- Research article
- Open Access
Reverse transcription quantitative real-time polymerase chain reaction reference genes in the spared nerve injury model of neuropathic pain: validation and literature search
BMC Research Notes volume 6, Article number: 266 (2013)
The reverse transcription quantitative real-time polymerase chain reaction (RT-qPCR) is a widely used, highly sensitive laboratory technique to rapidly and easily detect, identify and quantify gene expression. Reliable RT-qPCR data necessitates accurate normalization with validated control genes (reference genes) whose expression is constant in all studied conditions. This stability has to be demonstrated.
We performed a literature search for studies using quantitative or semi-quantitative PCR in the rat spared nerve injury (SNI) model of neuropathic pain to verify whether any reference genes had previously been validated. We then analyzed the stability over time of 7 commonly used reference genes in the nervous system – specifically in the spinal cord dorsal horn and the dorsal root ganglion (DRG). These were: Actin beta (Actb), Glyceraldehyde-3-phosphate dehydrogenase (GAPDH), ribosomal proteins 18S (18S), L13a (RPL13a) and L29 (RPL29), hypoxanthine phosphoribosyltransferase 1 (HPRT1) and hydroxymethylbilane synthase (HMBS). We compared the candidate genes and established a stability ranking using the geNorm algorithm. Finally, we assessed the number of reference genes necessary for accurate normalization in this neuropathic pain model.
We found GAPDH, HMBS, Actb, HPRT1 and 18S cited as reference genes in literature on studies using the SNI model. Only HPRT1 and 18S had been once previously demonstrated as stable in RT-qPCR arrays. All the genes tested in this study, using the geNorm algorithm, presented gene stability values (M-value) acceptable enough for them to qualify as potential reference genes in both DRG and spinal cord. Using the coefficient of variation, 18S failed the 50% cut-off with a value of 61% in the DRG. The two most stable genes in the dorsal horn were RPL29 and RPL13a; in the DRG they were HPRT1 and Actb. Using a 0.15 cut-off for pairwise variations we found that any pair of stable reference gene was sufficient for the normalization process.
In the rat SNI model, we validated and ranked Actb, RPL29, RPL13a, HMBS, GAPDH, HPRT1 and 18S as good reference genes in the spinal cord. In the DRG, 18S did not fulfill stability criteria. The combination of any two stable reference genes was sufficient to provide an accurate normalization.
While 20%-30% of the general populace are affected by chronic pain, a significant proportion, about 7%, experiences neuropathic pain characteristics[1, 2]. Defined by the International Association for the Study of Pain (IASP) as a pain “caused by a lesion or disease of the somatosensory nervous system”, neuropathic pain represents a daily challenge to medical practice and a worldwide public health problem since it is often refractory to treatment. Several animal models of neuropathic pain are used to study its different pathophysiological mechanisms and hopefully uncover new targets for treatment. Among them, the spared nerve injury (SNI) model represents an easy-to-perform and robust model of peripheral nerve injury. The axotomy of the tibial and peroneal branches of the sciatic nerve, sparing the sural nerve, allows a straightforward testing of the hind paw’s sural nerve territory for signs of hyperalgesia. After a peripheral nerve injury in rodents, numerous alterations in the somatosensory nervous system can be observed, which together lead to a hyperexcitability of the system. Besides changes affecting the primary nociceptors whose cell bodies are in the dorsal root ganglion (DRG) or the secondary neurons in the dorsal horn projecting into the brain, glial cells also react dramatically to a peripheral nerve injury like SNI. A common approach used to elucidate such changes in molecular machinery is to explore modifications in the expression of relevant genes[5, 6]. These variations can be detected and quantified in a sensitive, specific way using a reverse transcription quantitative real-time polymerase chain reaction (RT-qPCR), assuming that an accurate normalization has been performed with reference genes that have proved stable in all biological replicates and experimental conditions[7–10]. The recently published guidelines on the “minimum information for publication of quantitative real-time PCR experiments” (MIQE) strongly recommended the validation of reference genes used in different cell types and conditions. These guidelines outline the importance of RT-qPCR accuracy and recommend following detailed procedures to produce the most robust and reproducible RT-qPCR data.
