TITLE: SiMOA total Rab10 Homebrew Assay
AUTHORS: yuan.yuan, andrew.west

[DESCRIPTION]
Assay for the detection of total Rab10 protein (rodent or human) in biofluids or lysates.

[STEPS]
2. Prepare the Beads
3. Conjugate
SECTION: Prepare Capture Beads Concentrate (5-6 hours)
1. Prepare capture beads using a two-step EDC coupling protocol. Reaction occurs between the antibody primary amino groups (-NH2) and the carboxyl groups (-COOH) on the beads. 80ug of antibody is required for 0.2 mg/ml buffer exchanged antibody, producing 4.2 x 10^8 beads, sufficient for 500 tests at 5 x 10^5 beads/test.

 
Capture antibody for Homebrew Total Rab10 Assay is 
  

 
SECTION: Prepare Detector Antibodies (4 hours)
4. This protocol describes how to prepare biotinylated detector antibodies (IgG). The NHS‐PEG4‐biotin used in this protocol is an amine‐reactive ester that couples to primary amine groups (-NH2) of proteins. The hydrophilic polyethylene glycol (PEG) spacer improves water solubility. Other reactive groups (carboxyl, –SH) and spacers can be tried, but some optimization will be needed. This guide specifies preparing and testing an initial lot of detector with 1 mg/mL of antibody and a 40:1 ratio of biotin to antibody. Each biotinylation reaction requires 130 μg of antibody and will produce approximately 50 to 80 μg of detector.

Detector antibody for Homebrew Total Rab10 Assay is 
  

 
SECTION: Perform Simoa Assay (5 hours)
5. 
 
SECTION: Optimize Assay Conditions
6. Review Results

6.1 Export run report and data to an external flash drive. 
Select "Report" on home page of SR-X.
Select the run need to be generated a report from the drop box, then click on "Generate report"
View the report.
Export report (PDF or Excel) to an external hard drive.
 
Select "Data" on home page of SR-X.
Select the run need to be generated a run data.
Select "data table" on the top left corner. 
Select "Export data".
Select "Export all columns"
Export run data (csv) and to an external hard drive.
 
6.2 Evaluate LOD, LLOQ, and Signal‐to‐Background Ratio 
Open "Run report" excel file.
Check AEBs for standards.
Limit of Detection (LOD) is the lowest amount of analyte in a sample that can be detected with acceptable statistical certainty but not quantitated as an exact value. Quanterix calculates LOD at 2.5 x STD above Cal A Average AEB, and typical Quanterix kits use 4PL curve fitting with 1/y2 weighting. 
LLOQ is the lower limit of quantitation, calculated as the lowest concentration at which the CV’s are less than 20%.
The signal-to-background ratio between Calibrator A (background) and Calibrator B should be between 2.5–3. 

6.3 Ideal assay characteristics
Open "Run data" csv file.
Check "fon" column.
There should be a low background, less than 0.02 AEB (fon <~ 0.02). The ideal level is 0.005–0.01 AEB (fon ~ 0.005–0.01)
High signal-to-background ratio (robust dose-response slope) with an upper range of target signal on the order of ~16 AEB. Levels above 20 AEB should be avoided. Above this, the optics will begin to exhibit saturation at the current setting of exposure time. Signal saturation
will manifest as a reduction in the expected dose-response of the calibrator level(s) exhibiting saturation.
Approximately 4 logs of signal range are typical for a Simoa assay (0.005–16 AEB). A low slope indicates a larger dynamic range (+) but greater dose read-back imprecision at a given signal (-). A higher slope indicates a smaller assay range due to the camera ceiling (-)
but minimizes dose imprecision at a given signal (+).

6.4 For low-abundance analytes, it is more important to maximize sensitivity. The objective is to maximize signal-to-background ratios with the highest possible calibration curve slope and the lowest possible background.



SECTION: Prepare Capture Beads Concentrate (5-6 hours)
1.1. Prepare the Antibody: Buffer Exchange the Antibody into Bead-Coating Buffer

 

1.1.1 Block Amicon Filters
Insert one Amicon filter device into the supplied Amicon microcentrifuge tube, ensuring that the filter membranes align with the tube cap strap. 
Dilute IgG stock (2 mg/mL) with 1X PBS to 1 mg/mL. 
Add 500 uL of 1 mg/mL of IgG to the filter. 
Centrifuge at 17000 x g for 1 min at room temperature.
Remove flow thru and liquid from filter.
 
