Journal of Nucleic Acids

Journal of Nucleic Acids / 2014 / Article

Research Article | Open Access

Volume 2014 |Article ID 214929 | 8 pages |

Selective Evolution of Ligands by Exponential Enrichment to Identify RNA Aptamers against Shiga Toxins

Academic Editor: Birte Vester
Received19 Dec 2013
Revised06 Mar 2014
Accepted25 Mar 2014
Published15 Apr 2014


Infection with Shiga toxin- (Stx-) producing E. coli causes life threatening hemolytic uremic syndrome (HUS), a leading cause of acute renal failure in children. Of the two antigenically distinct toxins, Stx1 and Stx2, Stx2 is more firmly linked with the development of HUS. In the present study, selective evolution of ligands by exponential enrichment (SELEX) was used in an attempt to identify RNA aptamers against Stx1 and Stx2. After 5 rounds of selection, significant enrichment of aptamer pool was obtained against Stx2, but not against Stx1, using a RNA aptamer library containing 56 random nucleotides (N56). Characterization of individual aptamer sequences revealed that six unique RNA aptamers (mA/pC, mB/pA, mC, mD, pB, and pD) recognized Stx2 in a filter binding assay. None of these aptamers bound Stx1. Aptamers mA/pC, mB/pA, mC, and mD, but not pB and pD, partially blocked binding of Alexa 488-labeled Stx2 with HeLa cells in a flow cytometry assay. However, none of the aptamers neutralized Stx2-mediated cytotoxicity and death of HeLa cells.

1. Introduction

Infection with Shiga toxin- (Stx-) producing Escherichia coli (STEC) is the most significant cause of hemolytic uremic syndrome (HUS), the leading cause of acute renal failure in children [14]. Of the two antigenically distinct toxins, Stx1 and Stx2, Stx2 is more firmly linked with the development of HUS as STEC strains producing this toxin are more frequently associated with HUS than strains that produce both Stx1 and Stx2, while Stx1 alone has rarely been associated with HUS [57]. Stx1 and Stx2 are similar in basic structure [8], binding specificity [8], and mode of action. Both toxins consist of an A-subunit monomer and a B-subunit pentamer [810]. The pentameric B subunit binds to its cell surface receptor CD77, also called globotriaosylceramide (Gb3; Galα1-4Galβ1-4glucosyl ceramide) [11, 12]. This triggers endocytosis of the holotoxin, mainly through clathrin-coated pits [13]. The internalization of catalytically active A-subunit, delivered to cytosol via retrograde transport, causes shut down of protein synthesis and leads to cell death [14, 15].

Nucleic acid aptamers are being developed as therapeutic and diagnostic reagents against biotoxins [16]. Aptamers are short, synthetic, single stranded nucleic acids with unique three-dimensional conformations that bind strongly and selectively to a target molecule via shape specific recognition [1720]. Aptamers are similar in many respects to antibodies except that they are cheaper to produce, have extremely long shelf lives, and thus, are far more cost effective than to produce antibodies. A single aptamer against a Shiga toxin has been reported, but it is unknown whether the aptamer is against Stx1 or Stx2 [21]. Toxin-neutralizing ability of this toxin is also unknown [21]. The aim of the present study was to utilize selective evolution of ligands by exponential enrichment to identify ribonucleic acid (RNA) aptamers against Stx1 and Stx2.

2. Materials and Methods

2.1. Stx1 and Stx2

Stx1 and Stx2, purified as described previously [22], were obtained from Phoenix Laboratory (Tufts University, NEMC Microbial Products & Services Facility). Before use, the toxins were passed through Polyacrylamide 6000 Desalting column (Thermoscientific, IL) to suspend them in selection buffer (20 mM HEPES (pH 7.3), 150 mM NaCl, and 5 mM MgCl2). The toxins were quantified by UV spectrophotometry (ND-1000 Spectrophotometer, Nanodrop), aliquoted, and stored at −20°C.