Algorithms like geNorm or NormFinder were developed to help researchers assess candidate reference genes. GeNorm has been well described and widely accepted as a very useful tool for the normalization of RT-qPCR data. It measures the stability of potential reference genes by comparing their expression levels against one another. The expression ratio is supposed to be the same in all biological and technical replicates. This pairwise comparison permits the assessment and ranking of candidate reference genes and additionally demonstrates how many are necessary for an accurate normalization[9, 11]. To our knowledge, a validation of reference genes for the rat after spared nerve injury had never been published. We therefore performed a literature search for all studies using quantitative or semi-quantitative PCR in the SNI model and listed all the reference genes used. We then tested a total of 7 genes – including commonly used reference genes in the nervous system and those used in the SNI model – at different time points after nerve lesion in the spinal cord dorsal horn and in the DRG. These genes were Actin beta (Actb), Glyceraldehyde-3-phosphate dehydrogenase (GAPDH), ribosomal proteins 18S (18S), L13a (RPL13a) and L29 (RPL29), hypoxanthine phosphoribosyltransferase 1 (HPRT1) and hydroxymethylbilane synthase (HMBS)[12–15]. Selected genes were related to various metabolic pathways to avoid any co-regulation.
We carried out our experiments on Sprague–Dawley rats (Charles River, L’Abresle, France) weighing 250–300 grams. They were housed under 12 h day/night photoperiodic conditions, at a constant temperature and with free access to water and food. All procedures were approved by the Canton of Vaud’s Animal Experimentation Committee and were in accordance with the Swiss Federal Law on Animal Welfare and the IASP’s guidelines.
Rats were anesthetized with isoflurane 1.5%-2.5% (Abott, Baar, Switzerland) and surgical procedures were performed as previously described[3, 17]. Briefly, the left sciatic nerve was exposed at the mid-thigh level distal to the trifurcation, tibial and common peroneal branches were tightly ligated with 5.0 silk and axotomized, leaving the sural branch intact. Muscle and skin were closed in two layers and animals were allowed to recover. Three rats were sacrificed at 2, 4, 7, 10, 14 and 21 days after surgery.
We performed a literature search in the PubMed database using the keywords “spared nerve injury” and selected every study using semi-quantitative PCR or RT-qPCR in the rat SNI model (13 April 2013). We only selected articles in English. Reference genes used were noted, as were indications of their validation in the models.
RNA isolation and reverse transcription
Animals were transcardially perfused with NaCl 0.9% in order to expel the blood from collected tissue. Ipsilateral L4 and L5 DRG and spinal cord dorsal horn were rapidly dissected and immediately stored in RNAlater® (Qiagen, Switzerland) for stabilization at 4°C overnight, and then frozen at −80°C until processed. Samples were first homogenized with a POLYTRON® homogenizer and then total RNA was extracted using the RNeasy Plus Mini Kit (Qiagen). To ensure complete removal of gDNA, we treated the dorsal horn samples with a DNase (RNAqueous®-4PCR Kit, Ambion) and then the inactivation reagent recommended in the manufacturer’s instructions.
Nucleic acid purity was assessed measuring the A260/A280 ratio by spectrophotometer (NanoDrop). Total RNA integrity (RIN) and quantity were determined with an Agilent 2100 Bioanalyser (Agilent Technologies). RNA used had to have both a A260/A280 ratio between 1.8 and 2.1, as well as a RIN ≥8 for dorsal horn RNA extractions and ≥6.9 for DRG samples. The reverse transcription was achieved using Omniscript RT Kit (Qiagen), according to manufacturer’s instructions. All reactions took place for 1h at 37°C in a final volume of 40 μl containing 1 μg total RNA in the presence of 20 units RNase inhibitor (RNasin® Ribonuclease Inhibitor, Promega), 1 μg random hexamers (Microsynth), 4 μl 10× Buffer RT, 0.5 mM dNTPs and 8 units Omniscript reverse transcriptase (Omniscript RT Kit, Qiagen).
Selection of reference genes and primer design
Reference genes were chosen from those used previously in the SNI model. Other potentially suitable reference genes were selected among those used in published literature on the nervous system (Table 1). Whenever possible, primers fulfilled the following recommended criteria: amplicon length of 60 bp-150 bp, location of primers on two different exons, primer sequence length of 18 bp-25 bp, melting temperature of 60°C +/−1°C and GC content of 40%-60%[7, 18–20]. Primer specificity was checked in silico (Primer-BLAST Tool fromhttp://www.ncbi.nlm.nih.gov/tools/primer-blast/). All oligonucleotides were supplied unmodified and desalted (Microsynth AG, Switzerland).
