BHQplus Probes

Technical Specs

FAQs

• Product Usage:

  • 

    Can I use the Nanodrop® to measure the concentration of synthetic oligonucleotides?

    Nanodrop® technology can be used to measure the concentration of individual synthetic oligos using each oligonucleotide's unique analysis constant. By default, the Nanodrop equipment uses a value of "33" as a general constant for all single-stranded DNA, which is inappropriate for synthetic DNA. Oligonucleotides purchased through LGC Biosearch Technologies arrive with data sheets containing the extinction coefficient and molecular weight of each oligonucleotide. These numbers are used to calculate the analysis constant needed for Nanodrop concentration calculations.

    Use the formula below to calculate the Analysis Constant (AC):
    AC = (1/extinction coefficient) x (Molecular Weight (protonated)) x 1000 = AC in micrograms per OD260nm

    We have determined through internal research that when measuring labeled oligonucleotides, the Nanodrop's linear range of detection is much more limited than advertised. For oligonucleotide stocks in the 100 µM range, the Nanodrop will record an apparent concentration that is significantly below the actual concentration. For accurate measurements, we recommend diluting 100 µM stocks by 25-fold to achieve a concentration in the range of 4 µM.

  • 

    How do you determine the brightness of a dye?

    The absolute intensity of a dye is a product of the extinction coefficient and the quantum yield. We have not measured the quantum yield for our dyes as this value is highly dependent upon the local environment, including the buffer system used for the measurement. However, we do provide the extinction coefficients for dye modifications at their lambda max wavelength, and these values are available under the Technical Specs tabs of our Oligo Modifications webpages. While quantum yield and extinction coefficients both contribute to dye detectability, the principal determinant for Stellaris® RNA FISH assays is actually the instrument optics, including the excitation source, available filters, and quantum efficiency of the camera.

  • 

    How do I quantify oligonucleotides by spectrophotometer?

    Here is a protocol for the Quantification of Oligonucleotides by Spectrophotometer:

    1. Add an aliquot of the resuspended oligonucleotide into a volume of PBS so that the total volume is 1000 µl. Typical dilutions are 1:20 or 1:40 where the dilution factor (DF) is 1000/aliquot volume.
    2. Vortex or pipette up and down repeatedly for 15 seconds.
    3. Read the absorbance of this dilution at 260 nm (OD260). Use the average of at least 2 reads.
    4. Calculate concentration using the nmol/OD260 value presented on the Certificate of Analysis, i.e. multiply (nmol/OD260) x (average OD260) x (Dilution Factor) = [C], concentration in µM (micromolarity).
  • 

    How do I calibrate my instrument for the CAL Fluor® and Quasar® Dyes?

    CAL Fluor® and Quasar® dye calibration standards are designed to improve the accuracy of signal detection in real-time thermal cyclers that require spectral calibration. They enable the instrument to store the fluorescence profile of each dye and control for channel cross-talk. Crosstalk is the bleed-through of fluorescent signal from a reporter into an adjacent filter or channel, an issue of particular concern in a multiplexed assay. Many qPCR machines are pre-calibrated for Cy™3 and Cy5 dyes. In those machines, no calibration is necessary to use our Quasar 570 (Cy3 alternative) and Quasar 670 (Cy5 alternative) dyes. To use our CAL Fluor dye labels, particularly in a multiplexing assay, certain real-time PCR instruments need to be calibrated to anticipate crosstalk. LGC Biosearch Technologies does not make available pure dyes. Instead, our calibration standards are formulated to better mimic a fluorescent probe under experimental conditions by covalently linking the dye to an oligo-thymidine (dT10).  A complete list of available Calibration and Reference Dyes is available through our website. Instructions to calibrate select qPCR machines are available in our Spectral Calibration Instructions.

  • 

    How many PCR reactions will I be able to run with my probe or primer?

    The number of reactions per nmol of product delivered is dependent upon the concentration to be used and final reaction volume. Typically, 1 nmol of a primer designed for qPCR will provide sufficient material for at least 100 reactions if used at a 300 nM final concentration in a 20 µL total volume. Likewise, 1 nmol of dual-labeled BHQ probe will provide sufficient material for up to 500 reactions if used at a 100 nM final concentration in a 20 µL total volume.

