This work was supported by NIH grants R01GM080376, R35GM118139, and NSF Center for Engineering MechanoBiology CMMI: 15-48571 to Y.E.G., and by an NIAID pre-doctoral NRSA fellowship F30AI114187 to R.M.J.

NOTE: All steps can be completed in general lab space.
1. Glass coverslip cleaning
<ol>
	<li>To provide a clean surface for evaporative deposition of colloidal particles, place 24 x 30 mm optical borosilicate glass coverslips (0.16&#8722;0.19 mm thickness) within the grooved inserts of a coplin glass staining jar for cleaning. 
	NOTE: Make sure the coverslips stand upright and are well-separated so that all surfaces are clearly exposed during the cleaning process.</li>
	<li>Pour enough acetone in the staining jar to cover the coverslips, place the cover on, and sonicate for 10 min at 40 &#176;C.</li>
	<li>Pour out the acetone and rinse the coverslips by filling the staining jar with distilled H2O and pouring out the water. Repeat 2 more times.</li>
	<li>Repeat the acetone sonication (steps 1.2 and 1.3) once more.</li>
	<li>Pour enough 200 mM KOH in the jar to cover the coverslips and sonicate, covered, for 20 min at 40 &#176;C. 
	NOTE: The KOH slightly etches the glass.</li>
	<li>Rinse the coverslips with distilled H2O 6 times.</li>
	<li>Add ethanol to cover the coverslips, add the lid, and sonicate for 10 min at 40 &#176;C.</li>
	<li>Rinse the coverslips with distilled H2O 3 times.</li>
	<li>Pick up each coverslip at the edge using gentle forceps and dry the coverslips with N2 gas. Touch only the edges of the coverslip. Place each of the dried, cleaned coverslips in an individual clean Petri dish.</li>
</ol>
2. Evaporative deposition of polystyrene beads
<ol>
	<li>To create the colloidal crystal mask for the ZMW array, centrifuge 50 &#181;L of 1 &#181;m diameter, non-functionalized polystyrene beads (2.5% w/v in water) at 15,000 x g, 25 &#176;C for 5 min. 
	NOTE: Before pipetting the beads, the stock solution should be briefly vortexed in case the beads have settled to the bottom of the bottle.</li>
	<li>Discard the supernatant, leaving as little water remaining as possible. 
	NOTE: Residual water can change the evaporation properties of the ethanol resuspension39, so removal of a small amount of beads in order to remove all of the water is acceptable.</li>
	<li>Resuspend the beads from step 2.2 in 50 &#181;L of 1:400 TritonX-100:ethanol solvent. Pipette up and down several times to thoroughly mix the beads with the solvent. 
	NOTE: TritonX-100:ethanol solvent should be sealed with paraffin film after use and prepared fresh once a month. The beads tend to adhere to the sides of a plastic vessel, such as a microcentrifuge tube, so pipette along the sides to ensure that all beads are resuspended.</li>
	<li>To set up a humidity chamber for deposition, place 6 Petri dishes, each with one coverslip, on a bench in a line with lids left slightly ajar. In each dish, move the coverslip to the open region so that the coverslips are exposed to the environment when the humidity is increased in the next step.</li>
	<li>Place a hygrometer and a small electric fan centered behind the Petri dishes.</li>
	<li>Record the starting relative humidity (RH) in the lab. Fill a 200 mL beaker with 150&#8722;200 mL of ~75 &#176;C water and place it behind the fan.</li>
	<li>Turn on the fan and cover the Petri dishes, fan, beaker, and hygrometer with an overturned, transparent plastic storage container (66 cm x 46 cm x 38 cm).</li>
	<li>Let the RH in the chamber rise to 70&#8722;75%, which typically takes 5&#8722;10 min. 
	NOTE: If the ambient lab RH is low (below ~50%), let the chamber reach a higher RH, but no higher than 80%, to compensate for loss of humidity during deposition (see below).</li>
	<li>When the RH reaches 70&#8722;75%, record the RH and lift up the plastic storage container slightly to quickly place covers on the Petri dishes, which prevents over-wetting of the coverslips. 
	NOTE: The temperature in the chamber will be slightly warmer than room temperature, typically 25&#8722;26 &#176;C, as a result of humidification. If moisture is visible on the coverslips, then the glass surfaces are too wet. A commercial glove box might simplify this part of the protocol.</li>
	<li>Let the RH in the chamber continue to rise to 85%. At that point, record the RH in the humidity chamber and pipette 5 &#181;L of the bead suspension onto the center of each coverslip.</li>
	<li>Close the chamber and Petri dishes after each deposition to minimize loss of humidity. Aim to finish all 6 depositions within 2 min.</li>
	<li>Record the RH in the chamber after the deposition. 
	NOTE: The RH after deposition will help gauge how fast humidity was lost during deposition, which depends on ambient lab conditions. For a typical successful run, the chamber will start at 85% RH prior to deposition and end at 70&#8722;75% RH after the deposition.</li>
	<li>Let the bead droplets spread and dry for 5 min. 
	NOTE: If the colloidal crystals have many holes or multilayered regions, then the chamber was likely too humid or dry, respectively. Adjust the relative humidity at which to close the Petri dishes and begin the depositions (see the results section for further discussion of optimization).</li>
</ol>
3. Bead annealing for reducing pore size in the colloidal crystal template
<ol>
	<li>To provide a uniform temperature surface for annealing of the polystyrene beads, which narrows the inter-bead interstices and rounds the interstices&#8217; corners, place a flat, milled aluminum plate on top of a standard ceramic hot plate.</li>
	<li>Set the temperature of the hot plate to 107 &#176;C, the glass transition temperature of polystyrene40. 
	NOTE: To obtain stable and accurate temperature, a thermocouple probe was held in a 2&#8722;3 mm wide and 4&#8722;5 mm deep hole in the aluminum plate.</li>
	<li>Place a coverslip containing the bead template on the hot aluminum plate and anneal for 20 s (see the discussion section for explanation of melting time).</li>
	<li>After heating, remove the coverslip from the aluminum plate and promptly place it on another room temperature aluminum surface to cool it. 
	NOTE: It is helpful to either have the coverslips hang slightly over the edge of the plate or mill shallow channels (see the accompanying video) into the plate to facilitate pickup of the coverslips.</li>
</ol>
4. Nanofabrication of aluminum zero mode waveguides using the colloidal crystal template
<ol>
	<li>Using thermal or electron-beam evaporative deposition, deposit 300 nm of copper at 2 &#197;/s over the colloidal crystal template to generate posts in the interstices between the beads.</li>
	<li>Remove excess metal on top of the beads by gently pressing the surface with tape. Slowly peel the tape to pull off the metal. 
	NOTE: Some small patches of reflective excess metal may remain after the tape pull, and these can often be removed by a stream of N2 gas. If substantial patches of reflective excess metal remain after the tape pull, try soaking the templates in toluene for 2 h to partially dissolve the polystyrene beads. Wash the coverslips with distilled water, dry with N2, and repeat the tape pull. The additional soak should not completely dissolve the beads, as the beads help protect the posts from damage during the tape pull.</li>
	<li>To dissolve the polystyrene beads, place the bead templates in toluene and soak overnight. 
	CAUTION: Toluene fumes may be toxic. Work with toluene under a well-ventilated hood and wear personal protective equipment, including gloves, safety glasses, and a lab coat. Toluene should be stored in ventilated cabinets designated for flammable liquids.</li>
	<li>After the toluene incubation, rinse the templates once with chloroform and twice with ethanol. Handle coverslips carefully at this point because the delicate 200&#8722;300 nm tall metal posts are now exposed. Dry the templates with N2 and remove residual polymer and contaminants in an oxygen plasma cleaner for 30 min. 
	CAUTION: Chloroform fumes may be toxic. Work with chloroform under a well-ventilated hood and wear personal protective equipment, including gloves, safety glasses, and a lab coat. Chloroform should be stored in ventilated cabinets away from other flammable solvents.</li>
	<li>Using thermal or electron-beam evaporative deposition, deposit 3 nm of a titanium adhesion layer at 1 &#197;/s followed by 100&#8722;150 nm of aluminum at 4 &#197;/s around and on top of the copper posts. 
	NOTE: One can use thicker cladding to obtain deeper guides and better attenuation of background fluorescence, but this also decreases the yield after exposing and dissolving the posts in the next step (see the discussion section).</li>
	<li>To dissolve the metal posts, soak the coverslips in copper etchant (citric acid-based; Table of Materials) for 2 h. 
	CAUTION: Metal etchant can cause skin burns. Work with etchants under a well-ventilated hood and wear protective equipment. Wash hands thoroughly after handling. Metal etchant should be stored in ventilated cabinets designated for corrosive liquids.</li>
	<li>Rinse the coverslips with distilled water, dry with N2, and gently buff the surface of the metal cladding with lens paper to expose any posts that are still covered in cladding. Place the coverslips back in copper etchant for another 2 h, then rinse again with distilled water and dry with N2. 
	NOTE: ZMW slides should be stored in covered, clean Petri dishes to keep them free of contaminants.</li>
</ol>
5. Nanofabrication of gold zero mode waveguides using the colloidal crystal template
NOTE: The method to fabricate gold ZMWs (Supplemental Figure 1), which mirrors the protocol to fabricate aluminum ZMWs, is provided in this section.
<ol>
	<li>Using thermal or electron beam evaporative deposition, deposit 3 nm of a titanium adhesion layer at 1 &#197;/s followed by 300 nm of aluminum at 4 &#197;/s.</li>
	<li>Remove excess metal on top of the beads by gently pressing the surface with tape. Slowly peel the tape to pull off the metal.</li>
	<li>To dissolve the polystyrene beads, place the bead templates in toluene and soak overnight.</li>
	<li>After the toluene incubation, rinse the templates once with chloroform and twice with ethanol. Dry the templates with N2 and remove residual polymer contaminants in an oxygen plasma cleaner for 30 min.</li>
	<li>Using thermal or electron beam evaporative deposition, deposit 100&#8722;150 nm of gold at 5 &#197;/s around and on top of the aluminum posts.</li>
	<li>To dissolve the metal posts, soak the coverslips in aluminum etchant (phosphoric acid-based; Table of Materials) for 1 h.</li>
	<li>Rinse the coverslips with distilled water, dry with N2, and gently buff the surface of the metal cladding with lens paper to expose any posts that are still covered in cladding. Place the coverslips back in aluminum etchant for 1 h, then rinse again with distilled water and dry with N2. 
	NOTE: ZMW slides should be stored in covered, clean Petri dishes.</li>
</ol>

