Phloem small RNAs, nutrient stress responses, and systemic mobility
© Buhtz et al; licensee BioMed Central Ltd. 2010
Received: 31 July 2009
Accepted: 13 April 2010
Published: 13 April 2010
Nutrient availabilities and needs have to be tightly coordinated between organs to ensure a balance between uptake and consumption for metabolism, growth, and defense reactions. Since plants often have to grow in environments with sub-optimal nutrient availability, a fine tuning is vital. To achieve this, information has to flow cell-to-cell and over long-distance via xylem and phloem. Recently, specific miRNAs emerged as a new type of regulating molecules during stress and nutrient deficiency responses, and miR399 was suggested to be a phloem-mobile long-distance signal involved in the phosphate starvation response.
We used miRNA microarrays containing all known plant miRNAs and a set of unknown small (s) RNAs earlier cloned from Brassica phloem sap , to comprehensively analyze the phloem response to nutrient deficiency by removing sulfate, copper or iron, respectively, from the growth medium. We show that phloem sap contains a specific set of sRNAs that is distinct from leaves and roots, and that the phloem also responds specifically to stress. Upon S and Cu deficiencies phloem sap reacts with an increase of the same miRNAs that were earlier characterized in other tissues, while no clear positive response to -Fe was observed. However, -Fe led to a reduction of Cu- and P-responsive miRNAs. We further demonstrate that under nutrient starvation miR399 and miR395 can be translocated through graft unions from wild type scions to rootstocks of the miRNA processing hen1-1 mutant. In contrast, miR171 was not transported. Translocation of miR395 led to a down-regulation of one of its targets in rootstocks, suggesting that this transport is of functional relevance, and that miR395, in addition to the well characterized miR399, could potentially act as a long-distance information transmitter.
Phloem sap contains a specific set of sRNAs, of which some specifically accumulate in response to nutrient deprivation. From the observation that miR395 and miR399 are phloem-mobile in grafting experiments we conclude that translocatable miRNAs might be candidates for information-transmitting molecules, but that grafting experiments alone are not sufficient to convincingly assign a signaling function.
The levels of essential inorganic nutrients have to be tightly controlled inside individual cells and organs, but information about nutrient uptake and needs also have to be transferred between organs to optimize nutrient allocation, especially in plants growing under sub-optimal conditions. If an organ experiences nutrient starvation, it needs to communicate its requirements to the other organs in order to increase nutrient uptake or reallocate resources. This type of communication is probably mediated via the phloem. Recent work showed that microRNA (miRNA) 399 is potentially involved in long-distance communication via the phloem following phosphate deprivation [1–3]. miRNAs are short (21-24 nt), non-translated RNAs that are processed by Dicer-like proteins from large, characteristically folded precursor molecules. The majority of plant miRNAs target transcription factors and is therefore thought to mainly regulate developmental processes. However, recent studies have also identified miRNAs that are involved in responses to nutrient deficiencies. As mentioned earlier, miR399 is strongly induced during phosphate deprivation [4–7], while miR395 drastically increases under growth on low sulfur . In addition to macronutrients like sulfur and phosphate, also a lack of the micronutrient copper leads to an accumulation of miR397, 398, 408, and 857 [9–11]. miRNAs 395, 398 and 399 were recently shown to accumulate not only on the whole plant level, but also strongly within the phloem . Since sRNAs accumulating in phloem sap under stress could represent potential long-distance signaling molecules, we used sRNA microarrays from LC Sciences to comprehensively analyze phloem sRNAs. The customized arrays contained, in addition to all known plant miRNAs, a subset of small RNAs (sRNAs) of unknown function that was earlier sequenced from phloem sap of Brassica napus . First we established the miRNA patterns of phloem, leaves and roots of fully nutrient supplied, hydroponically grown oilseed rape plants to subsequently identify candidates that respond to growth under S, Cu or Fe deficiency, respectively. In addition, we used the highly -S induced miR395 as an example to examine whether this specific miRNA can be transported over graft unions when combining WT Arabidopsis with the miRNA biosynthesis mutant hen1-1. The specific aims were 1) to find phloem- and organ-enriched miRNAs, 2) to identify additional miRNAs that respond to S and Cu deficiencies, 3) to examine whether any miRNAs respond to Fe starvation, and 4) to demonstrate whether miR395 is phloem mobile or not.