  • 

    How do I adjust my thermal cycler’s settings to account for the BHQ® quencher?

    Dual-labeled BHQ®, BHQplus®, or BHQnova™ probes may be used on any qPCR instrument. These probes exhibit extremely low background fluorescence, enhancing detection sensitivity. The selection process for the quencher dye during set-up varies between instruments. Because Black Hole Quencher® dyes have no fluorescence emission, simply choose the setting for 'Non-fluorescent', 'dark quencher' or ‘none’.

• qPCR:

  • 

    What is the difference between static quenching and FRET?

    The static quenching mechanism is the formation of an intramolecular dimer between reporter and quencher, to create a non-fluorescent ground-state complex with a unique absorption spectrum. In contrast, the FRET quenching mechanism is dynamic and does not affect the probe's absorption spectrum. With either mechanism, disruption of quenching through hydrolysis of the probe releases signal from the fluorophore.
    
    For more information, please visit our Quenching Mechanisms in Probes webpage.

  • 

    Which dyes are compatible with my thermal cycler?

    LGC Biosearch Technologies offers many common fluorophores including FAM, HEX and TAMRA dyes, as well as our own proprietary dyes. Our CAL Fluor® and Quasar® dye series span the spectrum with emission wavelengths ranging from yellow to far-red, and represent alternatives to dyes such as VIC®, Cy™3, Texas Red, LC Red® 640, Cy5, and Cy5.5. For your convenience we have compiled a Multiplexing Dye Recommendations Chart outlining optimal dye combinations in select qPCR machines, as well as a Fluorophore & BHQ® Dye Selection Chart listing reporter-quencher pairings. In addition, you may use our Spectral Overlay Tool to visualize the absorption and emission spectra of multiple dyes together.

  • 

    I am a beginner at real-time qPCR. Does LGC Biosearch Technologies have information which will help me to design my assay?

    For an overview of available Dual-labeled BHQ® probe types, their mode of action and basic design guidelines, you may download our Fluorogenic Probes and Primers Brochure.

    For an in depth discussion on qPCR, including probe and primer design, we recommend reading the book entitled 'A-Z of Quantitative PCR' edited by Stephen A. Bustin.

    Additional resources are available on-line, including the website 'REAL-TIME PCR' maintained by M. Tevfik Dorak, MD, Ph.D., which offers a review of major topics for qPCR and historical links to valued information.

    For MIQE guidelines on experiment design, please see the original publication entitled, "The MIQE guidelines: minimum information for publication of quantitative real-time PCR experiments", by Bustin et al.

    For applications and the most recent methods in gene expression analysis, visit the website named 'www.Gene-Quantification.info: The Reference in qPCR - Academic & Industrial Information Platform'. This site offers many links to additional resources on qPCR.

    When you are ready to design your assay, use our FREE and user-friendly RealTimeDesign® software, available through our website.
  • 

    Is there a formula for calculating the efficiency of a qPCR reaction?

    For a singleplex reaction, the efficiency of qPCR is calculated as follows:

    Efficiency = 10^(-1/slope) - 1

    The slope is derived from a graph of Cycles to Threshold (Ct) values plotted against the Log₁₀ of the template amount. A slope of -3.32 indicates an amplification efficiency of 100%.

    Resource: Gene quantification using real-time quantitative PCR: An emerging technology hits the mainstream. David G. Ginzinger. Experimental Hematology 30 (2002): 503-512

  • 

    Does LGC Biosearch Technologies make available information on multiplex qPCR?

    For information on qPCR assay design, validation and troubleshooting please visit our Multiplexing qPCR webpage and review the information under the tabs. Additional information is presented in our blog series, The BiosearchTech Blog. If you have further questions, please contact our Technical Support team.

• Building Probes/Primers:

  • 

    What is the difference between Black Hole Quencher® (BHQ®) dye and TAMRA?