Quantitative real-time PCR (qPCR)
We performed qPCR on an iQ5 Cycler (Bio-Rad) with SYBR Green I. The reactions were carried out in 96-well plates (Thermo-Fast® 96 Semi-Skirted PCR Plate, Thermo Scientific, Switzerland) each with a total volume of 20 μl. Each well contained 5 μl of a 100-fold dilution of cDNA, 10 μl of iQ™ Sybr® Green Supermix (2× qPCR mix contains dNTPs, 50 U/ml iTaq DNA polymerase, 6 mM MgCl2, SYBR Green I, enhancers, stabilizers, 20 nM fluorescein) (Bio-Rad, Switzerland), 2 μl of each primer 1–3 μM and 1 μl water. We optimized qPCR conditions on the iQ5 thermal gradient cycler and by testing different concentrations of primers and templates. The qPCR program began with an initial three-minute denaturation step at 95°C to activate the hot-start iTaq™ DNA polymerase. This was followed by 45 cycles of 10 s at 95°C for denaturation and 45 s at 60°C for annealing and extension.
We confirmed the amplification of specific qPCR products by performing a melting-curve step at the end of each run. Serial dilution curves for each primer allowed us to calculate qPCR efficiencies. The 100-fold diluted cDNA utilized for all the amplifications was within the linear dynamic range of the calibration curve – between 10 and 1000-fold dilution. Across all the assays, none of the quantification cycle (Cq) values was higher than 30. No-template and no-reverse transcription controls were run to determine any contamination or the generation of primer dimers. All amplifications were run in triplicate, and any doubtful curves were excluded. To minimize technical variation between samples through different runs we preferred the sample maximization method, i.e. a run contained all the samples for one gene of interest respective to one reference gene.
Raw data was collected and computed by iQ5 BioRad software with an automated analysis of the baseline and threshold of each run, and then exported in Excel files for further analyses. We rescaled all Cq values for each gene to the lowest Cq value as an internal control, converted these rescaled Cq logarithmically into linear, relative quantities taking into account the gene specific amplification efficiency [relative quantity = (1+efficiency) ^ (Cqinternal control-Cqsample)]. Finally, we calculated arithmetical means from the replicates[11, 24]. To explore the stability of each candidate gene we calculated M-values from the geNorm algorithm and coefficients of variation (CV)[9, 11]. The M-value corresponds to the average pairwise variation between a gene and the other candidate genes. The more this value tends to zero, the more stably the gene is expressed in comparison to the others. For a heterogeneous sample, a candidate gene with an M-value below 1 can be considered as a reliable reference gene. The CV for a gene was obtained by calculating the ratio of the standard deviation (σ) to the mean (μ) of relative quantities (CV = σ / μ). For a heterogeneous panel, a value below 50% is proposed as satisfactory.
To rank the genes that satisfied the above criteria, M-values were recalculated after stepwise elimination of the worst candidate. To assess the number of reference genes needed for an accurate normalization, the effect of inclusion of a supplementary gene to those already considered stable was determined by calculating the pairwise variation of the added candidate gene to the others (standard deviation of logarithmically transformed expression ratios). If this pairwise variation goes below 0.15, no supplementary gene is needed.
Reference genes used in the SNI model
We found 484 articles in the PubMed database using “spared nerve injury” as keywords. Twenty-six articles were retrieved with semi-quantitative PCR or RT-qPCR performed in the rat DRG, spinal cord or brain. Despite its rigorous validation never having been mentioned, GAPDH was the most commonly used reference gene (16 times) whether in the DRG or in the dorsal horn. This was followed by Actb and 18S (3 times), HPRT1 (twice) and HMBS (once). HPRT1 and 18S were the only two reference genes with validation in the rat SNI model (Table 2).
Validation of reference genes in spinal cord dorsal horn over time after SNI
Rat spinal cord dorsal horn samples were analyzed in an overall panel without differentiating any timepoints, i.e. throughout a temporal follow-up with naive animals, 2nd, 4th, 7th, 10th, 14th and 21st postoperative day animals. The pairwise comparison of all the potential reference genes (Actb, 18S, GAPDH, RPL13a, RPL29, HPRT1 and HMBS) calculated using geNorm resulted in M-values below 0.5 for all but the 18S gene, which showed 0.52 (Figure 1). All genes were below the M-value cut-off of 1.0 proposed for a heterogeneous panel. CV ranged from 20% for HMBS to 34% for GAPDH and RPL13a, i.e. below the 50% cut-off for stability in a heterogeneous panel.
Validation of reference genes in DRG after SNI in a time-dependent panel
As for the dorsal horn, DRG samples were analyzed in an overall panel without differentiating any timepoints. M-values were below 1.0 and CV below 50% for Actb, GAPDH, RPL13a, RPL29, HPRT1 and HMBS. The 18S reference gene had the worst M-value, at 0.8, but this was still acceptable within the selection. However, we rejected it from our gene sample because of its 61% CV (Figure 1).
Ranking of reference genes
We reanalyzed the 7 tested reference genes (Actb, GAPDH, RPL13a, RPL29, HPRT1, HMBS and 18S) to rank them. After each step, the gene with the highest M-value was eliminated until we obtained the two most stable genes from the list. No further discrimination was possible.