1.1.2 Determine stock antibody concentration with BCA assay (with IgG standards) and A280. 

1.1.3 Calculate Antibody mass for a 150-uL reaction with 30% excess of antibody (e.g., 0.04 mg required for a coating concentration of 0.2 mg/mL). Calculate volume of stock antibody based on desired antibody coating concentration (0.2 mg/mL). 
 

1.1.4 Remove the antibody storage buffer
In a fresh 1.7 mL tube, add the calculated amount of Antibody.
Add sufficient Bead Conjugation Buffer to the Antibody tube to a total volume of 500 µL. 
Vortex and spin down.
Transfer to the pre-blocked Amicon filter and cap the filter.   
Place the filter device in the centrifuge, aligning the cap strap toward the center of the rotor. Counterbalance with a similar device. Centrifuge at 14000 x g for 5 min at Room temperature. 
Keep the flow through in a new separate 1.7 mL tube, then reinsert the filter. 
 


1.1.5 Wash with Bead Conjugation Buffer x2 to buffer exchange: 
Add 450 µL of BCB to the filter, centrifuge at 14000 x g for 5 min at Room temperature, and keep the flow through(s) in new separate 1.7 mL tube (labeled "Wash 1")

 

Repeat this buffer exchange procedure once, discard the flow through. 
 


SECTION: Prepare Capture Beads Concentrate (5-6 hours)
1.2. Recover the Buffer Exchanged Antibody
1.2.1 Invert the filter and place it inside a clean Amicon microcentrifuge tube (the cap will not close). Centrifuge at 1000 x g for 2 min at Room temperature to transfer the washed antibody from the filter to a new 1.7 mL tube (labeled "Buffer Exchanged Antibody").
 
1.2.2 Wash filter membranes:
Add 50 µL of BCB to the filter. Pipette the retained volume multiple times to wash both of the membranes on the filter. 
Carefully invert the filter into the Amicon microcentrifuge tube. 
Centrifuge at 1000 x g for 2 min at Room temperature
Transfer the rinsate from the filter to the buffer exchanged antibody tube.   
Remove the filter from the tube and discard the filter. 
 
1.2.3 Estimate the volume of buffer exchanged antibody, using a P-100 pipette(The antibody should 
         be in a 70~100 µL concentrated volume).  
SECTION: Prepare Capture Beads Concentrate (5-6 hours)
1.3. Dilute the buffer Exchanged Antibody with Bead Conjugation Buffer
1.3.1 Calculate the volume of buffer exchanged antibody required 
Measure and record the buffer exchanged antibody concentration using a BCA assay.
Calculate the volume of buffer exchanged antibody solution required:
         𝐴𝑏.𝐶𝑜𝑎𝑡𝑖𝑛𝑔 𝐶𝑜𝑛𝑐.(𝑚𝑔/𝑚𝐿)×𝐵𝑎𝑡𝑐ℎ 𝑆𝑖𝑧𝑒 (𝜇𝐿) / 𝑀𝑒𝑎𝑠𝑢𝑟𝑒𝑑 𝐴𝑏.𝐶𝑜𝑛𝑐𝑒𝑛𝑡𝑟𝑎𝑡𝑖𝑜𝑛 (𝑚𝑔/𝑚𝐿)=𝑉𝑜𝑙𝑢𝑚𝑒 𝑜𝑓  
         𝐵𝑢𝑓𝑓𝑒𝑟 𝐸𝑥𝑐ℎ𝑎𝑛𝑔𝑒𝑑 𝐴𝑏.(𝜇𝐿)

 


Calculate the required volume of Bead Conjugation Buffer required for the total conjugation 
      batch volume (i.e., 150 μL):
         𝐵𝑎𝑡𝑐ℎ 𝑆𝑖𝑧𝑒 (𝜇𝐿)−𝑉𝑜𝑙𝑢𝑚𝑒 𝑜𝑓 𝐵𝑢𝑓𝑓𝑒𝑟 𝐸𝑥𝑐ℎ𝑎𝑛𝑔𝑒𝑑 𝐴𝑏.(𝜇𝐿)=𝑅𝑒𝑞𝑢𝑖𝑟𝑒𝑑 𝑉𝑜𝑙𝑢𝑚𝑒 𝑜𝑓 𝐵𝑒𝑎𝑑 𝐶𝑜𝑛𝑗𝑢𝑔𝑎𝑡𝑖𝑜𝑛  
         𝐵𝑢𝑓𝑓𝑒𝑟 (𝜇𝐿)

 