    TAMRA dye is an effective quencher for fluorophores with emission maxima less than 560 nm. Dyes with longer wavelength emissions will not be effectively quenched by TAMRA. In addition, TAMRA has its own fluorescence which complicates data analysis due to crosstalk between the channels. In contrast, Black Hole Quencher® dyes are true "dark" quenchers with no fluorescent signal. Their use simplifies design, implementation and interpretation of qPCR assays.

    Furthermore, BHQ® dyes have broad absorption spanning 480-580 nm (BHQ-1), 559-670 nm (BHQ-2) and 620-730 nm (BHQ-3), to enable use of a large range of spectrally distinct reporter dyes in multiplexed assay designs. With some dye pairings, FRET quenching is supplemented by the static quenching mechanism. Specifically, hydrophobic and electrostatic interactions facilitate the association of BHQ dyes with certain reporters to form an intramolecular dimer, for enhanced quenching and improved signal to noise ratios. Thus, BHQ dyes may quench some fluorophores whose emission spectrum is beyond the limits of BHQ absorption. For more information on FRET and static quenching mechanisms in qPCR please visit our Quenching Mechanisms in Probes website.

  • 

    What is the difference between BHQ® and BHQplus® Probes?

    BHQ® probes are oligonucleotides with a Black Hole Quencher® modification, either internal or at the 3' end. While BHQ probes are typically 20 - 30 bases in length, BHQplus® probes are typically 15 - 25 bases in length. BHQplus probes are an advanced probe type with duplex-stabilizing chemistry to allow for the design of shorter oligonucleotides with relatively high melting temperatures. BHQplus probes are used to detect difficult targets, such as AT-rich regions or SNPs.
  • 

    What is the difference between LGC Biosearch Technologies' Quasar® dyes and the Cy™ dyes?

    The Quasar® dyes may be used as direct replacements for the Cy™ dyes and are anticipated to perform equivalently to their Cy dye counterparts. They share the same chromophore structure and spectral properties, differing principally in their linkage chemistry. Quasar 570 replaces Cy3, Quasar 670 replaces Cy5 and Quasar 705 replaces Cy5.5 dye. Quasar dyes are slightly more hydrophobic and therefore soluble in the reagents of DNA synthesis. Importantly, the Quasar dyes are available as amidites and may be incorporated during oligonucleotide synthesis, thus avoiding the post-synthesis dye conjugation required with Cyanine dyes.

  • 

    What different oligonucleotide purification options does LGC Biosearch Technologies offer?

    LGC Biosearch Technologies offers a full range of purification options including: Salt-free, Reverse Phase Cartridge (RPC), Reverse Phase HPLC (RP-HPLC), Anion Exchange HPLC (AX-HPLC) and Dual-HPLC (AX-HPLC followed by RP-HPLC). They are listed from least to most stringent, with the appropriate purification depending entirely on the application.

    For unlabeled oligonucleotides, such as qPCR primers, Salt-free or RPC purification is appropriate. For other applications using unmodified oligonucleotides we encourage RPC purification which typically provides ~70 % purity. With RPC purification, contaminants such as truncated sequences, ammonium salts and impurities are removed from the final product. In this process, the oligos are synthesized with the DMT group left on the final base which allows for separation by affinity of the DMT group to the resin in the cartridge. Truncated sequences will not have the final DMT group, will not bind to the cartridge and will be washed away.

    RP-HPLC is selected to eliminate fluorescent contaminants that remain following synthesis of a labeled oligo. When allowed to persist, this impurity elevates the baseline fluorescence and obscures the detection of probe signal. RP-HPLC typically yields products with ~80 % purity. This purification technique is similar to RPC purification except the resins provide greater sample capacity.

    AX-HPLC is selected to eliminate failure sequences that result from poor reporter or base coupling during the synthesis. When allowed to persist, this impurity competes with the oligo for binding to the target sequence which may result in delayed CT values in a qPCR reaction.

    For Dual-labeled BHQ® probes we recommend at a minimum RP-HPLC purification, but default to Dual-HPLC which typically provides products with ~90 % purity.

    In oligonucleotides containing wobbles, we avoid AX-HPLC which skews the ratio of different species synthesized in unison.