The authors have nothing to disclose.

For the colloidal self-assembly (protocol section 2), the use of ethanol rather than water as the suspension solvent speeds the evaporation process so that templates are ready in 2&#8722;3 min after deposition rather than 1&#8722;2 h as in previous methods48,49. The evaporative sedimentation protocol presented here is also simpler than previous sedimentation protocols that require controlling surface tilt, temperature, and air volume above the suspension49,50,51. The particle volume fraction used in this protocol is 2.4%, higher than the 0.2&#8722;0.5% used in previous sedimentation methods48, which resuspended colloids in water-glycerol mixtures for much longer settling time-scales. However, the quality of the depositions is robust to changes in the particle volume fraction, with past studies finding that it can be varied between 2&#8722;10%49,50,51. The grain sizes of the colloidal crystals obtained in a successful deposition from this protocol are 20&#8722;30 &#181;m across, larger than grains from previous sedimentation methods (typically several hundred nanometers across)48,49. Macroscopically, the roughly 2 cm in diameter areas of colloidal monolayer are also comparable to the 1 cm areas produced by previous methods49. The large size of the colloidal crystal templates produced in this method also allows 3&#8722;5 separated flow chambers44, each about 3&#8722;4 mm wide, to be made on each ZMW slide. Thus, multiple independent single molecule experiments can be performed on each slide.
Annealing the colloidal bead templates (protocol section 3) after self-assembly is a simple, but crucial step for sufficiently reducing background fluorescence with the ZMWs. As Supplemental Figure 2 shows, the effective cutoff wavelength for a waveguide with the triangular cross-section from an unannealed template is 894 nm. In comparison, the effective cutoff wavelength for a 130 nm diameter circular waveguide from an annealed template is 221 nm, as determined both analytically (1.7 times the diameter of the guide18) and numerically. Using smaller beads for deposition could also reduce the size of the template pores, but the waveguides would then be spaced closer than 200 nm, which is around the diffraction limit of visible light. Furthermore, the waveguides would remain triangular in cross-section, which leads to nonsymmetric power propagation through the waveguide (Supplemental Figure 2A&#8722;D). One drawback of the annealing step is that variability in melting time can introduce fluctuations in waveguide diameter, so accurate timing helps to minimize variation between batches. The interstices start to close at annealing times longer than 25 s, and post diameters do not decrease very much between 20&#8722;25 s (Supplemental Figure 3B&#8722;D). A quick test for interstice closure is to check whether annealed templates still produce a rainbow diffraction pattern when illuminated with light and viewed at an angle. If not, the majority of interstices likely have closed. The relationship between annealing time and typical pore diameters has been presented earlier38.
After achieving the desired pore size during the annealing step, copper is deposited (step 4.1) onto the templates to create a shadow of the mask. It is important to use line of sight deposition, with the metal approaching the template as perpendicularly as possible. Thus, increasing the distance between the sample and metal source as well as ensuring the plate holding the templates is not spinning, as is automatically done in some vapor deposition machines, will aid in minimizing lateral deposition of metal onto the polystyrene substrate. However, some lateral deposition is inevitable, which reduces the size of the interstitial hole and thus the post cross-section as more metal is deposited52. This results in pyramidal metal posts rather than prism-like structures52.
Because the copper posts are likely pyramidal rather than prism shaped, aluminum deposition (step 4.5) on top of the posts also covers some of the sloped sides, blocking accessibility of the copper etchant for some of the posts. Thus, the lens paper buffing step (step 4.7 or 5.7) was added after the first soak in etchant to mechanically disrupt any copper posts still covered in aluminum. Depositing more copper to create taller posts also makes the posts more susceptible to mechanical disruption during the lens paper buffing. However, more than 500 nm of copper should not be deposited since the goal of deposition is to project the interstitial hole at the 500 nm midline of the 1 &#181;m beads.
Another potential difficulty is the unintended removal of aluminum cladding during the lens paper buffing (step 4.7 or 5.7). It was found that loss of aluminum cladding during buffing became more frequent after the annealing step was added, likely due to increased polystyrene residue, which can interfere with aluminum adherence to glass (protocol section 3). However, the overnight toluene soak (step 4.3 or 5.3) after the tape pull resolved this issue. In the AFM image in Figure 4E, some residual rings of polystyrene can be seen between the posts, but the aluminum cladding still resisted multiple buffs in step 4.7. If loss of the aluminum cladding remains an issue after the overnight toluene soak, an RCA-1 (standard clean-1) wash, piranha wash, or further oxygen plasma cleaning can be added to step 4.4 or 5.4. These wash steps can also be added after the final etch step (step 4.7 or 5.7) and before passivation in order to further clean the ZMWs.
The performance of the ZMWs in single molecule FRET experiments was similar to that of ZMWs fabricated with EBL. In a previous study53 performing single molecule FRET on Cy3 labeled single stranded DNA with Cy5 labeled DNA helicase loader protein in solution (the same donor-acceptor arrangement as that in Figure 6A), FRET events were clearly discernible at 100 nM Cy5 background, were less clear (lower acceptor trace signal to noise) at 1 &#181;M, and not discernible at 10 &#181;M. We note that a previous study with commercial ZMWs reported single molecule FRET acceptor signals at background concentrations as high as 1 mM54, higher than we and other previous studies42,53 with in-house fabricated ZMWs have achieved. Further discussion of the signal-to-background performance among ZMWs is given in Jamiolkowski et al.38. Nonspecific interaction of fluorescent sample with the ZMW surfaces53 is a common challenge limiting access to higher concentrations, especially if the diffusing fluorescent species in solution is a large macromolecule. Studies with ZMWs on complex biochemical systems such as translation have typically limited free fluorescent substrate concentrations to 100&#8722;250 nM55,56,57,58. Regardless of the intended application of the ZMWs, optimization of passivation methods for different systems will likely be necessary to maintain acceptable signal to noise at high concentrations.
Overall, the method presented here requires no specialized skills or equipment, allows parallel fabrication of many templates at once, and can be adapted to fabricate ZMWs in different metals. In this work, copper and aluminum were substituted with aluminum and gold, respectively, to fabricate gold ZMWs (Supplemental Figure 3). This is advantageous for labs that use passivation methods of gold rather than aluminum. In addition, gold ZMWs have been shown to enhance emission for fluorophores that absorb in the red region of the visible spectrum, while aluminum ZMWs enhance emission for fluorophores that absorb in the green region59. In the future, fluorescent signal intensity from ZMWs fabricated with this method might be enhanced by etching into the glass below the ZMW metal cladding using HF16,26,60. This brings the immobilized biomolecules farther away from the metal walls, which can quench fluorophores61. Furthermore, there is a maximum in excitation illumination intensity below the entrance of the aperture, and this has been exploited previously to enhance single molecule emission26,60.