Measure the calculated volume of ice‐cold Bead Conjugation Buffer into a 1.7-mL tube.
Add the calculated volume of antibody.
Vortex the tube to mix.
Measure and record the diluted antibody concentration using a spectrophotometer at OD 280, blanked with Bead Conjugation Buffer to confirm the final reaction concentration.
Place the tube of diluted antibody on ice until use.
2.1. 2.1.1 Calculate the volume of beads required for the total conjugation batch volume
Consult the Certificate of Analysis online (via Link: http://www.quanterix.com/sds-and-coas/) using the lot number to determine the stock concentration of the supplied bead concentrate. 
Calculate the volume of well-mixed beads required to supply 1.4 x 109 beads per mL of         conjugation reaction.     
𝐵𝑎𝑡𝑐ℎ 𝑉𝑜𝑙𝑢𝑚𝑒 (𝜇𝐿) x 1.4×10^9 𝐵𝑒𝑎𝑑𝑠/𝑚𝐿/ 𝑆𝑡𝑜𝑐𝑘 𝐵𝑒𝑎𝑑 𝐶𝑜𝑛𝑐𝑒𝑛𝑡𝑟𝑎𝑡𝑖𝑜𝑛 (𝐵𝑒𝑎𝑑𝑠/𝑚𝐿)= 𝑉𝑜𝑙𝑢𝑚𝑒 𝑜𝑓 𝑆𝑡𝑜𝑐𝑘 𝐵𝑒𝑎𝑑𝑠 (𝜇𝐿)

 

          
Vortex the vial of Paramagnetic Carboxylated Beads for 30 seconds, then place on a rotator at 100 rpm at Room temperature for at least 10 min.
Add the calculated volume of well mixed beads to a 1.7 mL microtube.
2.2. Wash Beads 

 

2.2.1 Wash Beads with Bead Wash Buffer x3:
Place the tube in the magnetic separator for at least 1 minute.
Aspirate the supernatant.
Add Batch Volume (i.e. 150 µL) Bead Wash Buffer to the beads. 
Cap the tube and vortex for 5 seconds to disperse the beads. Pulse spin.
Place the tube in the magnetic separator for at least 1 minute to collect the beads to the side of the tube.
Aspirate the supernatant with a pipette.
Remove the tube from the magnet and add Batch Volume (i.e.,150 μL) Bead Wash Buffer to the       beads.
Repeat washing procedure for a total of 3 washes.
 

2.2.2 Wash the beads with cold Bead Conjugation Buffer x2:
Place the tube in the magnetic separator for at least 1 minute to collect the beads to the side of the tube.
Aspirate the supernatant. 
Add Batch Volume (i.e. 150 µL) cold Bead Conjugation Buffer to the beads.
Cap the tube and vortex for 5 seconds to disperse the beads. Pulse spin.
Repeat this washing procedure once, for a total of 2 washes. 

2.2.3 Re-suspend the beads: 
Place the tube in a magnetic separator for at least 1 minute.
Aspirate all of the supernatant. Make sure no residual volume is left.
Calculate the volume of EDC required to activate the beads for 0.3 mg/mL EDC concentration. 
       𝐵𝑎𝑡𝑐ℎ 𝑆𝑖𝑧𝑒 (𝑚𝐿) × 0.3𝑚𝑔/𝑚𝐿 𝐸𝐷𝐶 𝑖𝑛 𝐴𝑐𝑡𝑖𝑣𝑎𝑡𝑖𝑜𝑛 𝑅𝑒𝑎𝑐𝑡𝑖𝑜𝑛/ 10𝑚𝑔/𝑚𝐿 𝐶𝑜𝑛𝑐𝑒𝑛𝑡𝑟𝑎𝑡𝑒𝑑 𝐸𝐷𝐶= 𝑅𝑒𝑞𝑢𝑖𝑟𝑒𝑑   
       𝐸𝐷𝐶 𝑉𝑜𝑙𝑢𝑚𝑒 (𝑚𝐿)

 

        
Resuspend the beads in the Batch Volume (150 uL) of cold Bead Conjugation Buffer, minus the volume of EDC required as calculated above.
        𝐵𝑎𝑡𝑐ℎ 𝑆𝑖𝑧𝑒 (𝑚𝐿)−𝑅𝑒𝑞𝑢𝑖𝑟𝑒𝑑 𝐸𝐷𝐶 𝑉𝑜𝑙𝑢𝑚𝑒 (𝑚𝐿)= 𝐵𝑒𝑎𝑑 𝑅𝑒𝑠𝑢𝑠𝑝𝑒𝑛𝑠𝑖𝑜𝑛 𝑉𝑜𝑙𝑢𝑚𝑒 (𝑚𝐿)

 

            
Add calculated volume of EDC
Remove the tube from the magnet and vortex it to mix the beads. 
Pulse spin and place the tube on ice.
3.1. Activate Beads
3.1.1 Prepare the 10 mg/mL EDC solution:

 
   
 

Remove the 10‐mg vial of EDC from storage. Tap the vial on the bench top gently to force the powder towards the bottom of the vial.
Carefully open the vial of EDC and slowly add 1 mL of ice‐cold Bead Conjugation Buffer.
Cap the vial and vortex it until the EDC is completely dissolved.