In the spinal cord dorsal horn, the 2 most stable genes remaining after the stepwise elimination were RPL29 and RPL13a, and then in increasing order GAPDH, Actb, HMBS, HPRT1 and 18S (Figure 2A).
In the DRG, the 2 most stable genes remaining after the stepwise elimination were HPRT1 and Actb, and then in increasing order RPL29, RPL13a, HMBS, GAPDH and 18S (Figure 2B). The latter is used because this ranking only takes into account the M-value and not the CV.
Minimal number of reference genes
In the dorsal horn samples, the calculation of pairwise variations resulted in values much lower than 0.15 along the entire time course and in all samples. Using the two best reference genes the pairwise variation in dorsal horn was 0.07 (Figure 3). The addition of a supplementary reference gene did not significantly lower the pairwise variation. Results for DRG were similar, with a low pairwise variation of 0.05 if only the two most stable reference genes were taken in consideration.
We performed the same analysis using the least stable reference genes on our list for dorsal horn and DRG, and their pairwise variation was still below 0.15.
Here, we tested the stability of seven candidate reference genes according to the geNorm algorithm to ensure accurate RT-qPCR normalization. M-values below 1.0 together with CV lower than 50% for Actb, GAPDH, RPL13a, RPL29, HPRT1, and HMBS identified these candidate genes as good controls in the rat SNI model in the spinal cord dorsal horn and DRG. The 18S gene could not be validated in DRG because of a CV above 50%.
After SNI, gene expression changes in both sites can be enormous compared to the baseline and also over time. Because of this heterogeneity, meticulous RT-qPCR procedures relying on MIQE recommendations are essential to obtain consistent data. The most frequently chosen reference gene for RT-qPCR normalization after SNI in the rat is GAPDH, but its expression level had, to our knowledge, never been confirmed as being stable in this model (Table 2). Here, we confirm that GAPDH is a good candidate gene, even if it is not the most stable in our series.
The only 2 reference genes with previously mentioned validation in the rat SNI model are HPRT1 and 18S. HPRT1 was used by Shankarappa et al. in DRG at 2 timepoints after injury and chosen from among 5 different reference genes on an array. After showing that 18S had a very low variation of Cq values in all data sets, from both SNI and naive groups, Staaf et al. used it to normalize and compare the expression of the transient receptor potential (TRP) family of genes in DRG after SNI. They mentioned neither ranking between the different reference genes, nor the criteria used to choose 18S from among their list of them. These demonstrations are part of the workflow of RT-qPCR arrays where several reference genes are proposed, and their analysis is usually fully integrated in the procedure.
GeNorm is a popular algorithm for assessing different reference genes from a given panel[9, 11]. The calculation of M-values permits measurement of an average variation in the expression ratios of one potential reference gene with the others and consequently informs us whether the tested gene is constantly expressed compared to them. The CV of relative quantities of a gene merely reflects the dispersion of its expression level. It has been previously demonstrated that a CV below 25% was typically observed in stable reference genes as long as the experimental conditions were homogeneous. In a heterogeneous panel, such as in the present study, a CV below 50% is acceptable. As it measures the gene-specific variation, the CV in assessing the stability of a reference gene assumes a standardization of the procedures for all samples. Taken together, M-values and the CV are very useful tools for determining the most accurate reference genes because the information that they convey is different. All our candidate genes satisfied an M-value cut-off below 1.0 for a heterogeneous panel. 18S, despite its acceptable M-value, failed to satisfy the CV cut-off in DRG. Considering these results 18S could not be validated as a stable reference gene.
The more the M-value tends to zero, the more the candidate gene is stable compared to the other tested genes. Hence the stability of the different genes can be ranked. A first approximate classification was established after analyzing all the samples together (Figure 1). Actb, RPL13a and RPL29 were the 3 best genes in both tissues. A potentially more accurate classification can be performed if M-values are recalculated in a series of steps, after elimination of the worst scoring gene at each step. At the end, the two most reliable reference genes remain, but they cannot be further discriminated by definition of the M-value (Figure 2). Interestingly the ranking differed between dorsal horn and DRG. We again found RPL 29 and RPL13a to be the most stable genes in the spinal cord dorsal horn, however, in the DRG, HPRT1 and Actb were the best, followed immediately by RPL13a and RPL29. In the present study, differences in the ranking were very slight, and the former “rough” method would have been sufficient. In other circumstances, or with another panel of candidate genes, it could be useful to compare them further until a definitive ranking is obtained, so as to choose only the best control genes from amongst the candidates. M-value calculations and subsequent ranking were also performed independently for each different time point (data not shown) without being able to identify any time-dependent regulation. The primary goal of this study was to validate some suitable RT-qPCR reference genes at different time points, in different tissues, in a widely used neuropathic pain model.