Results and Discussion
Phloem sap shows a specific sRNA pattern that is distinct from that of inflorescence stem, leaves and roots
To ensure that the sRNAs observed in phloem sap were not resulting from contamination during sampling, and in order to identify phloem-enriched sRNAs, we performed a microarray hybridization experiment comparing phloem sap to the surrounding inflorescence stem tissue. This resulted in the identification of phloem-enriched sRNAs, while others were less abundant in phloem sap than in stem tissue (including phloem) collected after phloem sampling from the sampling site. Signal values for one miRNA per family are depicted in additional file 1. The distribution of ten miRNAs was re-evaluated by RNA gel blots from an independent set of plants, what confirmed the microarray results. miRNAs 162, 167, 168, 169, and 399 strongly accumulated in phloem samples as compared to inflorescence stem samples, while miR158, 396 and 397 were stem-enriched. This indicates that phloem samples are not significantly contaminated by the contents of the surrounding inflorescence stem cells, what had already previously been demonstrated [1, 12]. The observation that miR167 accumulates in phloem sap confirms an earlier study in pumpkin that found miR167 20-fold enriched in phloem sap as compared to the surrounding vascular tissue . Also the failure to detect miR171 in phloem sap and its low expression in stem samples is in accordance with earlier findings [13, 14].
Except for miR390, these miRNAs were also phloem-enriched as compared to inflorescence stem tissue (additional file 1). miRNAs from the families 156, 159, 160, 162, 164, 165, 166, 167, 393, 394, 396 and 403 were less abundant in the phloem as compared to both, leaves and roots. However, some of these miRNAs (159, 162, and 167) were more abundant in the phloem than in the surrounding stem.
miRNAs from the complete 156, 160, 166, 393, 396, and 528 families were found to be significantly enriched in roots as compared to leaves and phloem. In rice, miRNAs 156 and 166 have earlier been shown occur at higher levels in roots than in leaves . In addition, miR166 has been described to be expressed in roots of Medicago truncatula, where it functions in root and nodule development . In Arabidopsis, miRNAs 156 and 160 occur root-enriched , and miR160 has been implicated with root development [21, 22].
miR391 was the only miRNA that accumulated in leaves as compared to roots and phloem sap (figure 1). In an earlier study, miR391 was found to appear preferentially in rosette leaves of Arabidopsis, as compared to seedlings, flowers and siliques . According to the same publication, miR391 targets a beta-fructofuranosidase, but its function is currently not well understood. Although miR391 is regarded as being related to miR390, differing in only 5 nt , both miRNAs showed a quite distinct organ distribution: while miR391 was clearly leaf-enriched, miR390 was slightly, but significantly phloem-enriched, indicating that both miRNAs might still have distinct localizations and functions.
Phloem small RNA patterns change under nutrient deficiency
Since three miRNAs, miR395, 398 and 399, had been previously shown to accumulate in the phloem under the corresponding nutrient stress conditions , we intended to identify additional nutrient-responsive phloem sRNAs. They could represent novel information transmitters during nutrient deprivation, as has been suggested for miR399 under phosphate deficiency . To induce nutrient deprivation, we raised Brassica napus plants in hydroponic cultures under FN and omitted the respective nutrient from the medium for two (-S, -Cu experiments) or three weeks (-Fe experiment), respectively, before samples were collected. Under -S and -Cu conditions the plants did not show any obvious stress symptoms at the time of sampling. However, omitting Fe led to chlorosis symptoms in very young upper leaves after 4-5 days of stress (data not shown).