2.2. Preparation of RNA Library

The starting ssDNA library containing 56 random nucleotides flanked by constant regions (5′-CACAGCGGGACAGTTTAGC - N56 - GGTAGGTGGGTGCGTCTAAA-3′) was synthesized by Integrated DNA Technologies, Inc. (Coralville, IA). The DNA random library (4 nmoles or approximately 2.4 × 1015 sequences in 50 mL, that is, 80 nM) sequences were amplified by PCR with 200 μM of each dNTP along with 2 μM each of forward (5′-GATAATACGACTCACTATAGGGCACAGCGGGACAGTTTAGC-3′) and reverse (5′-TTTAGACGCACCCACCTACC-3′) primers using Taq DNA polymerase (New England Biolabs); the forward primer included a T7 promoter region (underlined) for in vitro transcription. In order to prevent the abundance of the original DNA library, PCR was performed for a total volume of 50 mL (100 μL/tube) and was limited to 10 cycles. After the PCR reactions, the amplified dsDNA library was subjected to ethanol precipitation and later converted to RNA library using AmpliScribe T7-Flash Transcription Kit (Epicentre, Madison, WI) according to the manufacturer’s instructions. The in vitro transcription reaction was set up with 12 μL of 65 μM of dsDNA (i.e., 0.8 nmoles or approximately 5 × 1014 sequences). The RNA was purified after completion of the transcription reaction and resuspended in 200 μL of dH2O. The final concentration of purified RNA was found to be 32 nmoles that would have corresponded to 40 copies of original DNA pool, that is, 5 × 1014 sequences (0.8 nmoles).

As unmodified RNA molecules are highly susceptible to nuclease degradation, nuclease resistant modifications were introduced chemically to generate modified RNA aptamer library. Modified library was generated by incorporating 2′-Fluorine-CTP (2′-F-dCTP), 2′-Fluorine-UTP (2′-F-dUTP), ATP, and GTP into full length transcripts with in vitro transcription using DuraScribe T7 transcription kit (Epicentre, Madison, WI, USA) as described elsewhere using Y639F mutant of T7 RNA polymerase [23, 24].

2.3. In Vitro Selection of Aptamers Using Nitrocellulose Membrane

Systematic evolution of ligands by exponential enrichment (SELEX) using nitrocellulose membrane (m-SELEX) was performed as described elsewhere [17] to select aptamers against Stx1 and Stx2. In every round, prior to selection, RNA was thermally equilibrated and refolded in selection buffer by heating to 70°C for 3 min and then slowly cooling to 37°C for at least 10 minutes. In order to minimize nonspecific binding of RNA with the nitrocellulose membrane, the refolded RNA pool was preadsorbed to a 0.45 μm nitrocellulose HAWP filter (Millipore, Bedford, MA) for 30 min prior to every round of selection with Stx1 or Stx2.

In the first selection cycle, the precleared random RNA pool (55.2 μg, 1.6 nmole, 9.6 × 1014 molecules) and Stx1 or Stx2 (0.4 nmole, RNA/toxin ratio 4/1) were incubated in 200 μL selection buffer on a rotating platform for 30 min at room temperature (RT). From round 2, competitor yeast tRNA (0.375 nmole) was also added to the reaction mixture. In rounds 3 and 4, SELEX was performed with equimolar ratio of RNA and toxin to increase the chances of RNA binding to the toxin. Later to improve the stringency of selection, RNA/toxin ratio was increased to 4/1 and 8/1 in rounds 5 and 7, respectively (Table 1). The toxin-RNA mixture was then passed through a prewetted nitrocellulose filter followed by 5 times of washing with 200 μL of selection buffer. The Stx1/Stx2 bound RNA was eluted from the filter with 400 μL TE Buffer (10 mM TRIS, 1 mM EDTA; pH 8.0) at 95°C for 5 min, followed by ethanol precipitation.

Selection roundMembrane-SELEXPlate-SELEX
Input RNA (pmoles)Input Stx1/Stx2 (pmoles)Input RNA (pmoles)Input Stx1/Stx2 (pmoles)


The recovered RNA pool was reverse-transcribed into cDNA in a total volume of 20 μL using MuLV Reverse Transcriptase (Applied Biosystems, CA) and amplified for 12 cycles of PCR followed by ethanol precipitation. Finally, the dsDNA was transcribed in vitro using T7 RNA polymerase and purified on 8% polyacrylamide/7 M urea gels as described above to synthesize the enriched RNA pool to be used for the next round of selection.