An erratum was issued for:&#160;<a href="https://www-jove-com.remotexs.ntu.edu.sg/t/61154">Fabrication of Zero Mode Waveguides for High Concentration Single Molecule Microscopy</a>. A figure was updated.
Figure 3 was updated from:
<img alt="Figure 3" class="xfigimg" src="/files/ftp_upload/61154/61154fig3.jpg" /> 
Figure 3: Representative results from evaporative deposition of colloids. (A) Example of optimal colloid deposition. (B) Example of an acceptable colloid deposition in which conditions were more humid (80% RH) than ideal. Holes in the crystal monolayer are apparent. (C) Example of an acceptable colloid deposition in which conditions were drier (65% RH) than optimal. The monolayer regions are slightly translucent while multilayered areas are white and opaque (perimeter and streaks inward). (D) A colloidal crystal illuminated with white light to highlight the rainbow diffraction from the crystals. (E) AFM image (tapping probe AFM in air) of a monolayer of hexagonally packed polystyrene beads from a successful colloid deposition (scale bar = 10 &#181;m). (F) Expanded AFM image of packed beads (scale bar = 2 &#181;m). <a href="https://www-jove-com.remotexs.ntu.edu.sg/files/ftp_upload/61154/61154fig3large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
to:
<img alt="Figure 3" class="xfigimg" src="/files/ftp_upload/61154/61154fig3v2.jpg" /> 
Figure 3: Representative results from evaporative deposition of colloids. (A) Example of optimal colloid deposition. (B) Example of an acceptable colloid deposition in which conditions were more humid (80% RH) than ideal. Holes in the crystal monolayer are apparent. (C) Example of an acceptable colloid deposition in which conditions were drier (65% RH) than optimal. The monolayer regions are slightly translucent while multilayered areas are white and opaque (perimeter and streaks inward). (D) A colloidal crystal illuminated with white light to highlight the rainbow diffraction from the crystals. (E) AFM image (tapping probe AFM in air) of a monolayer of hexagonally packed polystyrene beads from a successful colloid deposition (scale bar = 10 &#181;m). (F) Expanded AFM image of packed beads (scale bar = 2 &#181;m). <a href="https://www-jove-com.remotexs.ntu.edu.sg/files/ftp_upload/61154/61154fig3v2large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>

An erratum was issued for:&#160;<a href="https://www-jove-com.remotexs.ntu.edu.sg/t/61154">Fabrication of Zero Mode Waveguides for High Concentration Single Molecule Microscopy</a>. A figure was updated.

Erratum: Fabrication of Zero Mode Waveguides for High Concentration Single Molecule Microscopy

Single-molecule techniques such as single molecule fluorescence resonance energy transfer (smFRET) or single molecule fluorescence correlation spectroscopy (FCS) are powerful tools for molecular biophysics, allowing the study of dynamic movements, conformations, and interactions of individual biomolecules in processes such as transcription1,2,3, translation4,5,6, and many others7. For smFRET, total internal reflection fluorescence (TIRF) microscopy is a common method because many tethered molecules may be followed over time, and the evanescent wave generated by TIR is limited to a 100&#8722;200 nm region adjacent to the coverslip8. However, even with this restriction on excitation volume, fluorophores of interest still need to be diluted to pM or nM ranges in order to detect single molecule signals above background fluorecence9. Since the Michaelis-Menten constants of cellular enzymes are typically in the &#956;M to mM range10, biochemical reactions in single molecule studies are usually much slower than those in the cell. For example, protein synthesis occurs at 15&#8722;20 &#160;amino acids per second in E. coli11,12, while most prokaryotic ribosomes in smFRET experiments translate at 0.1&#8722;1 amino acid per second13. In protein synthesis, crystal structures and smFRET on stalled ribosomes showed that transfer RNAs (tRNAs) fluctuate between &#8216;hybrid&#8217; and &#8216;classical&#8217; states before the tRNA-mRNA translocation step14,15. However, when physiological concentrations of the translocation GTPase factor, EF-G, was present, a different conformation, intermediate between the hybrid and classical states, was observed in smFRET6. Studying dynamic molecular processes at rates and concentrations similar to those in the cell is important, but remains a technical challenge.
A strategy to increase the fluorescent substrate concentration is the use of metal-based, sub-visible wavelength apertures, called zero mode waveguides (ZMWs), to generate confined excitation fields that selectively excite biomolecules localized within the apertures16 (Figure 1). The apertures are typically 100&#8722;200 nm in diameter and 100&#8722;150 nm in depth17. Above a cutoff wavelength related to the size and shape of the wells (&#955;c &#8776; 2.3 times the diameter for circular waveguides with water as the dielectric medium18), no propagating modes are allowed in the waveguide, hence the term zero mode waveguides. However, an oscillating electromagnetic field, termed an evanescent wave, exponentially decaying in intensity still tunnels a short distance into the waveguide18,19. Although similar to TIR evanescent waves, ZMW evanescent waves have a shorter decay constant, resulting in 10&#8722;30 nm effective excitation region within the waveguide. At micromolar concentrations of fluorescently labeled ligands, only one or a few molecules are simultaneously present within the excitation region. This restriction of the excitation volume and consequent reduction of background fluorescence enables fluorescence imaging of single molecules at biologically relevant concentrations. This has been applied to many systems20, including FCS measurements of single protein diffusion21, single molecule FRET measurements of low-affinity ligand-protein22 and protein-protein interactions23, and spectro-electrochemical measurements of single molecular turnover events24.
ZMWs have been produced by directly patterning a metal layer using ion beam milling25,26 or electron beam lithography (EBL) followed by plasma-etching16,27. These maskless lithography methods create waveguides in series and typically require access to specialized nanofabrication facilities, preventing widespread adoption of ZMW technology. Another method, ultraviolet nanoimprint lithography lift-off28, uses a quartz slide mold to press an inverse ZMW template onto a resist film like a stamp. While this method is more streamlined, it still requires EBL for fabrication of the quartz mold. This article presents the protocol for a simple and inexpensive templated fabrication method that does not require EBL or ion-beam milling and is based on close-packing of nanospheres to form a lithographic mask.
Nanosphere or &#8220;natural&#8221; lithography, which was first proposed in 1982 by Deckman and Dunsmuir29,30, uses the self-assembly of monodisperse colloidal particles, ranging from tens of nanometers to tens of micrometers31, to create templates for surface patterning via etching and/or deposition of materials. The two-dimensional (2D) or three-dimensional (3D) extended periodic arrays of colloidal particles, referred to as colloidal crystals, are characterized by a bright iridescence from scattering and diffraction32. Although less widely used than electron-beam or photolithography, this masking methodology is simple, low cost, and easily scaled down to create feature sizes below 100 nm.
Directing the self-assembly of colloidal particles determines the success of using colloidal crystals as masks for surface patterning. If the size and shape of particles are homogeneous, colloidal particles can be readily self-assembled with hexagonal packing, driven by entropic depletion33. Water evaporation after drop-coating is an effective route to sediment the colloidal particles, although other methods include dip-coating34, spin coating35, electrophoretic deposition36, and consolidation at an air-water interface37. The protocol presented below is based on the evaporation sedimentation method, which was the simplest to implement. The triangular interstices between close-packed polystyrene beads form openings in which to plate a sacrificial metal, forming posts (Figure 2 and Supplemental Figure 1). Brief annealing of the beads before this step adjusts the shape and diameter of these posts. The beads are removed, a final metal layer is deposited around the posts, and then the posts are removed. After the two metal deposition steps onto the colloidal nanomask, removal of the intermediate posts, and surface chemistry modification for passivation and tethering, ZMW arrays are ready to use for single molecule imaging. More extensive characterization of the ZMW optical properties after fabrication can found in an accompanying article38. Besides a thermal evaporator for vapor deposition of the metals, no specialized tools are required.