    For more information, please review our Default and Recommended Methods of Purification Chart.

  • 

    What are "wobbles"?

    When comparing multiple sequences, one may find that alignment reveals no region with sufficient consensus to accommodate a unique single oligonucleotide for use as a primer or probe. In some cases, only one or two nucleotides are mismatched. When designing primers for those regions, one may choose to introduce a degenerate site, or "wobble", to compensate for the variability in the target sequence. Letter codes are used to represent the combination of two or more different nucleotide phosphoramidites blended at equimolar ratios prior to coupling at that position in the sequence. The final product is a blend of two or more different sequences made simultaneously during one synthesis.
    
    2 nucleotide wobble
    R = A+G
    W = A+T
    M = A+C
    Y = C+T
    S = C+G
    K = G+T
    
    3 nucleotide wobble
    B = C+T+G
    D = A+G+T
    H = A+C+T
    V = A+C+G
    
    Universal wobble
    N = A+C+T+G
  • 

    Does LGC Biosearch Technologies offer VIC®, NED or PET dyes?

    LGC Biosearch Technologies does not offer VIC®, NED or PET dyes as they are proprietary to Applied Biosystems, Inc. (part of Life Technologies). These dyes are often used for sequencing or fragment analysis, but other long-wavelength dyes do not perform well in fragment analyzers, such as the ABI 3730 series.  These types of instruments use a single wavelength (488 nm) for excitation which poorly excites red-shifted dyes. Applied Biosystems circumvents this problem by partnering red dyes such as NED with a FAM dye in a FRET construct. LGC Biosearch does not offer these “Big Dye” constructs and so we advise testing our dyes on an experimental basis for fragment analysis.

    For qPCR applications we do not offer direct replacements for NED or PET dyes, however, we do offer alternatives for VIC.  Our recommended VIC substitute depends on the optics of your qPCR machine which can be determined on our Multiplexing Dye Recommendations Chart. 

  • 

    Are locked nucleic acids (LNA™) available through LGC Biosearch Technologies?

    LGC Biosearch Technologies is not licensed to synthesize oligos with locked nucleic acid (LNA™) modifications.

  • 

    Does the LGC Biosearch Technologies' website have a list of all dyes available for DNA labeling?

    LGC Biosearch Technologies offers modified oligos with many common fluorophores including FAM, HEX and TAMRA, as well as our own proprietary dyes. Please refer to our Black Hole Quencher® and Dye Selection Chart for a complete list of various dyes/fluorophores we carry at LGC Biosearch.

    LGC Biosearch makes available many of these same dyes as reactive precursors for others to synthesize their own modified oligos. A full list of dyes and quenchers formulated for that purpose can be found in on our webpage for DNA/RNA Synthesis Reagents.

    To manually label oligos and other biomolecules, LGC Biosearch also offers carboxylic acid and succinimidyl ester formulations of certain dyes and quenchers. A complete list can be found on our Labeling Reagents webpage.

    If you have any questions regarding the availability of particular products, please contact our Technical Support team.

  • 

    What Black Hole Quencher® do you recommend for dyes with long wavelength emissions, such as the Quasar® and Pulsar® dyes?

    The BHQ®-2 dye is our preferred quencher for long wavelength fluorophores. This recommendation relates to the ease of manufacture using BHQ-2 over BHQ-3 dye. While both dyes represent excellent quenchers, the final yield is usually higher with BHQ-2 modified oligonucleotides, thus providing a more cost-effective synthesis with excellent purity and performance characteristics.
    
    In the context of Dual-labeled BHQ probes, the BHQ-2 dye is an excellent quencher for long wavelength emitters such as Quasar® 670, Quasar 705, and Pulsar® 650. With some dye pairings, FRET quenching is supplemented by the static quenching mechanism. Specifically, hydrophobic and electrostatic interactions facilitate the association of BHQ dyes with certain reporters to form an intramolecular dimer, for enhanced quenching and improved signal to noise ratios. Thus, BHQ dyes may quench some fluorophores whose emission spectrum is beyond the limits of BHQ absorption. More information on FRET and static quenching can be found on our Quenching Mechanisms in Probes webpage.