According to MIQE guidelines, the use of a single reference gene is not enough to compensate for the intrinsic variation within that reference gene and normalization against several reference genes should be performed[7, 9]. To define the minimal number of necessary reference genes, the pairwise variation permits an assessment of whether the removal of the worst reference gene may result in a greater variation (Figure 3). Here, in both DRG and dorsal horn, the two best candidate genes were sufficient to ensure an accurate normalization. This demonstration allows us to state that in our model, using only the two best reference genes would be sufficient: namely RPL 29 and RPL13a in the spinal cord dorsal horn and HPRT1 and Actb in the DRG. However, even the worst pair satisfied stability criteria, with a pairwise variation less than 0.15. In fact, all pairs of validated reference genes (not 18S because of its CV above 50%) provided a robust validation in both tissues and at all time points. GAPDH is often used, but according to MIQE guidelines it should not be used alone.
The criterion for choosing a reference gene is more than just its stability. 18S, for example, is disputed as a reference gene by some authors who argue that it by far exceeds the mRNA quantity of most genes of interest and it might be absent from pure mRNA extracts.
We validated 7 reference genes in the spinal cord dorsal horn: (Actin beta (Actb), Glyceraldehyde-3-phosphate dehydrogenase (GAPDH), ribosomal proteins L13a (RPL13a) and L29 (RPL29), hypoxanthine phosphoribosyltransferase 1 (HPRT1), hydroxymethylbilane synthase (HMBS) and 18S. In DRG, 18S did not fulfill all our criteria and could not be retained as a good reference gene, although the other 6 were. We were able to show that in both tissues, using any two of the proposed stable reference genes is sufficient to ensure an accurate validation. We were also able to confirm the stability of GAPDH, which is the most commonly used reference gene in the SNI model, but it should be used in combination with another control gene.
Availability of supporting data
The data sets supporting this article’s results are available in the Labarchives repository underhttp://dx.doi.org/10.6070/H4CZ3532.
Bouhassira D, Lanteri-Minet M, Attal N, Laurent B, Touboul C: Prevalence of chronic pain with neuropathic characteristics in the general population. Pain. 2008, 136 (3): 380-387. 10.1016/j.pain.2007.08.013.
Breivik H, Collett B, Ventafridda V, Cohen R, Gallacher D: Survey of chronic pain in europe: prevalence, impact on daily life, and treatment. Eur J Pain. 2006, 10 (4): 287-333. 10.1016/j.ejpain.2005.06.009.
Decosterd I, Woolf CJ: Spared nerve injury: an animal model of persistent peripheral neuropathic pain. Pain. 2000, 87 (2): 149-158. 10.1016/S0304-3959(00)00276-1.
Basbaum AI, Bautista DM, Scherrer G, Julius D: Cellular and molecular mechanisms of pain. Cell. 2009, 139 (2): 267-284. 10.1016/j.cell.2009.09.028.
Costigan M, Befort K, Karchewski L, Griffin RS, D'Urso D, Allchorne A, Sitarski J, Mannion JW, Pratt RE, Woolf CJ: Replicate high-density rat genome oligonucleotide microarrays reveal hundreds of regulated genes in the dorsal root ganglion after peripheral nerve injury. BMC Neurosci. 2002, 3: 16-10.1186/1471-2202-3-16.
Spofford CM, Brennan TJ: Gene expression in skin, muscle, and dorsal root ganglion after plantar incision in the rat. Anesthesiology. 2012, 117 (1): 161-172. 10.1097/ALN.0b013e31825a2a2b.
Bustin SA, Benes V, Garson JA, Hellemans J, Huggett J, Kubista M, Mueller R, Nolan T, Pfaffl MW, Shipley GL, Vandesompele J, Wittwer CT: The MIQE guidelines: minimum information for publication of quantitative real-time PCR experiments. Clin Chem. 2009, 55 (4): 611-622. 10.1373/clinchem.2008.112797.
Taylor S, Wakem M, Dijkman G, Alsarraj M, Nguyen M: A practical approach to RT-qPCR-publishing data that conform to the MIQE guidelines. Methods. 2010, 50 (4): S1-S5. 10.1016/j.ymeth.2010.01.005.