<table border="0" cellpadding="0" cellspacing="0" style="width:667px;" width="668">
	<colgroup>
		<col />
		<col />
		<col />
		<col />
	</colgroup>
	<tbody>
		<tr height="21">
			<td height="21" style="height:21px;width:215px;">1. Glass Coverslip Cleaning</td>
			<td style="width:103px;"></td>
			<td style="width:119px;"></td>
			<td style="width:231px;"></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:215px;">Acetone</td>
			<td style="width:103px;">Sigma</td>
			<td style="width:119px;">32201</td>
			<td>1 L</td>
		</tr>
		<tr height="42">
			<td height="42" style="height:42px;width:215px;">Coplin glass staining jar</td>
			<td style="width:103px;">Fisher Scientific</td>
			<td style="width:119px;">08-817</td>
			<td>Staining jar with 8 grooves and molded glass cover</td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:215px;">Coverslips</td>
			<td style="width:103px;">VWR</td>
			<td style="width:119px;">48404-467</td>
			<td>24 mm x 30 mm (No.1&#189;, Rectangular)</td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:215px;">Ethanol</td>
			<td style="width:103px;">Sigma</td>
			<td style="width:119px;">E7023</td>
			<td>1 L</td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:215px;">KOH</td>
			<td style="width:103px;">Sigma</td>
			<td style="width:119px;">30603</td>
			<td>Potassium hydroxide</td>
		</tr>
		<tr height="42">
			<td height="42" style="height:42px;width:215px;">Petri dishes</td>
			<td style="width:103px;">Fisher Scientific</td>
			<td style="width:119px;">R80115TS</td>
			<td>100 mm diameter, 15 mm deep</td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:215px;">Sonicator</td>
			<td style="width:103px;">Branson</td>
			<td style="width:119px;">Z245143</td>
			<td>Tabletop ultrasonic cleaner, 5510</td>
		</tr>
		<tr height="42">
			<td height="42" style="height:42px;width:215px;">2. Evaporative Deposition of Polystyrene Beads</td>
			<td style="width:103px;"></td>
			<td style="width:119px;"></td>
			<td></td>
		</tr>
		<tr height="42">
			<td height="42" style="height:42px;width:215px;">Clear storage container</td>
			<td style="width:103px;">Fisher Scientific</td>
			<td style="width:119px;">50-110-8222</td>
			<td>26 x 18 x 15 in.</td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:215px;">Desk fan</td>
			<td style="width:103px;">O2Cool</td>
			<td style="width:119px;">FD05001A</td>
			<td>Any small desk (~5 in.) fan will work</td>
		</tr>
		<tr height="42">
			<td height="42" style="height:42px;width:215px;">Glass beaker</td>
			<td style="width:103px;">Fisher Scientific</td>
			<td style="width:119px;">02-555-25B</td>
			<td>250 mL</td>
		</tr>
		<tr height="42">
			<td height="42" style="height:42px;width:215px;">Humidity meter</td>
			<td style="width:103px;">Fisher Scientific</td>
			<td style="width:119px;">11-661-19</td>
			<td></td>
		</tr>
		<tr height="42">
			<td height="42" style="height:42px;width:215px;">Microcentrifuge tubes</td>
			<td style="width:103px;">Fisher Scientific</td>
			<td style="width:119px;">21-402-903</td>
			<td>1.5 mL</td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:215px;">Polystyrene microspheres</td>
			<td style="width:103px;">Polysciences</td>
			<td style="width:119px;">18602-15</td>
			<td>1.00 &#181;m diameter, non-functionalized</td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:215px;">Triton X-100 deturgent</td>
			<td style="width:103px;">Sigma</td>
			<td style="width:119px;">X100</td>
			<td>100 mL</td>
		</tr>
		<tr height="63">
			<td height="63" style="height:63px;width:215px;">3. Bead Annealing for Reducing Pore Size in the Colloidal Crystal Template</td>
			<td style="width:103px;"></td>
			<td style="width:119px;"></td>
			<td></td>
		</tr>
		<tr height="42">
			<td height="42" style="height:42px;width:215px;">Aluminum plate</td>
			<td style="width:103px;">Fisher Scientific</td>
			<td style="width:119px;">AA11062RY</td>
			<td>Customized in-house to 14 cm x 14 cm</td>
		</tr>
		<tr height="42">
			<td height="42" style="height:42px;width:215px;">Ceramic hotplate</td>
			<td style="width:103px;">Fisher Scientific</td>
			<td style="width:119px;">HP88857100</td>
			<td>13 x 8.2 x 3.8 in.</td>
		</tr>
		<tr height="42">
			<td height="42" style="height:42px;width:215px;">Temperature controller</td>
			<td style="width:103px;">McMaster-Carr</td>
			<td style="width:119px;">38615K71</td>
			<td>Read temperature with thermocouple probe</td>
		</tr>
		<tr height="42">
			<td height="42" style="height:42px;width:215px;">Thermocouple probe</td>
			<td style="width:103px;">McMaster-Carr</td>
			<td style="width:119px;">9251T93</td>
			<td>Type K, surface probe</td>
		</tr>
		<tr height="63">
			<td height="63" style="height:63px;width:215px;">4/5. Nanofabrication of Zero Mode Waveguides Using the Colloidal Crystal Template</td>
			<td style="width:103px;"></td>
			<td style="width:119px;"></td>
			<td></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:215px;">Aluminum etchant</td>
			<td style="width:103px;">Transene</td>
			<td style="width:119px;">Type A</td>
			<td></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:215px;">Aluminum pellets</td>
			<td style="width:103px;">Kurt J. Lesker</td>
			<td style="width:119px;">EVMAL40QXHB</td>
			<td>For electron beam evaporation</td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:215px;">Chloroform</td>
			<td style="width:103px;">Sigma</td>
			<td style="width:119px;">288306</td>
			<td>1 L</td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:215px;">Copper etchant</td>
			<td style="width:103px;">Transene</td>
			<td style="width:119px;">49-1</td>
			<td></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:215px;">Copper pellets</td>
			<td style="width:103px;">Kurt J. Lesker</td>
			<td style="width:119px;">EVMCU40QXQA</td>
			<td>For electron beam evaporation</td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:215px;">Gold pellets</td>
			<td style="width:103px;">Kurt J. Lesker</td>
			<td style="width:119px;">EVMAUXX40G</td>
			<td>For electron beam evaporation</td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:215px;">Lens paper</td>
			<td style="width:103px;">Thorlabs</td>
			<td style="width:119px;">MC-5</td>
			<td></td>
		</tr>
		<tr height="42">
			<td height="42" style="height:42px;width:215px;">Plasma cleaner</td>
			<td style="width:103px;">Harrick Plasma</td>
			<td style="width:119px;">PDC-32G</td>
			<td></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:215px;">Scotch tape</td>
			<td style="width:103px;">Staples</td>
			<td style="width:119px;">MMM119</td>
			<td></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:215px;">Thin film deposition system</td>
			<td style="width:103px;">Kurt J. Lesker</td>
			<td style="width:119px;">PVD-75</td>
			<td>Tabletop thermal evaporation system will also work</td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:215px;">Titanium pellets</td>
			<td style="width:103px;">Kurt J. Lesker</td>
			<td style="width:119px;">EVMTI45QXQA</td>
			<td>For electron beam evaporation</td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:215px;">Toluene</td>
			<td style="width:103px;">Sigma</td>
			<td style="width:119px;">244511</td>
			<td>1 L</td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;width:215px;">Representative Results</td>
			<td style="width:103px;"></td>
			<td style="width:119px;"></td>
			<td></td>
		</tr>
		<tr height="21">
			<td height="21" style="height:21px;">COMSOL Multiphysics Modeling Software</td>
			<td>COMSOL, Inc.</td>
			<td style="width:119px;"></td>
			<td></td>
		</tr>
		<tr height="42">
			<td height="42" style="height:42px;width:215px;">Dual View spectral splitter</td>
			<td style="width:103px;">Photometrics, Inc.</td>
			<td style="width:119px;"></td>
			<td></td>
		</tr>
	</tbody>
</table>

fabrication of zero mode waveguides for high concentration single molecule microscopy

In single molecule fluorescence enzymology, background fluorescence from labeled substrates in solution often limits fluorophore concentration to pico- to nanomolar ranges, several orders of magnitude less than many physiological ligand concentrations. Optical nanostructures called zero mode waveguides (ZMWs), which are 100&#8722;200 nm in diameter apertures fabricated in a thin conducting metal such as aluminum or gold, allow imaging of individual molecules at micromolar concentrations of fluorophores by confining visible light excitation to zeptoliter effective volumes. However, the need for expensive and specialized nanofabrication equipment has precluded the widespread use of ZMWs. Typically, nanostructures such as ZMWs are obtained by direct writing using electron beam lithography, which is sequential and slow. Here, colloidal, or nanosphere, lithography is used as an alternative strategy to create nanometer-scale masks for waveguide fabrication. This report describes the approach in detail, with practical considerations for each phase. The method allows thousands of aluminum or gold ZMWs to be made in parallel, with final waveguide diameters and depths of 100&#8722;200 nm. Only common lab equipment and a thermal evaporator for metal deposition are required. By making ZMWs more accessible to the biochemical community, this method can facilitate the study of molecular processes at cellular concentrations and rates.