  • 

    Do unlabeled primers have a 3' phosphate?

    Unless otherwise requested at the time of the order, unlabeled primers are synthesized with free hydroxyls at both the 5' and 3' ends. Terminal phosphate modifications are available as custom modifications only.
    
    For a list of available modifications and associated pricing, please visit our Oligo Modifications webpage or contact our Customer Service team.

  • 

    Where can I find information that explains the differences between each of the probe types you offer?

    We offer a number of different qPCR probe types for your convenience, including: Dual-labeled BHQ® probes, BHQnova™ probes, BHQplus® probes, Molecular Beacons, and Scorpions® Primers. For detailed information about how these probes work, please watch our Real-time PCR Probe Animation Video. You may also download our Fluorogenic Probes and Primers Brochure.

• RealTimeDesign Software:

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    How do I enter in a SNP, MNP or InDel sequence into the RealTimeDesign™ software?

    Users must select the 'SNP Genotyping' application in order to have the RealTimeDesign™ (RTD™) software design assays to detect Single Nucleotide Polymorphisms (SNPs), Multi-Nucleotide Polymorphisms (MNPs) or Insertions/Deletions (InDels). Users need to annotate the polymorphism in one of the following formats:
    
    Single Nucleotide Polymorphism: [C/T] where C and T represent the single base pair mismatch. Alternatively, users can use the IUPAC code for the SNP represented in the following list:
    
    Nucleic acid codes:
    

    R = Purine (A or G) Y = Pyrimidine (C, or T) M = C or A K = T or G W = T or A

    S = C or G B = C, T, or G (not A) D = A, T, or G (not C) H = A, T, or C (not G) V = A, C, or G (not T)

    N = Any base (A, C, G, or T)

    Multi-Nucleotide Polymorphisms:
    [CA/GT] where CA and GT represent the multi-nucleotide mismatch
    
    Insertions/Deletions:
    [CA/-] where CA represents the insertion.
    
    To review this information while using RealTimeDesign software, use the pull down window for the Legend when designing in Custom mode.
  • 

    Does LGC Biosearch Technologies have software available for designing probes and primers?

    For the design of qPCR primers and probe sets, we offer our RealTimeDesign™ (RTD™) software. The RTD software is free, easy to use and can be accessed directly through your web browser. Our software offers a choice of design modes: an 'Express Mode' with pre-set parameters and a 'Custom Mode' in which the parameters can be adjusted by the user. There is an additional 'Batch Mode' which facilitates the design of up to 10 assays in series. 

  • 

    I have my own primer designs. Can LGC Biosearch Technologies' RealTimeDesign™ (RTD™) software design only the probe for me?

    To design a probe for compatibility with pre-designed primers, select application and design mode, then select the 'Include/Exclude' box at the bottom of the second pull-down menu. In the next screen, users may input the desired primer sequences into the 'Anchored' column of the oligonucleotide table. The RealTimeDesign™ (RTD™) software will then proceed to design a Dual-labeled BHQ® or BHQplus® probe within those predefined primer sequences.

    Note: LGC Biosearch Technologies does not recommend using primers designed outside of the RTD software because primers used for other applications (e.g. gel electrophoresis) are often inappropriate for qPCR. The RTD software uses parameter settings that are proven to design primers and probe sets with optimal performance.

  • 

    Is there any way of designating a specific region of my sequence for the RealTimeDesign™ software to design my primers, probe and assay?

    RealTimeDesign™ software users may restrict assay design to include a specific sequence location, i.e. an intron splice site, by placing a tilde (~) character within the sequence.
    
    For example: CAAAGGGTTGCAC~AAGATGGATGATCG
  • 

    How do I determine which design mode to use in LGC Biosearch Technologies' RealTimeDesign™ software?

    The RealTimeDesign™ (RTD™) software offers three different levels of user control to accommodate a range of needs:

    Express Mode - is designed with simplicity in mind. This mode does not require any input from the user other than sequence submission and label selection.

    Custom Mode - is designed for the advanced user who wishes to inspect, include or exclude certain oligonucleotide candidates from each stage of the design process. This mode provides the user with access to the parameter settings for advanced control.