Vandesompele J, De Preter K, Pattyn F, Poppe B, Van Roy N, De Paepe A, Speleman F: Accurate normalization of real-time quantitative RT-PCR data by geometric averaging of multiple internal control genes. Genome Biol. 2002, 3 (7): research0034.1-0034.11
Pfaffl MW, Tichopad A, Prgomet C, Neuvians TP: Determination of stable housekeeping genes, differentially regulated target genes and sample integrity: bestkeeper–excel-based tool using pair-wise correlations. Biotechnol Lett. 2004, 26 (6): 509-515.
Hellemans J, Mortier G, De Paepe A, Speleman F, Vandesompele J: QBase relative quantification framework and software for management and automated analysis of real-time quantitative PCR data. Genome Biol. 2007, 8 (2): R19-10.1186/gb-2007-8-2-r19.
Gubern C, Hurtado O, Rodriguez R, Morales JR, Romera VG, Moro MA, Lizasoain I, Serena J, Mallolas J: Validation of housekeeping genes for quantitative real-time PCR in in-vivo and in-vitro models of cerebral ischaemia. BMC Mol Biol. 2009, 10: 57-10.1186/1471-2199-10-57.
Nelissen K, Smeets K, Mulder M, Hendriks JJ, Ameloot M: Selection of reference genes for gene expression studies in rat oligodendrocytes using quantitative real time PCR. J Neurosci Methods. 2010, 187 (1): 78-83. 10.1016/j.jneumeth.2009.12.018.
Yao L, Chen X, Tian Y, Lu H, Zhang P, Shi Q, Zhang J, Liu Y: Selection of housekeeping genes for normalization of RT-PCR in hypoxic neural stem cells of rat in vitro. Mol Biol Rep. 2012, 39 (1): 569-576. 10.1007/s11033-011-0772-8.
Wan G, Yang K, Lim Q, Zhou L, He BP, Wong HK, Too HP: Identification and validation of reference genes for expression studies in a rat model of neuropathic pain. Biochem Biophys Res Commun. 2010, 400 (4): 575-580. 10.1016/j.bbrc.2010.08.106.
Zimmermann M: Ethical guidelines for investigations of experimental pain in conscious animals. Pain. 1983, 16 (2): 109-110. 10.1016/0304-3959(83)90201-4.
Pertin M, Gosselin RD, Decosterd I: The spared nerve injury model of neuropathic pain. Methods Mol Biol. 2012, 851: 205-212. 10.1007/978-1-61779-561-9_15.
Udvardi MK, Czechowski T, Scheible WR: Eleven golden rules of quantitative RT-PCR. Plant Cell. 2008, 20 (7): 1736-1737. 10.1105/tpc.108.061143.
Kubista M, Andrade JM, Bengtsson M, Forootan A, Jonak J, Lind K, Sindelka R, Sjoback R, Sjogreen B, Strombom L, Ståhlberg A, Zoric N: The real-time polymerase chain reaction. Mol Aspects Med. 2006, 27 (2–3): 95-125.
Dieffenbach CW, Lowe TM, Dveksler GS: General concepts for PCR primer design. PCR Methods Appl. 1993, 3 (3): S30-S37. 10.1101/gr.3.3.S30.
Ye J, Coulouris G, Zaretskaya I, Cutcutache I, Rozen S, Madden TL: Primer-BLAST: a tool to design target-specific primers for polymerase chain reaction. BMC Bioinforma. 2012, 13: 134-10.1186/1471-2105-13-134.
Proudnikov D, Yuferov V, LaForge KS, Ho A, Jeanne Kreek M: Quantification of multiple mRNA levels in rat brain regions using real time optical PCR. Brain Res Mol Brain Res. 2003, 112 (1–2): 182-185.
Tanga FY, Raghavendra V, DeLeo JA: Quantitative real-time RT-PCR assessment of spinal microglial and astrocytic activation markers in a rat model of neuropathic pain. Neurochem Int. 2004, 45 (2–3): 397-
Pfaffl MW: A new mathematical model for relative quantification in real-time RT-PCR. Nucleic Acids Res. 2001, 29 (9): e45-10.1093/nar/29.9.e45.
Kanda H, Kobayashi K, Yamanaka H, Noguchi K: COX-1-dependent prostaglandin D2 in microglia contributes to neuropathic pain via DP2 receptor in spinal neurons. Glia. 2013, 61 (6): 943-956. 10.1002/glia.22487.
Zhou J, Yang CX, Zhong JY, Wang HB: Intrathecal TRESK gene recombinant adenovirus attenuates spared nerve injury-induced neuropathic pain in rats. Neuroreport. 2013, 24 (3): 131-136. 10.1097/WNR.0b013e32835d8431.