2.4. In Vitro Selection of Aptamers Using Microtiter Plate

SELEX was also performed using microtiter plate (p-SELEX) to select aptamers against Stx1 and Stx2. The 96-well plate (Evergreen Scientific, Los Angeles, CA) was coated with 20 μg/mL of Stx1-specific mouse monoclonal antibody (MAb) 4D3 or Stx2-specific mouse MAb 3D1 overnight followed by blocking with 1% BSA (Amgen, Thousand Oaks, CA) and binding with 20 μg/mL of Stx1 or Stx2 (28 pmoles), respectively, in the selection buffer (20 mM HEPES (pH 7.4), 150 mM NaCl, 5 mM MgCl2, and 0.1% Tween 20) for 1 h at RT each. BSA was used instead of tRNA to reduce nonspecific binding of both toxins and RNA as described elsewhere for plate selection [25, 26]. Prior to every round of selection, RNA was thermally equilibrated and refolded as described above and preabsorbed with 4D3/BSA- or 3D1/BSA-bound plate to minimize nonspecific binding of RNA to the plate. After preclearing, RNA was incubated with Stx1 or Stx2 in 100 μL of the selection buffer for 1 h at RT followed by washing 6 times with 200 μL tween-selection buffer. Elution of RNA was performed by heating the plate at 95°C for 5 min and reverse transcription was directly done on the plate at 42°C in a total volume of 50 μL with MuLV Reverse Transcriptase (Applied Biosystems) followed by amplification into DNA by PCR with Taq Polymerase (New England Biolabs). Finally, the DNA was transcribed in vitro using T7 RNA polymerase (Epicentre) and purified on 8% polyacrylamide/7 M urea gels to synthesize the enriched RNA pool to be used for the next round of selection.

2.5. Nitrocellulose Filter Binding Assay

Nitrocellulose filter binding assay was used to evaluate the RNA pool binding capability after every other round [27]. RNA pools after 0, 1, 3, 5, and 7 rounds of selection were radiolabelled during transcription by incorporation of [α-32P]-ATP and subsequently purified on 8% polyacrylamide/7 M urea gels. Thermally equilibrated 10 nM radiolabelled RNA pools were incubated with 0.5 μM of Stx1 or Stx2 or BSA in selection buffer in the presence of 0.1 μg/μL yeast tRNA. The Stx1/Stx2-RNA mixtures were then passed through a vacuum manifold containing nitrocellulose and nylon membranes (the nitrocellulose membrane captures RNA+ protein complexes, while the nylon membrane captures all free RNA that flows through the nitrocellulose membrane) and washed three times with selection buffer. Both nylon and nitrocellulose membranes were exposed to a phosphor screen for at least 4 h and the radioactivity was measured using phosphorimager (Molecular Dynamics Storm Phosphoimager 840, GE/Amersham). The fraction of RNA bound to the Stx1 or Stx2 was calculated with the following formula: fraction bound = cpm on nitrocellulose/(cpm on nitrocellulose + cpm on nylon) × 100.

2.6. Cloning and Sequencing

After 7 rounds of selection with no further enrichment observed, the dsDNA from round 5 of SELEX was amplified by PCR and cloned into pCR 2.1-TOPO Vector cloning vector (Invitrogen, Grand Island, NY) and transformed into E. coli (Top 10 cells, Invitrogen). Fifty-one individual clones from membrane-SELEX (m-SELEX) and 45 clones from plate-SELEX (p-SELEX) were picked and sequenced using M13 forward primer. According to the alignments of individual sequences, membrane-SELEX aptamers were grouped into 5 groups and ELISA-SELEX aptamers were grouped into 4 groups. One representative sequence from each group was chosen for further analysis because of relative abundance within their group.