    Batch Mode - is similar to Express Mode however it allows users to initiate designs against as many as 10 target sequences and close the browser while they wait. An email will be sent alerting the user that the designs have completed.

    All designs may be reviewed on the Design Run History page.

  • 

    How do I order the primers and probe I have designed using the RealTimeDesign™ software?

    Once the RealTimeDesign™ (RTD™) software generates an assay design, users may review the primers and probe by clicking on the assay number. After reviewing the oligo sequences, you may order them on-line by clicking the 'ADD TO CART' button. In the next screen, you will be able to select the name, purification, quantity and synthesis scale for each primer and probe. Once all fields are filled in, click 'ADD TO CART' again. A window will inform you that the products have been successfully added to your cart, and you may continue shopping or else proceed to check out. In the 'CHECK OUT' window you will be required to fill in the purchasing information. To finalize the order, click 'NEXT' and confirm the information presented. When ready to place the order, click 'SUBMIT'.
  • 

    Within the RealTimeDesign™ software, how do I find the primers and probe sequences after I design them?

    RealTimeDesign automatically maintains a record of all past designs for each user’s account. To retrieve previous primer and probe designs through RTD, login and click on 'Main Menu', then select 'Design Run History'. All design records are listed with the most recent at the top and available for review by selecting 'Details'. If your designs are not listed, search the archived designs by clicking on the checkbox for 'Show Archived Runs'.
  • 

    How is the Tm calculated in LGC Biosearch’s Technologies' RealTimeDesign™ software?

    Our RealTimeDesign™ (RTD™) uses the SantaLucia "unified" nearest neighbor thermodynamic parameters in the algorithm to calculate melting temperature (or T_M). There are often discrepancies between the T_M values predicted using RTD and those of other programs due to different thermodynamic values and also different concentrations for the assay components. These differences are further explained in the following reference: Comparison of different melting temperature calculation methods for short DNA sequences. Alejandro Panjkovich and Francisco Melo. Bioinformatics 2005 21(6):711-722; 2004 doi: 10.1093/bioinformatics/bti066

    For more information, consider the publication: "A unified view of polymer, dumbbell, and oligonucleotide DNA nearest-neighbor thermodynamics", by John SantaLucia, Jr.

    We also recommend a general web tool to model oligo binding called DINAMelt, which can be adapted to a variety of experimental conditions. DINAMelt draws upon the same SantaLucia thermodynamic values as RTD, and a description of its algorithms may be found in the following publication: DINAMelt web server for nucleic acid melting prediction. Markham NR, Zuker M. Nucleic Acids Res. 2005 Jul 1;33:W577-81.

  • 

    What are the differences in parameter settings between the various modes within the RealTimeDesign™ software?

    The 'Most Restrictive' parameter set dictates very stringent guidelines for assay design. The resulting assays propose a short amplicon length (up to 100 bases), a short probe design (25 bases), a short interval between the forward primer and probe (no more than 10 bases distant) and no stable misalignments within and between the primers. While a robust PCR reaction may tolerate rule breaking without performance impact, this parameter set errs on the conservative side of caution. We recommend attempting to design your assay using the 'Most Restrictive' parameter set whenever possible.
    
    The 'Less Restrictive' parameter set relaxes the guidelines on amplicon lengths (up to 150 bases) and a longer probe length (28 bases). The parameters demanding a close proximity between the forward primer and probe are also extended slightly to 12 bases.
    
    The 'Least Restrictive' parameter set permits an amplicon length of up to 200 bases, a long probe design (30 bases), and probes that may anneal up to 20 bases distant from the forward primer.
    
    All three parameter sets adhere to the dogma of dual-labeled probe design. Assays proposed to any one of the three are expected to work well.
  • 

    What does the 'Overall Rank' score in your RealTimeDesign™ software represent?

    RealTimeDesign™ presents all candidate primers, probes, and assays in order of descending rank score. The rank score represents how closely the design matches the ideal values for each parameter setting. This aggregate value is principally used by the software to advance those candidate oligos that are most optimal, to ultimately present a single assay that is the most highly ranked.