Kashimoto R, Yamanaka H, Kobayashi K, Okubo M, Yagi H, Mimura O, Noguchi K: Phosphorylation of ezrin/radixin/moesin (ERM) protein in spinal microglia following peripheral nerve injury and lysophosphatidic acid administration. Glia. 2013, 61 (3): 338-348. 10.1002/glia.22436.
Shankarappa SA, Tsui JH, Kim KN, Reznor G, Dohlman JC, Langer R, Kohane DS: Prolonged nerve blockade delays the onset of neuropathic pain. Proc Natl Acad Sci USA. 2012, 109 (43): 17555-17560. 10.1073/pnas.1214634109.
Inquimbert P, Bartels K, Babaniyi OB, Barrett LB, Tegeder I, Scholz J: Peripheral nerve injury produces a sustained shift in the balance between glutamate release and uptake in the dorsal horn of the spinal cord. Pain. 2012, 153 (12): 2422-2431. 10.1016/j.pain.2012.08.011.
Zapata A, Pontis S, Schepers RJ, Wang R, Oh E, Stein A, Backman CM, Worley P, Enguita M, Abad MA, Trullas R, Shippenberg TS: Alleviation of neuropathic pain hypersensitivity by inhibiting neuronal pentraxin 1 in the rostral ventromedial medulla. J NeuroSci. 2012, 32 (36): 12431-12436. 10.1523/JNEUROSCI.2730-12.2012.
Samad OA, Tan AM, Cheng X, Foster E, Dib-Hajj SD, Waxman SG: Virus-mediated shRNA knockdown of Na(v)1.3 In Rat dorsal root ganglion attenuates nerve injury-induced neuropathic pain. Mol Ther. 2013, 21 (1): 49-56. 10.1038/mt.2012.169.
Kobayashi K, Yamanaka H, Yanamoto F, Okubo M, Noguchi K: Multiple P2Y subtypes in spinal microglia are involved in neuropathic pain after peripheral nerve injury. Glia. 2012, 60 (10): 1529-1539. 10.1002/glia.22373.
Liu M, Zhou L, Chen Z, Hu C: Analgesic effect of iridoid glycosides from paederia scandens (LOUR.) MERRILL (rubiaceae) on spared nerve injury rat model of neuropathic pain. Pharmacol Biochem Behav. 2012, 102 (3): 465-470. 10.1016/j.pbb.2012.06.007.
Tochiki KK, Cunningham J, Hunt SP, Geranton SM: The expression of spinal methyl-CpG-binding protein 2, DNA methyltransferases and histone deacetylases is modulated in persistent pain states. Mol Pain. 2012, 8: 14-10.1186/1744-8069-8-14.
Okubo M, Yamanaka H, Kobayashi K, Kanda H, Dai Y, Noguchi K: Up-regulation of platelet-activating factor synthases and its receptor in spinal cord contribute to development of neuropathic pain following peripheral nerve injury. Mol Pain. 2012, 8: 8-10.1186/1744-8069-8-8.
del Rey A, Yau HJ, Randolf A, Centeno MV, Wildmann J, Martina M, Besedovsky HO, Apkarian AV: Chronic neuropathic pain-like behavior correlates with IL-1beta expression and disrupts cytokine interactions in the hippocampus. Pain. 2011, 152 (12): 2827-2835. 10.1016/j.pain.2011.09.013.
Kuhlein HN, Tegeder I, Moser C, Lim HY, Haussler A, Spieth K, Jennes I, Marschalek R, Beckhaus T, Karas M, Fauth M, Ehnert C, Geisslinger G, Niederberger E: Nerve injury evoked loss of latexin expression in spinal cord neurons contributes to the development of neuropathic pain. PLoS One. 2011, 6 (4): e19270-10.1371/journal.pone.0019270.
Yamanaka H, Kobayashi K, Okubo M, Fukuoka T, Noguchi K: Increase of close homolog of cell adhesion molecule L1 in primary afferent by nerve injury and the contribution to neuropathic pain. J Comp Neurol. 2011, 519 (8): 1597-1615. 10.1002/cne.22588.
de Novellis V, Vita D, Gatta L, Luongo L, Bellini G, De Chiaro M, Marabese I, Siniscalco D, Boccella S, Piscitelli F, Di Marzo V, Palazzo E, Rossi F, Maione S: The blockade of the transient receptor potential vanilloid type 1 and fatty acid amide hydrolase decreases symptoms and central sequelae in the medial prefrontal cortex of neuropathic rats. Mol Pain. 2011, 7: 7-10.1186/1744-8069-7-7.
Vega-Avelaira D, Geranton SM, Fitzgerald M: Differential regulation of immune responses and macrophage/neuron interactions in the dorsal root ganglion in young and adult rats following nerve injury. Mol Pain. 2009, 5: 70-10.1186/1744-8069-5-70.