3.1.2 Activate the beads:
Vortex the beads well (~30 seconds), and immediately add the required volume of the 10 mg/mL EDC stock (calculated above) to the tube of beads.
 

Cap the tube and vortex for 10 seconds.
Place the tube in a rotator for 30 min   at 2-8 °C . Visually ensure that the mixing is  adequate for a homogenous bead solution during activation.
 


3.2. Wash Beads

 

3.2.1 Wash the activated beads with Beads Conjugation Buffer:
Briefly centrifuge the tube for 1–2 seconds to collect all the liquid into the tube.
Place the tube in the magnetic separator for at least 1 minute to collect the beads to the side of the tube.
Aspirate and discard the supernatant.
Remove the tube from the magnet and add the Batch Volume (i.e., 150 μL) of ice‐cold Bead Conjugation Buffer to the tube.
Vortex for 5 seconds to disperse the beads. Briefly centrifuge the tube for 1–2 seconds to collect all the liquid into the tube.
Place the tube in a magnetic separator with the bead pellet adjacent to the magnet for approximately 1 minute, to collect the beads to the side of the tube. 
Aspirate and discard the supernatant completely.
3.3. Conjugate the antibody to the activated beads:
Remove the tube of activated beads from the magnet.
Add the Batch Volume (i.e., 150 μL) ice‐cold buffer exchanged capture antibody to the beads.
Cap the tube and mix by vortexing for 10 seconds.
Place the tube in the rotator and mix for 120 min at 2-8 °C . Visually ensure that the  mixing is adequate for a homogenous bead solution during activation.

3.4. Clean Up: Wash & Block the Beads
3.4.1 Collect the reaction supernatant:
Briefly centrifuge the reaction tube of activated beads and antibody.
Place the tube in a magnetic separator for at least 1 minute to collect the beads to the side of the tube.
Aspirate the supernatant and dispense it into a new 1.7‐mL tube labeled ‟Supernatant.”
 


3.4.2 Wash the beads 2 times with Bead Wash Buffer:
Remove the tube from the magnet.
Add the Batch Volume (i.e., 150 μL) of Bead Wash Buffer to the tube.
Vortex for 5 seconds to disperse the beads. Briefly centrifuge the tube.
Place the tube in a magnetic separator for at least 1 minute to collect the beads to the side of the tube.
Aspirate the wash liquid and dispense it into a new 1.7‐mL tube labeled ‟Wash 1.”
 

Repeat this washing procedure once, for a total of 2 washes. Discarding the second wash.

3.4.3 Block the beads:
Remove the tube from the magnetic separator.
Add the Batch Volume (i.e., 150 μL) Bead Blocking Buffer to the washed beads.
Vortex for 5 seconds to disperse the beads. Briefly centrifuge the tube.
Place the tube on a rotator and incubate for 45 min at Room temperature . Visually ensure that the mixing is  adequate for a homogenous bead solution during activation.

 


3.4.4 Wash the beads with Bead Wash Buffer:
Briefly centrifuge the tube.
Place the tube in a magnetic separator for at least 1 minute to collect the beads to the side of the tube.
Aspirate the supernatant.
Remove tube from the magnet and add Batch Volume (i.e., 150 μL) of Bead Wash Buffer to the beads.
Vortex for 5 seconds to disperse the beads.
Briefly centrifuge the tube.
Place the tube in a magnetic separator for at least 1 minute to collect the beads to the side of the tube.
Aspirate and discard the supernatant.

3.4.5 Perform the final wash and re‐suspend the beads in Bead Diluent:
Remove the tube from the magnet and add Batch Volume (i.e., 150 μL) Bead Diluent to the beads.
Vortex for 5 seconds to disperse the beads.
Briefly centrifuge the tube.
Place the tube in a magnetic separator for at least 1 minute to collect the beads to the side of the tube.
Aspirate the supernatant.
Remove the tube from the magnet and add Batch Volume (i.e., 150 μL) Bead Diluent.
Mix and then briefly centrifuge the tube to remove beads from the cap.
Store the beads at 2-8 °C until you are ready to use them.