The self-assembly of the polystyrene colloidal particles via evaporative sedimentation (steps 2.1&#8722;2.13) can produce a range of results since it requires control of the solvent evaporation rate. However, because the depositions are fast (10&#8722;15 min per round), the procedure can be quickly optimized for different ambient lab conditions. Figure 3A shows a well-formed colloidal template after deposition and evaporation. Macroscopically, the region of beads is circular, with borders defined by an opaque, multilayered ring of beads. The translucent, but not white regions in the image are the desired monolayer areas. Figure 3B shows a colloidal template that was packed in an overly humid environment (80% RH when Petri dishes were closed). These templates tend not to have a clean circular boundary and have multilayered tendrils extending outward. The deposition is acceptable and can be used in subsequent phases, but the holes in the lattice reduce the number of useable ZMW array areas for single molecule imaging. Figure 3C shows a colloidal template that was packed in an overly dry environment (65% RH when Petri dishes were closed). These templates are usually smaller in diameter compared to the ideal, well spread templates. The deposition can be used, but the multilayered, white regions, which streak inward, reduce the area usable for imaging. Thus, we do not recommend performing more than 6 depositions at a time since depositions toward the end of the process will occur at a lower humidity as the chamber is opened and closed. Figure 3D shows the rainbow pattern produced by diffraction of reflected light from the polystyrene crystal. This pattern can be used to confirm success and quality of crystal packing by eye. Figure 3E,F shows atomic force microscopy (AFM) images of well-packed colloidal templates. The defects between grains arise from jamming during the evaporative sedimentation41, and distinct grains can be seen with a 10x objective. Thus, examining the colloid depositions with a low-power light microscope can also be used to assess packing.
After deposition of copper onto the annealed colloidal templates (step 4.1), the rainbow diffraction pattern should still be visible and enhanced by the reflective metal coating the tops of the beads (Figure 4A,B). The templates lose the reflective rainbow diffraction pattern after the Scotch tape pull (step 4.2) that removes excess copper (Figure 4C). Figure 4D,E shows AFM images of a typical field of copper posts after metal deposition. The defects in between the colloidal crystal grains in Figure 3E are visible in the copper post images as larger regions of copper. Analysis of AFM images shows that, for a copper deposition thickness of 300 nm, the eventual copper posts average 255 nm (Figure 4F) in height and 121 nm in diameter (Figure 4G).
Deposition of the aluminum cladding (step 4.5) where the beads were and on top of the copper posts, and subsequent dissolution of the posts (steps 4.6 and 4.7) result in the aluminum ZMWs shown in Figure 5A&#8722;C. Defects between the colloidal crystal grains are visible as larger openings (Figure 5B). The average distance between the ZMW centers in Figure 5C is 559 nm, consistent with the spacing set by the hexagonal close packing geometry of the 1 &#181;m beads (<img alt="Equation 1" src="/files/ftp_upload/61154/61154eq1.jpg" /> Using polystyrene templates that were annealed for 20 s results in waveguides that are on average 118 nm in diameter (Figure 5D,E), consistent with the post diameters and sufficiently small to cut off propagation of visible light. A height profile of a waveguide from Figure 5D also shows that it is ~120 nm deep.
Single molecule FRET was performed in the ZMWs to test for functionality (Figure 6A). A typical field of ZMWs for imaging is shown in Figure 6B, which contains &#62;3000 waveguides in a 40 x 80 &#181;m field of view. The ZMWs were first passivated using protocols described previously42,43. Briefly, the aluminum ZMWs were passivated with poly(vinylphosphonic acid) to coat the aluminum cladding followed by methoxy-terminated polyethylene glycol (PEG) doped with biotin-terminated PEG to coat the glass bottoms of the ZMWs. Gold ZMWs can be passivated with thiol-derivatized PEG to coat the gold cladding followed by a similar PEG treatment for the glass bottoms. Flow chambers, ~20 &#181;L volume, were then constructed for single molecule imaging44. Single molecule FRET imaging of the DNA duplexes was performed as described previously38. Briefly, 100 pM&#8722;1 nM of cyanine-3/cyanine-5 (Cy3/Cy5), biotinylated DNA duplexes (33 base pair length) were incubated for 10 min in flow channels functionalized with streptavidin (5 min incubation, 0.5 mg/mL solution). The concentration of labeled macromolecules can be titrated to achieve ~20% loading of the waveguides with one molecule, leading to &#60;5% waveguides loaded with more than one molecule, based on Poisson distributed loading (most waveguides, ~75%, will have no molecules)45. Unbound DNA was washed away with nuclease-free duplex buffer followed by illumination buffer (0.3% [w/v] glucose, 300 &#956;g/mL glucose oxidase, 120 &#956;g/mL catalase, and 1.5 mM Trolox [6-hydroxy-2,5,7,8-tetramethyl-chromane-2-carboxylic acid]). Non-biotinylated Cy5-labeled DNA duplexes (33 base pair length) were present in the illumination buffer at 0, 50, 100, and 500 nM as background fluorophores in solution. Single molecule FRET traces from the immobilized Cy3/Cy5 duplex DNA molecules were recorded with a custom-built TIRF microscope adjusted to epi-fluorescence conditions. Movies were recorded with a 1.48 numerical aperture (NA) 100x oil immersion objective with alternating 532 nm and 640 nm excitation (100 ms exposure) and a dual view spectral splitter to record Cy3 and Cy5 emission simultaneously on an electron-multiplying charge-coupled device (EMCCD) camera. Single molecule FRET traces with single step bleaches in the Cy5 channel were detectable at all concentrations of ambient Cy5 tested (Figure 6C&#8722;F). In comparison, single molecules would only be detectable in TIRF illumination with pM to low nM solution fluorophore concentrations46.
<img alt="Figure 1" class="xfigimg" src="/files/ftp_upload/61154/61154fig1.jpg" /> 
Figure 1: Schematic of zero mode waveguides. Diagram of ZMW array with expanded cross-sectional diagram of a single ZMW on the right. Single fluorescently tagged enzymes of interest (brown ribosome with red circle to represent fluorescent dye) chemically immobilized (via the mRNA in this example) to the glass bottom of the ZMWs (typically functionalized with biotinylated-PEG) can be imaged with a typical laser-based epifluorescence microscopy setup. The 532 nm excitation light (green arrows) is reflected at the glass-metal boundary due to the small size of the aperture (100&#8722;200 nm diameter), but a non-propagating evanescent wave that decays exponentially in intensity is present within the ZMW. This results in a 10&#8722;30 nm effective illumination depth (green shading in aperture). Individual fluorescent ligands (blue tRNAs with green circles as fluorescent tags) at nM to &#181;M concentrations are added. An individual ligand that diffuses into the aperture and interacts with the enzyme is imaged without prohibitive background fluorescence. <a href="https://www-jove-com.remotexs.ntu.edu.sg/files/ftp_upload/61154/61154fig1large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 2" class="xfigimg" src="/files/ftp_upload/61154/61154fig2.jpg" /> 
Figure 2: Schematic of colloidal templating method developed to fabricate aluminum ZMW arrays. Polystyrene beads, 1 &#181;m in diameter, are deposited and self-assembled on a cleaned glass coverslip, as described in section 2 of the protocol. Beads are then annealed to reduce pore sizes (section 3), followed by copper deposition and bead dissolution in toluene. Aluminum is deposited around and on top of the copper posts, which are then selectively etched away to leave behind a hexagonal array of nanoapertures (section 4). For the last three steps, cross-sectional views are provided to the right of the plan views to show the widths and heights of the copper posts and aluminum ZMWs. <a href="https://www-jove-com.remotexs.ntu.edu.sg/files/ftp_upload/61154/61154fig2large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 3" class="xfigimg" src="/files/ftp_upload/61154/61154fig3v2.jpg" /> 