Costigan M, Moss A, Latremoliere A, Johnston C, Verma-Gandhu M, Herbert TA, Barrett L, Brenner GJ, Vardeh D, Woolf CJ, Fitzgerald M: T-cell infiltration and signaling in the adult dorsal spinal cord is a major contributor to neuropathic pain-like hypersensitivity. J Neurosci. 2009, 29 (46): 14415-14422. 10.1523/JNEUROSCI.4569-09.2009.
Okubo M, Yamanaka H, Kobayashi K, Noguchi K: Leukotriene synthases and the receptors induced by peripheral nerve injury in the spinal cord contribute to the generation of neuropathic pain. Glia. 2010, 58 (5): 599-610.
Staaf S, Oerther S, Lucas G, Mattsson JP, Ernfors P: Differential regulation of TRP channels in a rat model of neuropathic pain. Pain. 2009, 144 (1–2): 187-199.
Moss A, Ingram R, Koch S, Theodorou A, Low L, Baccei M, Hathway GJ, Costigan M, Salton SR, Fitzgerald M: Origins, actions and dynamic expression patterns of the neuropeptide VGF in rat peripheral and central sensory neurones following peripheral nerve injury. Mol Pain. 2008, 4: 62-10.1186/1744-8069-4-62.
Berta T, Poirot O, Pertin M, Ji RR, Kellenberger S, Decosterd I: Transcriptional and functional profiles of voltage-gated Na(+) channels in injured and non-injured DRG neurons in the SNI model of neuropathic pain. Mol Cell Neurosci. 2008, 37 (2): 196-208. 10.1016/j.mcn.2007.09.007.
Millecamps M, Centeno MV, Berra HH, Rudick CN, Lavarello S, Tkatch T, Apkarian AV: D-cycloserine reduces neuropathic pain behavior through limbic NMDA-mediated circuitry. Pain. 2007, 132 (1–2): 108-123.
Moss A, Beggs S, Vega-Avelaira D, Costigan M, Hathway GJ, Salter MW, Fitzgerald M: Spinal microglia and neuropathic pain in young rats. Pain. 2007, 128 (3): 215-224. 10.1016/j.pain.2006.09.018.
Apkarian AV, Lavarello S, Randolf A, Berra HH, Chialvo DR, Besedovsky HO, del Rey A: Expression of IL-1beta in supraspinal brain regions in rats with neuropathic pain. Neurosci Lett. 2006, 407 (2): 176-181. 10.1016/j.neulet.2006.08.034.
Pertin M, Ji RR, Berta T, Powell AJ, Karchewski L, Tate SN, Isom LL, Woolf CJ, Gilliard N, Spahn DR, Decosterd I: Upregulation of the voltage-gated sodium channel beta2 subunit in neuropathic pain models: characterization of expression in injured and non-injured primary sensory neurons. J Neurosci. 2005, 25 (47): 10970-10980. 10.1523/JNEUROSCI.3066-05.2005.
Takahashi N, Kikuchi S, Dai Y, Kobayashi K, Fukuoka T, Noguchi K: Expression of auxiliary beta subunits of sodium channels in primary afferent neurons and the effect of nerve injury. Neuroscience. 2003, 121 (2): 441-450. 10.1016/S0306-4522(03)00432-9.
Scholz J, Abele A, Marian C, Haussler A, Herbert TA, Woolf CJ, Tegeder I: Low-dose methotrexate reduces peripheral nerve injury-evoked spinal microglial activation and neuropathic pain behavior in rats. Pain. 2008, 138 (1): 130-142. 10.1016/j.pain.2007.11.019.
This study is supported by the Swiss National Science Foundation grants 310030A_124996 (ID) and 33CM30-124117 (MRS and ID), the 2011 IASP Early Career Grant funded by the ScanDesign Foundation BY INGER & JENS BRUUN (MRS) and the Swiss Society of Anesthesiology (MRS).
The authors declare that they have no competing interests.
NP performed the surgeries, the tissue extraction, the RT-qPCR, the literature search, the statistical analysis and drafted the manuscript. ID participated in the study design and in the drafting of the manuscript. MRS conceived the study, participated in its design and coordination and supervised the drafting of the manuscript. All authors read and approved the final manuscript.
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Piller, N., Decosterd, I. & Suter, M.R. Reverse transcription quantitative real-time polymerase chain reaction reference genes in the spared nerve injury model of neuropathic pain: validation and literature search. BMC Res Notes 6, 266 (2013). https://doi.org/10.1186/1756-0500-6-266
- Neuropathic pain
- Spared nerve injury
- Reference gene