3.5. Clean Up: Determine Antibody Coating Efficiency
3.5.1 Measure the antibody concentration in both the supernatant and the "Wash 1" samples using a      
         spectrophotometer at OD 280 and record the concentration values in the table below.
      • For the supernatant sample, blank using Bead Conjugation Buffer.
      • For the wash sample, blank using Bead Wash Buffer.

3.5.2 Calculate the amount of antibody coated onto the beads.
 
SECTION: Prepare Detector Antibodies (4 hours)
4.1. Prepare the Antibody

4.1.1 Follow instructions in Section 1 to block Amicon filters.   

4.1.2 Remove the detector antibody from storage and allow it to warm to room temperature.
Determine stock Ab concentration with BCA assay (with IgG standards) and A280.  
Calculate the mass of antibody required for a 100‐μL reaction with 30% excess of antibody (e.g., 0.13 mg).
Calculate the volume of antibody solution required to obtain the desired antibody mass. Use the stock antibody label concentration or measure the concentration by a spectrophotometer at OD 280, blanked with the antibody storage buffer.
         𝑅𝑒𝑞𝑢𝑖𝑟𝑒𝑑 𝐴𝑏 𝑀𝑎𝑠𝑠 (𝑚𝑔)𝐴𝑏 𝑆𝑡𝑜𝑐𝑘 𝐶𝑜𝑛𝑐𝑒𝑛𝑡𝑟𝑎𝑡𝑖𝑜𝑛 (𝑚𝑔/𝑚𝐿)=𝑅𝑒𝑞𝑢𝑖𝑟𝑒𝑑 𝐴𝑏 𝑆𝑡𝑜𝑐𝑘 𝑉𝑜𝑙𝑢𝑚𝑒 (𝑚𝐿)

 

4.1.3 Remove the antibody storage buffer:
Insert one Amicon filter device into a supplied Amicon microcentrifuge tube, ensuring that the filter membranes align with the tube cap strap.
Mix the antibody vial by vortexing. Pulse spin.
Add the calculated antibody volume to the filter.
Add sufficient Biotinylation Reaction Buffer to the filter for a total volume of 500 μL and cap the filter.
Place the filter device in the centrifuge, aligning the cap strap toward the center of the rotor.
Centrifuge the tube at 14000 x g for 5 min.
Remove the filter device from the centrifuge and separate the filter from the tube.
Discard the flow through and reinsert the filter into the tube.
Note! The antibody is now concentrated on the filter. Proceed immediately to the next step.

4.1.4 Buffer exchange the antibody using 2 washes with Biotinylation Reaction Buffer:
Add 450 μL of Biotinylation Reaction Buffer to the filter and cap it.
Place the filter device in the centrifuge, aligning the cap strap toward the center of the rotor.
Centrifuge the tube at 14000 x g for 5 min.
Remove the filter device from the centrifuge and separate the filter from the tube.
Discard the flow through.
Repeat this buffer exchange procedure once, for a total of 2 buffer exchanges. If volume in the  filter is greater than 50 μL, repeat the procedure once more, for a total of 3 buffer exchanges.

4.1.5 Recover the antibody:
Invert a clean Amicon microcentrifuge tube onto the top of the filter and invert the assembled device to collect the purified antibody.
Centrifuge the device (with filter inverted) at  1000 x gfor 2 min to transfer the washed antibody from the filter to the tube.
Add 50 μL of Biotinylation Reaction Buffer to the filter.
Pipette up and down multiple times washing both membranes in the filter assembly.
Carefully invert the filter into the same Amicon microcentrifuge tube from step b.
Centrifuge the tube inverted at 1000 x g for 2 min to transfer the rinsate from the filter to the tube.
Remove the filter from the tube and discard the filter.
Cap the tube and retain it.

4.1.6 Adjust the antibody concentration to 1 mg/mL:
Measure and record the buffer exchanged antibody concentration using a spectrophotometer at OD 280, blanked with biotinylation reaction buffer.
Estimate the volume of buffer exchanged antibody, using a P‐100 pipette.
Calculate and record the amount of Biotinylation Reaction Buffer to add to adjust the antibody (Ab) concentration to 1 mg/mL.
        [ 𝐴𝑏 𝐶𝑜𝑛𝑐.(𝑚𝑔𝑚𝐿)×𝐴𝑏 𝑣𝑜𝑙.(𝜇𝐿)/1 𝑚𝑔/𝑚𝐿] −𝐴𝑏 𝑣𝑜𝑙.(𝜇𝐿)=𝑅𝑒𝑎𝑐𝑡𝑖𝑜𝑛 𝐵𝑢𝑓𝑓𝑒𝑟 𝑣𝑜𝑙.(𝜇𝐿)

 

Add the calculated volume of Biotinylation Reaction Buffer to the concentrated antibody. Cap the tube and vortex for 5 seconds to mix.