Initial analysis of the expression of selected genes that are known to be altered by the respective nutrient stress clearly confirmed that the plants were nutrient deficient in all three kinds of stress experiments performed (additional file 3). As expected, S starvation led to an increase in the expression of the two high-affinity sulfate transporters st1 (AJ416460) and st2 (AJ311388), especially in roots. Copper deprivation was confirmed by a slight decrease in the amount of Cu-Zn SOD transcripts, while the amount of the high-affinity copper transporter COPT1 increased markedly. Fe deprived plants showed only a slight reduction in the expression of the iron storage protein ferritin LSC30 in leaves and roots, accompanied by an increase in the transcript of the root-specific iron transporter IRT1 in roots (additional file 3).
Subsequently, material from the same batch of plants was used for dual-color microarray hybridizations of stressed and FN samples. Since only one array per stress experiment was hybridized, we applied specific criteria to only identify the most drastic positive changes (>four-fold increases, log2 >2) upon stress treatments and furthermore restricted the analyses to abundant sRNAs with signal intensities of >100 in one of the two (FN or stressed) samples.
Under iron deficiency only miR158 increased in the phloem more than four-fold (ath-miR158a increased from 231 to 1201), what was verified by sqRT-PCR in an independent experiment (inset in figure 3). miR158 was described as a non-conserved miRNA from Arabidopsis that could, for example, not be detected in citrus . miR158 is predicted to target a pentatricopeptide repeat-containing protein of unknown function, a lipase, and xyloglucan-fucosyl transferases . None of these potential targets has an obvious connection to iron uptake or metabolism, and thus the increase of miR158 might be a secondary effect on plant development. Moreover, the accumulation of miR158 seemed to be phloem sap-specific, as it could not be observed in leaf or root samples (see data submitted to GEO, series accession number GSE20263). Comparative high-throughput sequencing of FN and -Fe samples would help to clarify if an as yet unknown (and therefore not represented on the chip) sRNA increases under -Fe, or if there is really no small RNA accumulating during this deprivation response.
Interestingly, however, miRNAs 397, 398, 399, 408 and 2111 notably decreased during iron starvation, showing an opposite response to their increases observed under -Cu (figure 3, figure 4). This response was verified for miR398, 399, 408 and 2111 by sqRT-PCR from a set of independently grown plants (inset in figure 3). Decreases in the levels of -Cu-responsive miRNAs were visible not only in the phloem, but also in leaves and comparably weak in roots (figure 4). A decrease of these Cu starvation-responsive miRNAs suggests that copper uptake is stimulated by iron deficiency, as has already been observed in Brassica and other plant species [29, 30]. The need for higher Cu uptake under -Fe could be explained by the fact that many iron and copper-containing enzymes can substitute for each other when one of the two elements is present at suboptimal levels, e.g. SODs, cytochrome oxidase, or diiron oxidase [31, 32].
Interestingly, a phloem response opposite to the -Cu reaction under -Fe was also observed for the -P-responsive miRNAs 399 and 2111, which were more than two- (399), respectively more than four-fold (2111) decreased. The responses of miR399 and miR2111 were undetectable in leaves and roots (figure 4). This confirms the observation from a previous study that demonstrated that miR399 responds stronger to -P in phloem sap than in leaves and roots . The decrease of -P-responsive miRNAs in phloem sap suggests that Fe deficiency positively influences P uptake and metabolism, what has already been demonstrated in earlier studies e.g. [33, 34]. The other way around, high Fe can lead to lower P concentrations in the plant . If more Fe is taken up during growth under -Cu in order to replace Fe in Cu-containing enzymes, this could explain the observed increase of the -P-responsive miRNAs in phloem sap under Cu deprivation.
Taken together, the data from the -Cu and -Fe experiments indicate a tight link between iron and phosphate metabolism that has earlier been described. Moreover, they suggest a close linkage between iron and copper uptake, although it is known that in higher plants this link is at least not as close as, for example, in yeast or Chlamydomonas, where iron uptake is directly Cu-dependent [35, 36]. It is interesting to note that the tissues/compartments analyzed react differentially to specific stress triggers, but the physiological meaning of this observation needs to be evaluated in future experiments.