Figure 3: Representative results from evaporative deposition of colloids. (A) Example of optimal colloid deposition. (B) Example of an acceptable colloid deposition in which conditions were more humid (80% RH) than ideal. Holes in the crystal monolayer are apparent. (C) Example of an acceptable colloid deposition in which conditions were drier (65% RH) than optimal. The monolayer regions are slightly translucent while multilayered areas are white and opaque (perimeter and streaks inward). (D) A colloidal crystal illuminated with white light to highlight the rainbow diffraction from the crystals. (E) AFM image (tapping probe AFM in air) of a monolayer of hexagonally packed polystyrene beads from a successful colloid deposition (scale bar = 10 &#181;m). (F) Expanded AFM image of packed beads (scale bar = 2 &#181;m). <a href="https://www-jove-com.remotexs.ntu.edu.sg/files/ftp_upload/61154/61154fig3v2large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 4" class="xfigimg" src="/files/ftp_upload/61154/61154fig4.jpg" /> 
Figure 4: Macroscopic and microscopic images of ZMW templates after copper deposition. (A) Picture of slides after physical evaporation of copper on top of the bead templates. (B) Rainbow diffraction pattern from bead templates after copper deposition. (C) Picture of a template (right) after a tape pull to remove excess copper and the tape (left). (D) AFM image of copper posts after tape pull and complete dissolution of the polystyrene beads (scale bar = 5 &#181;m). (E) Higher magnification AFM image of panel D (scale bar = 2 &#181;m). (F) Histogram of the copper post heights (defined as maximum height measurement within each post), n = 534. (G) Histogram of the copper post Feret diameters, n = 201. Feret diameter is the maximum distance between two parallel lines tangent to the post boundary (quantified in ImageJ47). To identify particles for analysis, a threshold halfway between the top of the cladding and the bottom glass surface was used. <a href="https://www-jove-com.remotexs.ntu.edu.sg/files/ftp_upload/61154/61154fig4large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 5" class="xfigimg" src="/files/ftp_upload/61154/61154fig5.jpg" /> 
Figure 5: Macroscopic and microscopic images of aluminum ZMWs. (A) Picture of slides after physical evaporative deposition of 150 nm of aluminum around and on top of the copper posts. (B) AFM image of aluminum ZMWs after post dissolution (scale bar = 5 &#181;m). (C) Higher magnification image of panel B (scale bar = 0.2 &#181;m). (D) Typical depth profile of an individual ZMW from panel C. Profile taken from the green line drawn in panel C. (E) Histogram of ZMW Feret diameters, n = 240. Feret diameters were measured as in Figure 4. <a href="https://www-jove-com.remotexs.ntu.edu.sg/files/ftp_upload/61154/61154fig5large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
<img alt="Figure 6" class="xfigimg" src="/files/ftp_upload/61154/61154fig6.jpg" /> 
Figure 6: Single molecule FRET imaging in ZMWs. (A) Schematic (not to scale) of single molecule FRET imaging of Cy3, Cy5-labeled DNA duplexes in ZMWs with Cy5 labeled duplexes in the background. (B) Example field of ZMWs under white light illumination (scale bar = 10 &#181;m). (C&#8722;F) Single molecule FRET recordings of DNA duplexes immobilized in the ZMWs in the presence of 0 (C), 50 (D), 100 (E), and 500 nM (F) Cy5-labeled duplexes in solution. For each concentration, the top panel shows the Cy3 (green) and Cy5 (red) fluorescence intensity under 532 nm laser illumination (FRET imaging), middle panel shows the Cy5 fluorescence intensity under 640 nm laser illumination (direct acceptor excitation), and the lowest panel shows the FRET efficiency (<img alt="Equation 2" src="/files/ftp_upload/61154/61154eq2.jpg" /> ) calculated from the raw Cy3 (ID) and Cy5 (IA) fluorescence intensities. During imaging, the excitation wavelength alternated between 532 and 640 nm every 100 ms. <a href="https://www-jove-com.remotexs.ntu.edu.sg/files/ftp_upload/61154/61154fig6large.jpg" target="_blank">Please click here to view a larger version of this figure.</a>
Supplemental Figure 1: Schematic of colloidal templating method developed to fabricate gold ZMW array. Protocol to fabricate gold ZMW array is analogous to protocol to fabricate aluminum ZMW array (Figure 2). Instead of depositing copper on top of the polystyrene beads, aluminum is deposited. After dissolving the beads in toluene, gold is deposited instead of aluminum on top of the posts. Aluminum posts are then selectively etched to leave behind gold ZMW array. For the last three steps, cross-sectional views are provided to the right of the plan views to show the widths and heights of the aluminum posts and gold ZMWs. <a href="https://www-jove-com.remotexs.ntu.edu.sg/files/ftp_upload/61154/61154supfig1large.jpg" target="_blank">Please click here to download this file.</a>
Supplemental Figure 2: Finite element modeling of electromagnetic field propagation in ZMWs. (A&#8722;D) Cross sections of the magnitude of the time-averaged Poynting vector (W/m2) through a waveguide made from an unannealed template (A,C) and an annealed template (B,D). Linearly polarized electromagnetic plane waves (1 W distributed over the area of the slide) at the wavelengths listed in the figure (400 nm or 1,000 nm) were projected onto the bottom surface, and the lowest (fundamental) mode, which has the lowest wavenumber, was computed using modeling software (Table of Materials) with the finite element method for solving Maxwell&#8217;s equations and appropriate boundary conditions. The boundaries of the waveguides were assumed to be perfect electrical conductors, which is well approximated by aluminum or gold walls. The cross-section from the unannealed waveguide template was determined by the hexagonal packing of 1 &#956;m diameter circles, and the three-pointed tips from the resulting triangular shape were clipped to ~60 nm width to model a realistic physical aperture. The cross-section from the annealed templates was approximated as a circle 130 nm in diameter. Both waveguides had a 130 nm depth, similar to the cladding depth after fabrication. (E,F) In addition to excitation wavelengths of 400 nm and 1,000 nm, the models were solved at 100 excitation wavelengths evenly spaced between 400 nm and 1,000 nm, and the effective mode index (defined as <img alt="Equation 3" src="/files/ftp_upload/61154/61154eq3.jpg" />, where kz is the wavenumber in the waveguide, which is decreased due to restriction in the transverse plane, and k is the excitation light wavenumber in vacuum) was plotted against excitation wavelength for the triangular (E) and circular (F) waveguides. For shorter wavelengths, higher modes are excited, and the effective mode index increases (max effective mode index is 1, which is the limiting case where the electromagnetic plane wave travels unbounded in the transverse dimension). The effective cutoff wavelengths of the waveguides were estimated as the wavelength at which the effective mode index drops to 0. Note that the circular guide &#955;cutoff = 221 nm from finite element modelling (F) is consistent with the theoretical prediction of a circular waveguide&#8217;s cutoff wavelength (&#955;cutoff,analytical = 1.7d = 221 nm, where d is the waveguide diameter). <a href="https://www-jove-com.remotexs.ntu.edu.sg/files/ftp_upload/61154/61154supfig2large.jpg" target="_blank">Please click here to download this file.</a>
Supplemental Figure 3: Representative results from Au ZMW fabrication. (A) Macroscopic picture of gold ZMW arrays. (B&#8722;D) AFM images of aluminum posts from a bead template that was not annealed (B), a template that was annealed at 107 &#176;C for 20 s (C), and a template that was annealed at 107 &#176;C for 25 s (D). (E) AFM image of gold ZMWs after dissolution of aluminum posts. (F) Higher magnification AFM image of panel E. (G) Typical depth profile of a gold ZMW. Profile taken from the green line drawn in panel F (scale bar = 1 &#181;m in B, C, D, and F; 5 &#181;m in E). <a href="https://www-jove-com.remotexs.ntu.edu.sg/files/ftp_upload/61154/61154supfig3large.jpg" target="_blank">Please click here to download this file.</a>