    Note: Every assay proposed by RealTimeDesign is expected to function regardless of the rank score. In other words, there is no threshold or cut-off ranking below which all assays will under-perform.
  • 

    What is the 'Failure Count Data' in your RealTimeDesign™ software?

    The RealTimeDesign™ (RTD™) software uses a variety of parameter settings (e.g. amplicon length, melting temperature and GC percentage) in order to design optimal primers and probes. An oligo candidate will fail the design process if it falls outside the minimum or maximum values for each parameter limitation. The 'Failure Count Data' indicates how many candidates failed for each particular parameter. Editing individual parameters can overcome a failed assay design by increasing the number of oligo candidates, but may not function satisfactory in qPCR.
  • 

    What is meant by 'Tandem Repeats' and 'Mask Tandems' when using the RealTimeDesign™ software?

    The 'Custom Mode' of the RealTimeDesign™ (RTD™) software will identify strings of a single base and short simple repeats within the input sequence. These features called ‘Tandem Repeats’ are automatically masked and avoided during assay design by converting the repeat bases into strings of N’s. By using Custom Mode the user may choose to unmask some or all of these repeat sequences and make them available for placement of the probes and primers. To unmask repeat sequences, expand the 'Features' window by clicking on the box for 'TandemRepeats' and select 'Unmask All' or choose specific tandem repeats to unmask.

• Troubleshooting:

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    I am performing real time qPCR and my negative controls are amplifying. Why would this happen?

    The most common reason negative controls come up positive is cross-contamination by a positive control such as a plasmid template. Below are a few suggestions to prevent contamination:
    
    1) Aliquot your probe and primers into small aliquots with enough product to run only a few experiments. Not only does this guard against contamination but will also help minimize the number of freeze/thaw cycles which degrade oligonucleotide quality.
    
    2) Use separate work areas for qPCR reagent preparation, DNA/template addition and amplification product handling.
    
    3) Clean qPCR work areas and pipettes (designated for qPCR use only) regularly with a DNA degradative agent and follow up with 70% ethanol.
    
    4) Use only sterile, filtered pipette tips to minimize aerosol contamination of the pipettes.
    
    5) If you continue to have trouble, consider using Uracil-N-Glycosylase (UNG) in your assay set up.
  • 

    Why do I get different Ct values for the same probe sequence when labeled with a different dye?

    It is not unusual to observe slightly different cycles to threshold (Ct or Cq) values for the same probe sequence labeled with different fluorophores. Such variation is typically on the order of 1 to 2 cycles and relates to the differences in dye intensity as well as the variation in instrument optics across the different channels. Fundamentally, all real-time thermal cyclers are engineered to detect fluorescein (FAM) first and foremost, so dyes with longer wavelength emission may be detected less sensitively. Occasionally, changing the fluorophore can have a profound impact on functional performance, particularly when the melting temperature of the probe is marginal. Such an outcome might relate to the hydrophobic attraction between modifications, or a change in melting temperature with the new fluorophore.
  • 

    Why is it that when a sequence contains a ‘wobble’ it has variable functionality?

    Incorporation of 'wobbles' into a sequence decreases the effective concentration of each species. With increased numbers of 'wobbles' the number of distinct species increases exponentially thereby decreasing the likelihood that any individual sequence has the desired specificity. Only one species is usually present in a biological sample. As some portion of the oligo species are not completely complementary to the target, some variability in function is to be expected. To further complicate matters, the individual nucleotide amidites can have different coupling rates. Each time the same 'wobble' sequence is synthesized, there is the potential that one species will be produced in preference over another.
    
    Tips:
    1) Be conservative. Introduce as few 'wobbles' as possible; one trinucleotide 'wobble' and one dinucleotide 'wobble' or two dinucleotide 'wobbles' in two different locations such that there is a maximum of 6 variants in a single oligonucleotide and;
    
    2) Increase the concentration of your 'wobble' sequence by as much as two fold to compensate for the presence of multiple unique sequences.
    
    If you have specific questions regarding minimum yields for a particular probe, please contact our Technical Support team.