2.7. HeLa Cell Cytotoxicity Assay

An in vitro HeLa cell cytotoxicity, optimized to evaluate ability of RNA aptamers to neutralize cytotoxic effects of Stx2, was used. HeLa cells were cultured on 96-well plates at 1 × 104 cells/well in DMEM medium with 10% fetal bovine serum overnight at 37°C (complete DMEM medium). After reaching 60–70% cell confluence, cells were washed 4 times with nuclease free phosphate-buffered saline (NF-PBS) (Ambion, TX, USA) before adding Stx2. Stx2 at 0.5 ng/well (0.007 pmole) or 4 ng/well (0.056 pmole) was preincubated either with individual aptamers at 50 μg/well (1550 pmole) or with Stx2-neutralizing HuMAb 5H8 at 1.0 μg/well (6.66 pmole) at 37°C for 30 min before adding to the cells. All reagents were diluted in NF-PBS. Cells were then incubated with either Stx2 alone or Stx2 with RNA aptamers or Stx2 with 5H8 HuMAb at 37°C for 30 min. The supernatants in the wells were collected and run on PAGE to determine degradation of RNA aptamers. The cells were again washed with NF-PBS 4 times and incubated in complete DMEM medium for 24 h at 37°C. The percentage of cell survival in the presence or absence of aptamers and HuMAbs was assessed by crystal violet assay as described [28]. Briefly, cells were washed with PBS and fixed with 4% paraformaldehyde (PF). Crystal violet solution was added to the cells, and after intensive washing with water and drying, the cells were lysed with 100% ethanol. The optical density at 690 nm was measured in a microplate reader. The absorbance (OD) of each well was read at 590 nm. The percentage of cell survival, which is a measurement of the toxin neutralization, was calculated by the following formula: [()/()] × 100.

2.8. Flow Cytometry Analysis

To determine whether Stx2-specific aptamers inhibit binding of Stx2 to its receptor Gb3 on the cell surface, flow cytometry analysis was performed as described [29]. HeLa cell suspensions were produced by treating the cells with 0.05% trypsin-53 mM EDTA. Cells were then washed three times with cold NF-PBS by centrifugation at 300 ×g at 4°C for 10 min. AF488-labeled Stx2 (Stx2-AF) at 0.6 μg/mL (100 μL, 0.8 pmole)NF-PBS was preincubated at 37°C for 1 h with aptamers (500 μg/mL NF-PBS, 100 μL, 1550 pmole), cooled to 4°C, and then added to suspensions of 5 × 105 cells which were also precooled to 4°C. After a 30 min incubation at 4°C, the cells were washed twice in cold NF-PBS and resuspended in 4% PF for 15 min at 4°C. The cells were washed and resuspended in PBS. The cell-associated fluorescence (20,000 cells per treatment) was collected by using BD Accuri C6 flow cytometer (BD Biosciences). Histogram analysis was performed by using BD Accuri C6 software.

3. Results

3.1. Selection of RNA Aptamers for Stx1 and Stx2

The filter binding assay was used to monitor the progress of selection after each SELEX cycle. Strong enrichment of N56 (56 random nucleotides) unmodified RNA aptamer pool for Stx2-binders occurred at 5th round of selection by m-SELEX and p-SELEX as 41% and 29% of the input RNA bound with Stx2, respectively, whereas binding to the membrane and unrelated protein BSA was <5% (Figure 1). The enrichment did not increase with additional rounds of selection by m-SELEX as 47% of the input RNA bound with Stx2 in 7th round of selection, but nonspecific RNA binding to the membrane and BSA increased to >12% (Figure 1(a)). Although 7th round of selection by p-SELEX increased enrichment slightly to 33% with no increase in background binding (Figure 1(b)), the enrichment did not increase following additional rounds of selection by p-SELEX (data not shown). Therefore, highly enriched unmodified RNA aptamer pools of 5th selection rounds by m-SELEX and p-SELEX were cloned and sequenced.

Although identical selection conditions were used to perform SELEX as mentioned above with two modified (nuclease resistant) libraries of 35 and 101 random nucleotides, we could not enrich libraries with Stx2-binders (data not shown). Similarly, none of the unmodified or modified libraries showed any enrichment for Stx1-binders even after 12–20 rounds of selection with each library (data not shown).