Watch this Scientific Journal Video about Fabrication of Zero Mode Waveguides for High Concentration Single Molecule Microscopy at JoVE.com

Fabrication of Zero Mode Waveguides for High Concentration Single Molecule Microscopy

Described here is a nanosphere lithography method for parallel fabrication of zero mode waveguides, which are arrays of nanoapertures in a metal-clad glass microscopy coverslip for single molecule imaging at nano- to micromolar concentrations of fluorophores. The method takes advantage of colloidal crystal self-assembly to create a waveguide template.

In single molecule fluorescence enzymology, background fluorescence from labeled substrates in solution often limits fluorophore concentration to pico- to ...

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7.9K Views.  University of Pennsylvania. Described here is a nanosphere lithography method for parallel fabrication of zero mode waveguides, which are arrays of nanoapertures in a metal-clad glass microscopy coverslip for single molecule imaging at nano- to micromolar concentrations of fluorophores. The method takes advantage of colloidal crystal self-assembly to create a waveguide template.

Video: Fabrication of Zero Mode Waveguides for High Concentration Single Molecule Microscopy

Low-Cost Cryo-Light Microscopy Stage Fabrication for Correlated Light/Electron Microscopy

The coupling of cryo-light microscopy (cryo-LM) and cryo-electron microscopy (cryo-EM) poses a number of advantages for understanding cellular 
dynamics and ultrastructure. First, cells can be imaged in a near native environment for both techniques. Second, due to the vitrification process, samples are
 preserved by rapid physical immobilization rather than slow chemical fixation. Third, imaging the same sample with both cryo-LM and cryo-EM provides correlation of
 data from a single cell, rather than a comparison of "representative samples". While these benefits are well known from prior studies, the widespread use of correlative 
 cryo-LM and cryo-EM remains limited due to the expense and complexity of buying or building a suitable cryogenic light microscopy stage. Here we demonstrate the 
 assembly, and use of an inexpensive cryogenic stage that can be fabricated in any lab for less than $40 with parts found at local hardware and grocery stores. This 
 cryo-LM stage is designed for use with reflected light microscopes that are fitted with long working distance air objectives. For correlative cryo-LM and cryo-EM 
 studies, we adapt the use of carbon coated standard 3-mm cryo-EM grids as specimen supports. After adsorbing the sample to the grid, previously established protocols 
 for vitrifying the sample and transferring/handling the grid are followed to permit multi-technique imaging. As a result, this setup allows any laboratory with a 
 reflected light microscope to have access to direct correlative imaging of frozen hydrated samples.

We demonstrate the fabrication of a low-cost cryogenic stage designed to fit most reflected light microscopes. This lab-built cryogenic stage enables efficient and reliable correlative imaging between cryo-light and cryo-electron microscopy.

The coupling of cryo-light microscopy (cryo-LM) and cryo-electron microscopy (cryo-EM) poses a number of advantages for understanding cellular 
dynamics ...

Multiplexed Single-molecule Force Proteolysis Measurements Using Magnetic Tweezers

The generation and detection of mechanical forces is a ubiquitous aspect of cell physiology, with direct relevance to cancer metastasis1, atherogenesis2 and wound healing3. In each of these examples, cells both exert force on their surroundings and simultaneously enzymatically remodel the extracellular matrix (ECM). The effect of forces on ECM has thus become an area of considerable interest due to its likely biological and medical importance4-7.
	Single molecule techniques such as optical trapping8, atomic force microscopy9, and magnetic tweezers10,11 allow researchers to probe the function of enzymes at a molecular level by exerting forces on individual proteins. Of these techniques, magnetic tweezers (MT) are notable for their low cost and high throughput. MT exert forces in the range of ~1-100 pN and can provide millisecond temporal resolution, qualities that are well matched to the study of enzyme mechanism at the single-molecule level12. Here we report a highly parallelizable MT assay to study the effect of force on the proteolysis of single protein molecules. We present the specific example of the proteolysis of a trimeric collagen peptide by matrix metalloproteinase 1 (MMP-1); however, this assay can be easily adapted to study other substrates and proteases.

In this article we describe the use of magnetic tweezers to study the effect of force on enzymatic proteolysis at the single molecule level in a highly parallelizable manner.

The  generation and detection of mechanical forces is a ubiquitous aspect of cell physiology,  with direct relevance to cancer metastasis1, atherogenesis2 ...

Fabrication of Carbon Nanotube High-Frequency Nanoelectronic Biosensor for Sensing in High Ionic Strength Solutions

The unique electronic properties and high surface-to-volume ratios of single-walled carbon nanotubes (SWNT) and semiconductor nanowires (NW) 1-4 make them good candidates for high sensitivity biosensors. When a charged molecule binds to such a sensor surface, it alters the carrier density5 in the sensor, resulting in changes in its DC conductance. However, in an ionic solution a charged surface also attracts counter-ions from the solution, forming an electrical double layer (EDL). This EDL effectively screens off the charge, and in physiologically relevant conditions ~100 millimolar (mM), the characteristic charge screening length (Debye length) is less than a nanometer (nm). Thus, in high ionic strength solutions, charge based (DC) detection is fundamentally impeded6-8.
We overcome charge screening effects by detecting molecular dipoles rather than charges at high frequency, by operating carbon nanotube field effect transistors as high frequency mixers9-11. At high frequencies, the AC drive force can no longer overcome the solution drag and the ions in solution do not have sufficient time to form the EDL. Further, frequency mixing technique allows us to operate at frequencies high enough to overcome ionic screening, and yet detect the sensing signals at lower frequencies11-12. Also, the high transconductance of SWNT transistors provides an internal gain for the sensing signal, which obviates the need for external signal amplifier.
Here, we describe the protocol to (a) fabricate SWNT transistors, (b) functionalize biomolecules to the nanotube13, (c) design and stamp a poly-dimethylsiloxane (PDMS) micro-fluidic chamber14 onto the device, and (d) carry out high frequency sensing in different ionic strength solutions11.

We describe the device fabrication and measurement protocol for carbon nanotube based high frequency biosensors. The high frequency sensing technique mitigates the fundamental ionic (Debye) screening effect and allows nanotube biosensor to be operated in high ionic strength solutions where conventional electronic biosensors fail. Our technology provides a unique platform for point-of-care (POC) electronic biosensors operating in physiologically relevant conditions.

The unique electronic properties and high surface-to-volume ratios of single-walled carbon nanotubes (SWNT) and semiconductor nanowires (NW) 1-4 make them ...

Microfluidic Picoliter Bioreactor for Microbial Single-cell Analysis: Fabrication, System Setup, and Operation

In this protocol the fabrication, experimental setup and basic operation of the recently introduced microfluidic picoliter bioreactor (PLBR) is described in detail. The PLBR can be utilized for the analysis of single bacteria and microcolonies to investigate biotechnological and microbiological related questions concerning, e.g.&#160;cell growth, morphology, stress response, and metabolite or protein production on single-cell level. The device features continuous media flow enabling constant environmental conditions for perturbation studies, but in addition allows fast medium changes as well as oscillating conditions to mimic any desired environmental situation. To fabricate the single use devices, a silicon wafer containing sub micrometer sized SU-8 structures served as the replication mold for rapid polydimethylsiloxane casting. Chips were cut, assembled, connected, and set up onto a high resolution and fully automated microscope suited for time-lapse imaging, a powerful tool for spatio-temporal cell analysis. Here, the biotechnological platform organism Corynebacterium glutamicum&#160;was seeded into the PLBR and cell growth and intracellular fluorescence were followed over several hours unraveling time dependent population heterogeneity on single-cell level, not possible with conventional analysis methods such as flow cytometry. Besides insights into device fabrication, furthermore, the preparation of the preculture, loading, trapping of bacteria, and the PLBR cultivation of single cells and colonies is demonstrated. These devices will add a new dimension in microbiological research to analyze time dependent phenomena of single bacteria under tight environmental control. Due to the simple and relatively short fabrication process the technology can be easily adapted at any microfluidics lab and simply tailored towards specific needs.

In this protocol the fabrication, setup and basic operation of a microfluidic picoliter bioreactor (PLBR) for single-cell analysis of prokaryotic microorganisms is introduced. Industrially relevant microorganisms were analyzed as proof of principle allowing insights into growth rate, morphology, and phenotypic heterogeneity over certain time periods, hardly possible with conventional methods.

In this protocol the fabrication, experimental setup and basic operation of the recently introduced microfluidic picoliter bioreactor (PLBR) is described ...

Investigating Receptor-ligand Systems of the Cellulosome with AFM-based Single-molecule Force Spectroscopy

Cellulosomes are discrete multienzyme complexes used by a subset of anaerobic bacteria and fungi to digest lignocellulosic substrates. Assembly of the enzymes onto the noncatalytic scaffold protein is directed by interactions among a family of related receptor-ligand pairs comprising interacting cohesin and dockerin modules. The extremely strong binding between cohesin and dockerin modules results in dissociation constants in the low picomolar to nanomolar range, which may hamper accurate off-rate measurements with conventional bulk methods. Single-molecule force spectroscopy (SMFS) with the atomic force microscope measures the response of individual biomolecules to force, and in contrast to other single-molecule manipulation methods (i.e.&#160;optical tweezers), is optimal for studying high-affinity receptor-ligand interactions because of its ability to probe the high-force regime (&#62;120 pN). Here we present our complete protocol for studying cellulosomal protein assemblies at the single-molecule level. Using a protein topology derived from the native cellulosome, we worked with enzyme-dockerin and carbohydrate binding module-cohesin (CBM-cohesin) fusion proteins, each with an accessible free thiol group at an engineered cysteine residue. We present our site-specific surface immobilization protocol, along with our measurement and data analysis procedure for obtaining detailed binding parameters for the high-affinity complex. We demonstrate how to quantify single subdomain unfolding forces, complex rupture forces, kinetic off-rates, and potential widths of the binding well. The successful application of these methods in characterizing the cohesin-dockerin interaction responsible for assembly of multidomain cellulolytic complexes is further described.