4.1.7 Confirm the antibody concentration and volume and record the findings:
Measure and record the antibody concentration using a spectrophotometer at OD 280, blanked with Biotinylation Reaction Buffer. The target concentration is 0.95 – 1.05 mg/mL.
Estimate the volume of antibody using a P-100 pipette.

SECTION: Prepare Detector Antibodies (4 hours)
4.2. Conjugate
4.2.1 Remove 1 vial of NHS‐PEG4‐Biotin from –20°C storage and allow it to warm to room temperature.
 

4.2.2 Reconstitute the NHS‐PEG4‐Biotin to a 8.9 mM stock concentration:
Immediately before use, unscrew the yellow cap.
Add 383 μL of deionized water.
Mix by pipetting up and down. Alternatively, the vial can be vortexed for a few seconds to ensure a homogeneous solution.

4.2.3 Measure into a new 1.7‐mL tube the required volumes of 1 mg/mL antibody, reconstituted NHS‐PEG4‐Biotin, and Biotinylation Reaction Buffer for the detector concentration that you want to prepare, according to the following table. NOTE: use values correlating to a 40x ratio to start.
 
4.2.4 Mix the reaction by vortexing.
4.2.5 Centrifuge the tube for 2 seconds to collect all the liquid into the bottom of the tube.
4.2.6 Incubate the tube for 30 min minutes at rRoom temperature

 

SECTION: Prepare Detector Antibodies (4 hours)
4.3. Purify the Biotinylated Antibody
4.3.1 Concentrate the antibody:
Follow instructions in Section 1 to block Amicon filters.  

 

Add all of the conjugated antibody to the blocked Amicon filter.
Add sufficient Biotinylation Reaction Buffer to the filter for a total volume of 500 μL (approximately 400 μL) and cap the filter.
Place the filter device in the centrifuge, aligning the cap strap toward the center of the rotor. Centrifuge at 14000 x gfor 5 min.
Remove the filter device from the centrifuge and separate the filter from the tube.
Discard the flow through and reinsert the filter into the tube.

4.3.2 Purify the antibody using 4 washes with Biotinylation Reaction Buffer:
Add 450 μL of Biotinylation Reaction Buffer to the filter and cap it.
Place the filter device in the centrifuge, aligning the cap strap toward the center of the rotor.  Centrifuge at 14000 x g for 5 min.
Remove the filter device from the centrifuge and separate the filter from the tube.
Discard the flow through.
Repeat this washing procedure 3 times, for a total of 4 washes.

 

4.3.3 Recover the antibody and Storage:
Invert a clean Amicon microcentrifuge tube onto the top of the filter and invert the assembled device to collect the purified antibody.
Centrifuge the device (with filter inverted) at 1000 x g for 2 min to transfer the washed antibody from the filter to the tube.
Add 50 μL of Biotinylation Reaction Buffer to the filter.
Pipette up and down multiple times washing both membranes in the filter assembly.
Carefully invert the filter into the same Amicon microcentrifuge tube from step b.
Centrifuge the tube inverted at 1000 x g for 2 min to transfer the rinsate from the filter to the tube.
Remove the filter from the tube and discard the filter.
The final detector concentrate should be in a 90-µL volume. Store the concentrate at 4 °C until use. 

4.3.4 Characterization
Measure and record the concentration of biotinylated antibody using a spectrophotometer at OD 280, blanked with Biotinylation Reaction Buffer.
Calculate the antibody Biotinylation reaction yield:
[𝐹𝑖𝑛𝑎𝑙 𝐷𝑒𝑡𝑒𝑐𝑡𝑜𝑟 𝑉𝑜𝑙𝑢𝑚𝑒 (𝜇𝐿) x 𝐷𝑒𝑡𝑒𝑐𝑡𝑜𝑟 𝐶𝑜𝑛𝑐𝑒𝑛𝑡𝑟𝑎𝑡𝑖𝑜𝑛 (𝑚𝑔/𝑚𝐿)]/ [𝑅𝑒𝑎𝑐𝑡𝑖𝑜𝑛 𝑉𝑜𝑙𝑢𝑚𝑒 (𝜇𝐿)x𝑅𝑒𝑎𝑐𝑡𝑖𝑜𝑛 𝐶𝑜𝑛𝑐𝑒𝑛𝑡𝑟𝑎𝑡𝑖𝑜𝑛 (𝑚𝑔/𝑚𝐿)]×100%

 

SECTION: Perform Simoa Assay (5 hours)
5.1. Preparing Reagent Solutions
5.1.1 Determine the number of individual samples that will be run, including calibrators and samples 
        that will be diluted manually on the SR-X Analyzer.