3.2. Analysis of the Selected Stx2 Aptamers

Highly enriched unmodified RNA aptamer pools for Stx2-binders were cloned, and ~100 clones from each pool were sequenced. The individual clones were classified into 5 groups from m-SELEX and 5 groups from p-SELEX based on the alignments of individual aptamer sequences. One representative sequence from each group was chosen for further characterization because of their relative abundance within their group (Table 2). The sequences within each group were almost identical except groups m-singles and p-singles which contained sequences that occurred only once. Seventy-eight percent of m-SELEX sequences were grouped into groups mA and mB and 36% of p-SELEX sequences into groups pA and pC. These groups contained an identical 19-nucleotide (ATTCGATCAGGCAGTACGT) region (Table 2). Furthermore, sequences of groups mA and mB were identical to sequences of groups pC and pA, respectively. However, the other 4 groups (mC, mD, pB, and pD) did not have any similarities between them. Filter binding assay was performed to confirm the binding activity of these selected individual aptamers with Stx2 (Figure 2). Except for the group mC (mC_Apt41), all other groups showed strong specific binding with Stx2. Nonetheless, mC_Apt41 also bound Stx2. None of the aptamers from any group bound Stx1 (results not shown).

Groupn 1Sequence2

m-Singles8Orphan sequences6
p-Singles42Orphan sequences5

Number of isolates harboring the represented sequence in each group. 2Complete random sequences of the aptamer core regions (5′-3′) are shown. 3Underlined sequence of 19 bases is identical among groups mA, mB, pA and pC. 4Complete sequences of mA and pC groups are identical. 5Complete sequences of mB and pA groups are identical. 6Orphan sequences are the sequences that are seen only in one isolate.
3.2.1. Flow Cytometry Analysis

In absence of any aptamer, Stx2-AF (0.6 μg/mL, 8 nM) labeled ~78% of the HeLa cells (Figure 3). Control aptamer did not block binding of Stx2 with HeLa cells as 76% cells were labeled by Stx2-AF. Most of the Stx2-specific aptamers (mA_Apt1, mB_Apt23, mC_Apt41, mD_Apt46, pA_Apt1, and pCApt22) inhibited Stx2 binding weakly as approximately 50% of HeLa cells were labeled in the presence of these aptamers (Figure 3). Similar to the unrelated control aptamer, the remaining 2 Stx2-binding aptamers (pB_Apt14 and pD_Apt25) did not inhibit Stx2 binding (Figure 3).

3.2.2. Neutralization of Stx2-Mediated HeLa Cell Cytotoxicity by Aptamers

A limited neutralization of Stx2-mediated cytotoxicity and death of HeLa cells was observed with aptamers mA_Apt1 (~40% cell survival), mB_Apt23 (~20% cell survival), and pC_Apt22 (≤60% cell survival) (Figure 4). Aptamer mC_Apt41 neutralized 0.007 pmole of Stx2 (≤60% cell survival) but not 0.056 pmole of Stx2 (Figure 4). None of the other aptamers neutralized the cytotoxic effects of Stx2 (Figure 4). RNA aptamers did not degrade in the HeLa cell assay as RNA band of HeLa cell-incubated aptamer was of similar intensity in PAGE analysis as that of the unincubated aptamer (not shown).

4. Discussion

The goal of the present study was to identify aptamers that can bind and inactivate Stx1 and Stx2. The well known in vitro SELEX procedure [17, 18] was used to derive RNA aptamers that specifically bind to Stx1 and Stx2. Aptamer libraries without any modifications were used initially to demonstrate proof-in-principle that SELEX can be used to identify aptamers for Stx1 and Stx2. Generally, the aptamer pools with short randomized regions (15 nucleotides) are sufficient for a successful aptamer selection [30]. However, longer randomized regions give the pools a greater structural complexity [31, 32] and an increased possibility for selection of high-affinity aptamers [33]. Thus, we initially performed SELEX using a RNA pool containing 5 × 1014 unique sequences with a central stretch of 56 random nucleotides (N56) and identified aptamers that bound Stx2. However, despite using the same N56 pool and other pools with random nucleotide lengths (N35 and N101) and the same selection conditions as used for Stx2, we could not identify aptamers that bound Stx1. Although reasons for not identifying Stx1-binding aptamers are unclear, it can be assumed that Stx1 may not be a “good” target as evidenced by other studies that not every target is suitable for aptamer selection [32, 34].