Cellulosomes are multienzyme complexes designed for digesting cellulose. AFM-based SMFS was used to study the mechanical properties and folding configuration of cellulosome-associated protein assemblies. We present a complete workflow for protein immobilization, data acquisition, and data analysis to study the interactions of individual receptor-ligand complexes involved in cellulosome assembly.

Cellulosomes are discrete multienzyme complexes used by a subset of anaerobic bacteria and fungi to digest lignocellulosic substrates. Assembly of the ...

High-resolution Spatiotemporal Analysis of Receptor Dynamics by Single-molecule Fluorescence Microscopy

Single-molecule microscopy is emerging as a powerful approach to analyze the behavior of signaling molecules, in particular concerning those aspect (e.g., kinetics, coexistence of different states and populations, transient interactions), which are typically hidden in ensemble measurements, such as those obtained with standard biochemical or microscopy methods. Thus, dynamic events, such as receptor-receptor interactions, can be followed in real time in a living cell with high spatiotemporal resolution. This protocol describes a method based on labeling with small and bright organic fluorophores and total internal reflection fluorescence (TIRF) microscopy to directly visualize single receptors on the surface of living cells. This approach allows one to precisely localize receptors, measure the size of receptor complexes, and capture dynamic events such as transient receptor-receptor interactions. The protocol provides a detailed description of how to perform a single-molecule experiment, including sample preparation, image acquisition and image analysis. As an example, the application of this method to analyze two G-protein-coupled receptors, i.e., &#946;2-adrenergic and &#947;-aminobutyric acid type B (GABAB) receptor, is reported. The protocol can be adapted to other membrane proteins and different cell models, transfection methods and labeling strategies.

This protocol describes how to use total internal reflection fluorescence microscopy to visualize and track single receptors on the surface of living cells and thereby analyze receptor lateral mobility, size of receptor complexes as well as to visualize transient receptor-receptor interactions. This protocol can be extended to other membrane proteins.

Single-molecule microscopy is emerging as a powerful approach to analyze the behavior of signaling molecules, in particular concerning those aspect (e.g., ...

Ordering Single Cells and Single Embryos in 3D Confinement: A New Device for High Content Screening

Biological cells are usually observed on flat (2D) surfaces. This condition is not physiological, and phenotypes and shapes are highly variable. Screening based on cells in such environments have therefore serious limitations: cell organelles show extreme phenotypes, cell morphologies and sizes are heterogeneous and/or specific cell organelles cannot be properly visualized. In addition, cells in vivo are located in a 3D environment; in this situation, cells show different phenotypes mainly because of their interaction with the surrounding extracellular matrix of the tissue. In order to standardize and generate order of single cells in a physiologically-relevant 3D environment for cell-based assays, we report here the microfabrication and applications of a device for in vitro 3D cell culture. This device consists of a 2D array of microcavities (typically 105 cavities/cm2), each filled with single cells or embryos. Cell position, shape, polarity and internal cell organization become then normalized showing a 3D architecture. We used replica molding to pattern an array of microcavities, &#8216;eggcups&#8217;, onto a thin polydimethylsiloxane (PDMS) layer adhered on a coverslip. Cavities were covered with fibronectin to facilitate adhesion. Cells were inserted by centrifugation. Filling percentage was optimized for each system allowing up to 80%. Cells and embryos viability was confirmed. We applied this methodology for the visualization of cellular organelles, such as nucleus and Golgi apparatus, and to study active processes, such as the closure of the cytokinetic ring during cell mitosis. This device allowed the identification of new features, such as periodic accumulations and inhomogeneities of myosin and actin during the cytokinetic ring closure and compacted phenotypes for Golgi and nucleus alignment. We characterized the method for mammalian cells, fission yeast, budding yeast, C. elegans with specific adaptation in each case. Finally, the characteristics of this device make it particularly interesting for drug screening assays and personalized medicine.

We report a device and a new method to study cells and embryos. Single cells are precisely ordered in microcavity arrays. Their 3D confinement is a step towards 3D environments encountered in physiological conditions and allows organelle orientation. By controlling cell shape, this setup minimizes variability reported in standard assays.

Biological cells are usually observed on flat (2D) surfaces. This condition is not physiological, and phenotypes and shapes are highly variable. Screening ...

Preparation of Mica Supported Lipid Bilayers for High Resolution Optical Microscopy Imaging

Supported lipid bilayers (SLBs) are widely used as a model for studying membrane properties (phase separation, clustering, dynamics) and its interaction with other compounds, such as drugs or peptides. However SLB characteristics differ depending on the support used. 
Commonly used techniques for SLB imaging and measurements are single molecule fluorescence microscopy, FCS and atomic force microscopy (AFM). Because most optical imaging studies are carried out on a glass support, while AFM requires an extremely flat surface (generally mica), results from these techniques cannot be compared directly, since the charge and smoothness properties of these materials strongly influence diffusion. Unfortunately, the high level of manual dexterity required for the cutting and gluing thin slices of mica to the glass slide presents a hurdle to routine use of mica for SLB preparation. Although this would be the method of choice, such prepared mica surfaces often end up being uneven (wavy) and difficult to image, especially with small working distance, high numerical aperture lenses. Here we present a simple and reproducible method for preparing thin, flat mica surfaces for lipid vesicle deposition and SLB preparation. Additionally, our custom made chamber requires only very small volumes of vesicles for SLB formation. The overall procedure results in the efficient, simple and inexpensive production of high quality lipid bilayer surfaces that are directly comparable to those used in AFM studies.

We present a method of preparing mica supported lipid bilayers for high resolution microscopy. Mica is transparent and flat on an atomic scale, but rarely used in imaging because of handling difficulties; our preparation results in even deposition of the mica sheet, and reduces the material used in bilayer preparation.

Supported lipid bilayers (SLBs) are widely used as a model for studying membrane properties (phase separation, clustering, dynamics) and its interaction ...

Single Molecule Fluorescence Microscopy on Planar Supported Bilayers

In the course of a single decade single molecule microscopy has changed from being a secluded domain shared merely by physicists with a strong background in optics and laser physics to a discipline that is now enjoying vivid attention by life-scientists of all venues 1. This is because single molecule imaging has the unique potential to reveal protein behavior in situ in living cells and uncover cellular organization with unprecedented resolution below the diffraction limit of visible light 2. Glass-supported planar lipid bilayers (SLBs) are a powerful tool to bring cells otherwise growing in suspension in close enough proximity to the glass slide so that they can be readily imaged in noise-reduced Total Internal Reflection illumination mode 3,4. They are very useful to study the protein dynamics in plasma membrane-associated events as diverse as cell-cell contact formation, endocytosis, exocytosis and immune recognition. Simple procedures are presented how to generate highly mobile protein-functionalized SLBs in a reproducible manner, how to determine protein mobility within and how to measure protein densities with the use of single molecule detection. It is shown how to construct a cost-efficient single molecule microscopy system with TIRF illumination capabilities and how to operate it in the experiment.

Preparation of protein-functionalized planar glass-supported lipid bilayers, determination of protein mobility within and measurement of protein densities is shown here. A roadmap to building a noise-reduced Total Internal Reflection microscope is outlined, which allows visualizing single bilayer-resident fluorochromes with high spatiotemporal resolution.

In the course of a single decade single molecule microscopy has changed from being a secluded domain shared merely by physicists with a strong background ...

Label-free Single Molecule Detection Using Microtoroid Optical Resonators

Detecting small concentrations of molecules down to the single molecule limit has impact on areas such as early detection of disease, and fundamental studies on the behavior of molecules. Single molecule detection techniques commonly utilize labels such as fluorescent tags or quantum dots, however, labels are not always available, increase cost and complexity, and can perturb the events being studied. Optical resonators have emerged as a promising means to detect single molecules without the use of labels. Currently the smallest particle detected by a non-plasmonically-enhanced bare optical resonator system in solution is a 25 nm polystyrene sphere1. We have developed a technique known as Frequency Locking Optical Whispering Evanescent Resonator (FLOWER) that can surpass this limit and achieve label-free single molecule detection in aqueous solution2. As signal strength scales with particle volume, our work represents a &#62; 100x improvement in the signal to noise ratio (SNR) over the current state of the art. Here the procedures behind FLOWER are presented in an effort to increase its usage in the field.

We have developed a label-free biosensing system based on optical resonator technology known as Frequency Locking Optical Whispering Evanescent Resonator (FLOWER) that is capable of detecting single molecules in solution. Here the procedures behind this work are described and presented.

Detecting small concentrations of molecules down to the single molecule limit has impact on areas such as early detection of disease, and fundamental ...