5.1.2 Prepare Bead Reagent
Based on the bead concentration determined previously (1.4 x 10^9 beads /mL), calculate the volume of bead concentrate required to yield a solution of sufficient volume (calculated below) at a working concentration of 2.0 x 10^7 beads/mL (25 uL bead reagent per test/reaction, which gives 500k beads per reaction).
((𝑅𝑒𝑎𝑔𝑒𝑛𝑡 𝑉𝑜𝑙𝑢𝑚𝑒 𝑅𝑒𝑞𝑢𝑖𝑟𝑒𝑑 𝑝𝑒𝑟 𝑡𝑒𝑠𝑡+10 μL) × 𝑁𝑢𝑚𝑏𝑒𝑟 𝑜𝑓 𝑡𝑒𝑠𝑡𝑠)x 25 uL 𝐵𝑒𝑎𝑑    

𝑉𝑜𝑙.𝐶𝑜𝑛𝑐𝑒𝑛𝑡𝑟𝑎𝑡𝑒𝑑 𝐵𝑒𝑎𝑑 𝑆𝑡𝑜𝑐𝑘 𝑅𝑒𝑞.(𝑚𝐿)= [𝑊𝑜𝑟𝑘𝑖𝑛𝑔 𝑉𝑜𝑙 𝐵𝑒𝑎𝑑 𝑅𝑒𝑎𝑔𝑒𝑛𝑡 𝑅𝑒𝑞. (𝑚𝐿) ×𝑊𝑜𝑟𝑘𝑖𝑛𝑔 𝐵𝑒𝑎𝑑 𝐶𝑜𝑛𝑐𝑒𝑛𝑡𝑟𝑎𝑡𝑖𝑜𝑛(𝑏𝑒𝑎𝑑𝑠/𝑚𝐿)]/ 𝐵𝑒𝑎𝑑 𝑆𝑡𝑜𝑐𝑘 𝐶𝑜𝑛𝑐𝑒𝑛𝑡𝑟𝑎𝑡𝑖𝑜𝑛 (𝑏𝑒𝑎𝑑𝑠/ 𝑚𝐿)

 

Vortex the bead stock for at least 30 seconds to completely resuspend beads.
Add calculated volume of bead stock to 1.7-mL tube.
Add 300 uL of Bead Diluent to the beads. Vortex to mix.
Vortex this tube briefly (followed by a spin if beads get lodged into the lid), then place on the magnetic rack.
Wait for ~60 seconds (when all beads have pelleted to the side of the tube) then carefully remove supernatant.
Take tube off magnet and add back ~300uL bead diluent, repeat these steps x2.
In final wash leave the beads in the 300uL diluent.     
Add the appropriate/calculated volume of Bead Diluent (Working Vol. Bead Reagent Req.)to the bead stock and vortex to mix. Keep this on ice until needed. 

5.1.3 Prepare Detector Reagent
Based on the detector stock concentration determined previously, calculate the volume of detector   stock required to yield a solution of sufficient volume (calculated above) at the desired working concentration. A final detector concentration of 0.1-0.3 μg/mL may be appropriate for a preliminary test of untested reagents.
𝑉𝑜𝑙.𝐷𝑒𝑡𝑒𝑐𝑡𝑜𝑟 𝑆𝑡𝑜𝑐𝑘 𝑅𝑒𝑞.(𝑚𝐿)= 𝑊𝑜𝑟𝑘𝑖𝑛𝑔 𝑉𝑜𝑙 𝐷𝑒𝑡𝑒𝑐𝑡𝑜𝑟 𝑅𝑒𝑎𝑔𝑒𝑛𝑡 𝑅𝑒𝑞.(𝑚𝐿) × 𝑊𝑜𝑟𝑘𝑖𝑛𝑔 𝐷𝑒𝑡𝑒𝑐𝑡𝑜𝑟 𝐶𝑜𝑛𝑐. ( 𝜇𝑔/𝑚𝐿)/ 𝐷𝑒𝑡𝑒𝑐𝑡𝑜𝑟 𝑆𝑡𝑜𝑐𝑘 𝐶𝑜𝑛𝑐.(𝜇𝑔/𝑚𝐿)

 

Spike the volume of detector stock calculated above into the appropriate volume of Detector Diluent in a 1.7 uL tube. 
Keep this on ice until needed.


