allows for faster and more precise targeting and preparation inside the FIB-SEM. This protocol is especially useful for samples that require preparation by high-pressure freezing for a reliable ultrastructural preservation but do not gain enough contrast during the freeze substitution for volume imaging using FIB-SEM. In combination with the minimal resin embedding, this protocol provides an efficient workflow for the acquisition of high-quality volume data.

Here we present a protocol for combining two sample processing techniques, high-pressure freezing and microwave-assisted sample processing, followed by minimal resin embedding for acquiring data with a focused ion beam scanning electron microscope (FIB-SEM). This is demonstrated using a mouse tibial nerve sample and Caenorhabditis elegans.

The described sample preparation technique is designed to combine the best quality of ultrastructural preservation with the most suitable contrast for the ...

Rapid Freezing using Sandwich Freezing Device for Good Ultrastructural Preservation of Biological Specimens in Electron Microscopy

Chemical fixation has been used for observing the ultrastructure of cells and tissues. However, this method does not adequately preserve the ultrastructure of cells; artifacts and extraction of cell contents are usually observed. Rapid freezing is a better alternative for the preservation of cell structure. Sandwich freezing of living yeast or bacteria followed by freeze-substitution has been used for observing the exquisite natural ultrastructure of cells. Recently, sandwich freezing of glutaraldehyde-fixed cultured cells or human tissues has also been used to reveal the ultrastructure of cells and tissues. 
These studies have thus far been carried out with a handmade sandwich freezing device, and applications to studies in other laboratories have been limited. A new sandwich freezing device has recently been fabricated and is now commercially available. The present paper shows how to use the sandwich freezing device for rapid freezing of biological specimens, including bacteria, yeast, cultured cells, isolated cells, animal and human tissues, and viruses. Also shown is the preparation of specimens for ultrathin sectioning after rapid freezing and procedures for freeze-substitution, resin embedding, trimming of blocks, cutting of ultrathin sections, recovering of sections, staining, and covering of grids with support films.

Here we show how to use the sandwich freezing device for rapid freezing of biological specimens, including bacteria, yeast, cultured cells, isolated cells, animal and human tissues, and viruses. We also show how to prepare specimens for ultrathin sectioning after rapid freezing.