Specific miRNAs that accumulate in phloem sap under stress are also mobile in grafting experiments
When analyzing grafts grown under sulfate starvation, we observed the translocation of miR395 from WT scions to hen1-1 rootstocks in different independently grafted plants. We also observed signals for miR395 in WT scions, but not in WT rootstocks (figure 5A). However, miR395 has been previously shown to be expressed in roots under sulfur starvation , and we could also detect signals in roots of intact WT plants (figure 5B). This result could be reproduced in several independent experiments. This could indicate that miR395 translocation from shoot to root is required for root miR395 expression in the WT, but further experiments will be needed to substantiate this assumption. The earlier studies of miR399 translocation do not allow any conclusions about the (non) existence of such a crosstalk, since a comparable graft situation of a stressed WT rootstock with an "unstressed" (not miRNA-producing) scion cannot be achieved when grafting overexpressors with WT plants [2, 3].
For both, miR399 and miR395, we only found signals in hen1-1 rootstocks and never in hen1-1 scions, indicating that mobility was restricted to the direction from shoot-to-root in Arabidopsis seedlings (figure 5A). The reason for this unidirectional translocation might lie in the early developmental stage analyzed, where roots constitute the only real sink organ that needs nutrient supply from the phloem translocation stream. However, the results do not rule out that mobile miRNAs can reach other organs than roots at different developmental stages with different source-sink relationships. Our experiments also did not allow concluding whether mature miR395 or its PT is the translocated species. In the case of miR399, however, it has been previously shown that exclusively mature miRNA and not PTs is transported through graft unions . In addition, no miRNA precursors were detectable in B. napus phloem sap , suggesting that mature miRNAs are the translocated molecules.
The graft translocation of miR395 coincides with a down-regulation of the target APS4
Is the transport of specific miRNAs of biological relevance in intact plants?
Most miRNAs are believed to act in a locally restricted manner, in contrast to the mobile class of siRNAs . Their limited mobility is suggested by the closely correlating patterns of miRNA transcription and activity , the spatial restriction of miRNA gene expression [43, 44], and the limited area of mature miRNA localization . However, phloem mobility of miR399 across graft unions has been demonstrated in earlier studies by grafting miR399 overexpressor with WT plants [2, 3]. In this study, we observed the transport of miR395 and 399 from WT scions to hen1-1 mutant rootstocks. Moreover, one of the miR395 targets, APS4, was down-regulated in grafted mutant roots. This indicates that miR395, like miR399, is transported from shoot to root to down-regulate its target(s). However, the question whether such a miRNA transport is physiologically relevant remains, since members of the miR395 and 399 families can indeed be synthesized in roots of wild type plants under the respective stress [7, 39] (figure 5B). Interestingly, expression of miRNAs 395 and 399 was shown to be highly overlapping, being predominant in vascular tissue, especially in root phloem companion cells (CC) [7, 39].
Different scenarios could explain the observation that specific miRNAs are present in phloem sap and mobile in grafting experiments: 1) None of the phloem miRNAs is specifically targeted for translocation, but instead a portion of all miRNAs highly expressed in CC leaks into sieve elements. No miRNA would represent a signaling molecule. 2) A portion of all miRNAs highly expressed in CC reaches phloem sap, but some of these miRNAs can act as long-distance regulators under certain physiological conditions. 3) Selected miRNAs synthesized in CC are specifically targeted for transport and only these are released into the phloem stream. In this case, all miRNAs present in the phloem would be translocatable information transmitters.
No matter how miRNAs reach phloem sap, they would then be swept away from source to sink organs (in our system from shoots to roots). The translocated miRNAs would probably exit the translocation stream into sink CC in an unspecific manner, as rather unselective unloading of macromolecules into sink tissues has been suggested . Here, they would down-regulate their target mRNAs, no matter whether they are intended to function as signaling molecules or not.