5.1.4 Prepare SBG Reagent     

 

Prepare a 150 pM solution of SBG with the fill volume calculated below using SBG Concentration (stock concentration 50mM) by spiking the required volume concentrate into the appropriate volume of SBG Diluent in a 15 mL tube.
  𝑉𝑜𝑙𝑢𝑚𝑒 𝑆𝐵𝐺 𝑆𝑡𝑜𝑐𝑘 𝑅𝑒𝑞𝑢𝑖𝑟𝑒𝑑 (𝑚𝐿)= [𝑉𝑜𝑙 𝑆𝐵𝐺 𝑆𝑜𝑙𝑢𝑡𝑖𝑜𝑛 𝑅𝑒𝑞.(𝑚𝐿)× 150 𝑝𝑀/ 𝑆𝐵𝐺 𝑆𝑡𝑜𝑐𝑘 𝐶𝑜𝑛𝑐. (𝑛𝑀)]× [1 𝑛𝑀1000 𝑝𝑀]

 

Label the tube and store at room temp until needed.

5.1.5 Prepare Homebrew Sample Diluent Reagent
Base on the number of samples and dilution factors needed for samples, calculate the volume of sample diluent required.
Spike in appropriate amount of sodium dodecyl sulfate, sodium deoxycholate and freshly prepared dithiothreitol to Homebrew Sample Diluent Buffer to the desired concentration described in the table below.
     Sodium Dodecyl Sulfate      0.1%        Sodium Deoxycholate      0.05%        Dithiothreitol      0.4mM   

SECTION: Perform Simoa Assay (5 hours)
5.2. Prepare standards and samples
5.2.1 Prepare standards
 

  was used as standard in this Homebrew Assay. Use Homebrew Sample Diluent Buffer to produce a dilution series (ranging from 1000 pg/mL to 0.1 pg/mL). Use Homebrew Sample diluent as the zero standard (0 pg/mL).
Transfer 100 µL of each standard to the desired wells of the 96-well assay plate.  


5.2.2 Prepare samples
 

 

Quick thaw samples in water bath at 37 °C.
Immediately transfer sample tubes on ice.
For each sample to be tested, transfer the appropriate volume of sample diluent to
the desired wells of the 96-well assay plate. Add the appropriate volume of well mixed sample (e.g. 5ul samples + 95 uL Sample Diluent Buffer) and mix briefly by pipetting up and down. 

SECTION: Perform Simoa Assay (5 hours)
5.4. Starting the Assay
5.4.1  Incubate plate and RGP Reagent on the Microplate Shaker.
 
 


Set up temperature and shaking speed on Microplate shaker. (optimized 2-step protocol is used in this assay in West lab).
Incubate the samples, calibrators, and bead solution with detector solution at RT on the microplate shaker at 800 rpm for 60 min. Cover plate with lid or aluminum foil during incubation.
Prior to use, RGP must be solubilized fully by heating with constant vigorous shaking. Incubate RGP bottle in the plate shaker at 800 rpm. Minimum required shaking time at specific temperature is shown below:
 


5.4.2 Wash the plate on the Microplate Washer.
 
Check and refill Wash Buffer in A and B and Milli-Q water in C.
Empty the waste bottle.
After incubation completed, transfer the plate to the Microplate washer, remove lid.
Begin the semi-automated 2-step assay on the Simoa Washer.  
 
After the first wash, incubate samples with 100 uL SBG for 10 minutes at 37 °C at   on the Microplate shaker.
 

When the 2-step assay wash protocol has been completed, check the positions of the bead pellets in the wells. If the pellets are too high, manually add buffer B to the well, shake, place back on magnet, and aspirate buffer. 

 
5.4.3 Analyze the plate on Quanterix SR-X (2 hours)
Turn on the SR-X.
Select "Run" on the home page.

 
Load the tips, micro-discs and RGP onto the instrument, ensure the waste is emptied and sealing Oil is enough (2-3% of sealing oil will be used per run).
 
Choose a proper Homebrew analysis protocol and define plate layout.
 
 When the semi-automated protocol has been completed and the assay plate is dry, transfer the plate to the Quanterix SR-X.
 

Start the run. 
 
 


SECTION: Perform Simoa Assay (5 hours)
5.3. Load Bead  and Detector Reagents to the plate  
Add the appropriate volume of beads and detectors to desired wells of the assay plate.
For 2-step Dispense Protocol, 25 uL of Beads and 20 uL of Detector reagent were loaded to each well.