If certain miRNAs should indeed be translocated to transmit information, one possible rationale could be that roots are unable to synthesize sufficient amounts of these miRNAs under stress, or that they need a trigger from the shoot to initialize miRNA synthesis. This might be suggested by the absence of mature miR395 in WT rootstocks of grafted plants that was, however, well detectable in roots of complete WT plants (figure 5). Another explanation might be that some organs experience nutrient deprivation earlier than others, and that the translocated miRNAs serve to coordinate physiological responses with plant parts that are not yet stressed and therefore do not yet synthesize stress-responsive miRNAs themselves. This would resemble the situation in grafted plants, where only scions of the graft produced the stress-induced miRNAs (stressed WT in this study, overexpressors in ), while rootstocks did not (hen1-1 mutants in this study, non-stressed WT in ).
This study demonstrates that the phloem sap sRNA complement is distinct from that of stems, leaves and roots, and that a set of phloem-enriched sRNAs exists. It also shows that the abundance of several phloem sap sRNAs changes under nutrient deficiency conditions. While the results confirmed that the known miRNAs reacting to -S or -Cu, respectively, also respond in phloem sap, they provided no clear indications that the response to -Fe involves miRNA regulation, despite of influencing copper uptake/metabolism.
Grafting studies between WT plants and hen1-1 mutants demonstrated that two phloem stress-reactive miRNAs, 395 and 399, can indeed be transported from shoot to root in Arabidopsis seedlings, and that this translocation leads to a reduction of the amount of their target mRNAs in roots. The grafting experiments also revealed that not all miRNAs are phloem translocatable, since miR171 did not move.
Therefore, this study demonstrates that identifying phloem-enriched macromolecules and analyzing their translocation in grafting studies is a very useful approach to distinguish between phloem translocatable and non-mobile molecules. It is tempting to classify miR395 and 399 as systemic signaling molecules, because they not only move from source to sink, but also induce a measurable effect on their target mRNAs in sink tissue in grafting experiments. However, we conclude that profiling phloem components combined to grafting studies is still not sufficient to doubtless decide whether a phloem-translocatable macromolecule is really a long-distance signal or not.
Plant material and growth conditions
For hydroponic growth, Brassica napus (cv. Drakkar, Serasem GIE, la Chapelle d'Armentiers, France) seeds were germinated on wet filter paper for 1 week. Germ buds were transferred to plastic boxes containing nutrient medium for 10 weeks. Nutrient medium: 0.6 mM NH4NO3, 1 mM Ca(NO3)2*4H2O, 0.04 mM Fe-EDTA, 0.5 mM K2HPO4, 0.5 mM K2SO4, 0.4 mM Mg(NO3)2*6H2O. Micro nutrients added: 0.8 μM ZnSO4*7H2O, 9 μM MnCl2*4H2O, 0.1 μM Na2MoO4*2H2O, 23 μM H3BO3, 0.3 μM CuSO4*5H2O. The pH was adjusted to 4.7 with 37% HCl. Nutrient solutions were changed after 4 weeks, and then renewed once a week. After 5 to 6 weeks, media were constantly aerated by an aquarium air pump (Sera, Heinsberg). Sulfur and copper starvation were applied for two, and iron starvation for three weeks before flowering started by changing to medium without sulfur, copper, or iron, respectively. Here, 0.5 mM K2SO4 were substituted by 0.5 mM K2HPO4 and instead of ZnSO4*7H2O and CuSO4*5H2O as micro nutrients, 1 μM ZnCl2 and 1 μM CuCl2*2H2O were added for low sulfate experiments. For copper deprivation, the 0.3 μM CuSO4*5H2O were omitted from the full nutrient solution. For low iron experiments Fe-EDTA was omitted from the medium.
For the growth of Arabidopsis thaliana WT (ecotype Ler-0) and hen1-1  mutant plant seeds (NASC code N6583) were surface-sterilized in 70% (v/v) ethanol for 3 min and further incubated in 20% sodium hypochlorite solution containing 0.1% (v/v) surfactant (Triton X-100) for 10 min. After exhaustive washing with sterile water, seeds were placed on plates on half-concentrated MS medium  supplemented with 1% (w/v) sucrose and solidified with 0.7% (w/v) agar. After keeping them in the dark for three days at 4°C, seeds were germinated by transferring the plates in a growth chamber under controlled long day conditions (16 h day, 8 h night) at 25°C for 13 days. For hydroponic cultivation these plantlets were transferred into plastic boxes containing the nutrient solution previously described in  with minor modifications in the content of magnesium sulfate, boric acid and potassium dihydrogen phosphate (4 mM MgSO4*7H2O and 0.1 mM H3BO3, 2.5 mM KH2PO4). The hydroponic growth was carried out under short day conditions (8 h day at 20°C, 16 h night at 16°C). For sulfur deprivation experiments starvation was applied directly after the transfer of plantlets to hydroponic culture with nutrient solution omitting all sulfate-containing components for two weeks. Instead of MgSO4*7H2O 0.8 mM MgCl2*6H2O were added to the medium. Phosphate starvation was performed analogously in nutrient solution that contained potassium nitrate instead of potassium dihydrogen phosphate.
For micrografting experiments four-day-old Arabidopsis thaliana wild type and hen1-1 mutant seedlings were cut transversely using a sterile small razor blade part and combined within silicon tubing (0.3 mm internal diameter) as previously described . The grafts were grown on 1.5% (w/v) agar plates with half-strength MS medium for nine days under controlled short day conditions. Successfully grafted plantlets were subsequently grown hydroponically for two weeks before plant material from stock and scion was harvested. To avoid contaminations, the area close to the graft union was omitted from sampling and grafts were microscopically inspected for adventitious root formation, what led to exclusion from analysis.
Sampling and RNA isolation
Phloem sampling from Brassica napus plants was performed as described earlier [1, 12] from 4 - 8 small punctures into the inflorescence stems. After discarding the first droplets to avoid contaminations, 500 μl to 1.5 ml phloem sap from three independent sets of plants were obtained, yielding about 10-50 μg of total RNA. Total RNA from phloem sap was isolated by Trizol LS reagent (Invitrogen) according to manufacturer's instructions.
RNA from 100 mg frozen material of stem, leaf and root tissue of Brassica napus and Arabidopsis thaliana, respectively, was extracted using the normal Trizol reagent. Total RNA from all samples was dissolved in 25 μl DEPC-treated water and RNA concentrations were determined photometrically with a Biophotometer (Eppendorf).
Microarray assays were performed by LC Sciences (Houston, Texas). The assays started from 2 to 5 μg total RNA samples that were size fractionated using a YM-100 Microcon centrifugal filter (Millipore) and the sRNAs (< 300 nt) isolated were 3'-extended with a poly(A) tail using poly(A) polymerase. An oligonucleotide tag was then ligated to the poly(A) tail for later fluorescent dye staining. Two different tags were used for the two RNA samples in dual-sample experiments. Hybridization was performed overnight on μParaflo microfluidic chips using a micro-circulation pump (Atactic Technologies). On the commercial microfluidic chip, each detection probe consisted of a chemically modified nucleotide coding segment complementary to a known target plant miRNA (from miRBase, http://microrna.sanger.ac.uk/sequences/, releases 10.0 (-S), 10.1(-Fe) or 11.0 (-Cu)). The known plant miRNAs were mainly from Arabidopsis thaliana, Oryza sativa, Populus trichocarpa and Physcomitrella patens. Among the total number of unique miRNA sequences (release 10.0, 623 miRNAs, 10.1, 653 miRNAs and 11.0, 714 miRNAs) all arrays contained a constant number of 154 miRNAs from Arabidopsis thaliana. Additionally to these known miRNAs, the customized array contained a set of 85 sRNAs of unknown function that were derived from an earlier high-throughput sequencing experiment of phloem sap  (sequences and accession numbers in additional file 5). Coding segments were coupled to a spacer segment of polyethylene glycol to place the coding segment away from the substrate. The detection probes were prepared by in situ synthesis using PGR (photogenerated reagent) chemistry. The hybridization melting temperatures were balanced by chemical modifications of the detection probes. For hybridization 100 μL 6 × SSPE buffer (0.90 M NaCl, 60 mM Na2HPO4, 6 mM EDTA, pH 6.8) containing 25% formamide at 34°C were used. After hybridization, signals were detected after fluorescence labeling using tag-specific Cy3 and Cy5 dyes. Hybridization images were collected using a laser scanner (GenePix 4000B, Molecular Devices) and digitized using Array-Pro image analysis software (Media Cybernetics). Data were analyzed by first subtracting the background and then normalizing the signals using a LOWESS (locally-weighted regression) filter.
To allow inter-array comparisons of FN samples, signal intensities were normalized to the median signal intensity of each sample and p-values of the t-test were calculated for the three replicates of each organ (phloem, leaves, and roots). Signals with p-values lower than 0.05 were regarded as being differential.
For the stress experiments (two color hybridizations), the ratio of the two sets of detected signals (log2 transformed, balanced) and p-values of the t-test were calculated and signals with p-values lower than 0.01 were regarded as being differential. Since only one array per stress was hybridized, we further restricted the data evaluation to sRNAs that showed a signal intensity of >100 in the FN or the stressed sample, an accumulation upon stress, and a more than four-fold difference (log2s of >2 or <-2) between stress and FN. All microarray data have been submitted to GEO, series accession No. GSE20263.
For semi-quantitative RT-PCR (sqRT-PCR), Trizol isolated RNA was cleaned with the RNeasy Plant Mini Kit (Qiagen) and a DNase I digest following the manufacturers instructions was performed. For nutrient stress-responsive marker gene and miRNA target transcript analysis, 500 - 1000 ng RNA were used for cDNA synthesis in the presence of 2.5 μM oligo(dT)20 primer (Qiagen), 0.5 mM dNTPs, 5 mM DTT (Invitrogen), 40 U RNaseOUT RNase Inhibitor (Invitrogen) and 200 U M-MLV reverse trancriptase (Promega) in 1× M-MLV reverse transcriptase reaction buffer (Promega) in a final volume of 20 μl. The reverse transcription reactions were carried out in a Primus Thermocycler (Peqlab) at 50°C for 45 min followed by 70°C for 15 min to denature the reverse transcriptase enzyme. 2 μl of the reverse transcription reaction were used for each PCR amplification with gene specific oligonucleotide primer pairs (additional file 6). The reaction mixtures containing 1.5 mM MgCl2 (Invitrogen), 0.2 mM dNTPs (Promega), 0.2 μM of both forward and backward primer and 2 U of Paq5000 DNA Polymerase in a 50 μl volume of 1× Paq5000 DNA polymerase buffer (Agilent Technologies) were divided into three equal volumes in reaction tubes and semi-quantitative RT-PCR was performed with different cycle numbers under the following conditions: 30 s at 94°C, 30 s at 55°C, 1 min at 72°C and a 10 min end-elongation step at 72°C. The PCR reaction was stopped after a certain number of cycles and PCR products were separated electrophoretically in 2% (w/v) agarose gels for size estimation and semi-quantitative analysis.
PCR of mature miRNAs was performed by following the method of Shi and Chiang . Total RNA (1 μg) was first polyadenylated by a poly(A) polymerase [E-PAP, Poly(A) Tailing Kit (Ambion)] at 37°C for 1 h in a 50-μL reaction mixture containing 1× E-PAP buffer, 2.5 mM MnCl2, 1 mM ATP and 1 U E-PAP. Samples were purified from E-PAP by a further RNA extraction using TriFast FL reagent (Peqlab) and resolved in 50 μl DEPC-treated water. 10 μl of the polyadenylated RNA samples were used as a template for reverse transcription performed as described above using 0.5 μg poly(T) adapter instead of the oligo(dT)20 primer. miRNAs were subsequently amplified using 1 μl of the reverse transcribed sample, miRNA-specific forward and poly(T) adapter-specific reverse primers (additional file 6) under the same PCR-cycler conditions used in sqRT-PCR described above.
RNA gel blot analysis
We would like to thank Leslie Sieburth (University of Utah, USA) for help with micrografting and Berit Ebert (MPI-MP Potsdam, Germany) for microscopic work. The work presented was financially supported by grant No. BIO2008-03432 and the I3 program from the Spanish Ministry of Science and Innovation (MICINN).
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