Nucleic acid aptamers with binding affinities comparable to those of antibodies have been utilized for flexible applications ranging from diagnostic to therapeutic assay formats. To our knowledge this is the first study that attempted to discover aptamers against Stx2 and identified 6 unique unmodified RNA aptamer groups with Stx2-binding abilities. Although the Stx2-binding aptamers were discovered using N56 aptamer library, almost all aptamers had 39 random nucleotides except the group pD aptamers which had 56 random nucleotides. This is a common occurrence [35, 36] which might be because of the accumulation of either near-full length or nonfull length products in the pool during synthesis or primers recognizing the sequence of nucleotides similar to constant region in the randomized region [37].

All aptamers that bound Stx2 in the filter-binding assay also inhibited Stx2 binding partially with the HeLa cells except the aptamers of groups pB and pD which did not inhibit Stx2 binding. As antibodies that bind Stx2 B subunit but not A subunit are known to inhibit binding of the toxin with its cell surface [29], aptamers of groups mA, mB, mC, mD, pA, and pC that inhibited Stx2 binding may bind Stx2 B subunit. The Stx2-inhibiting aptamers seem to be of low affinity as very high concentrations (1550 pmole) of the aptamers relative to Stx2 concentrations (0.8 pmole) could not inhibit toxin binding completely. The affinity of aptamer was not increased as unmodified aptamers are nuclease sensitive which makes them unsuitable for therapy. These aptamers lost their ability to bind with Stx2 following modification (by incorporating Flourine at the 2′ position in pyrimidine bases) to gain nuclease resistant.

Very high concentrations of aptamers (1550 pmole) neutralized two different concentrations of Stx2 (0.007 pmole and 0.056 pmole) only marginally in HeLa cell assay. In contrast, the HuMAb 5H8 at 6.66 pmole (232 times lower than the aptamer concentrations) completely neutralized Stx2 at the two toxin concentrations. As very high concentrations of aptamers did not neutralize toxin’s activity completely, dose response studies with aptamers were not performed. The insignificant neutralization of the toxin was not due to degradation of the aptamers as HeLa cell assay was performed in nuclease free conditions, and RNA aptamers did not degrade following incubation with HeLa cells.

Although we standardized SELEX to select Stx2-specific unmodified aptamers, our repeated attempts with modified libraries generated using 2′-Fluorine-CTP (2′-F-dCTP) and 2′-Fluorine-UTP (2′-F-dUTP) to identify nuclease resistant RNA aptamers against Stx1 or Stx2 were unsuccessful. As the 2′-fluoro modifications on the ribose ring influence the tertiary structure of an oligonucleotide, it may be expected that modified aptamers form completely unrelated structures compared to unmodified aptamers [23]. Moreover, we could not enrich the libraries with Stx2- or Stx1-binders as background binding was always as much as binding with Stx2 or Stx1 even after 12 rounds and, in a couple of instances, 20 rounds, of selection which might be because of increased hydrophobicity due to replacement of OH with fluorine in the RNA. This shows that SELEX technology is hard to adapt to select aptamers against some targets, such as Stx [34].

5. Conclusions

SELEX procedures, p-SELEX and m-SELEX, yielded unmodified aptamers that bound Stx2 but not Stx1. Each procedure generated 2 groups of Stx2-binding aptamer sequences that were unique to each SELEX procedure and another 2 groups of Stx2-binding aptamer sequences that were shared by the 2 SELEX procedures. These aptamers may be useful to develop Stx2-specific diagnostic assays in the future. Several attempts with modified RNA aptamer libraries to generate nuclease resistant aptamers against Shiga toxins were unsuccessful.

Conflict of Interests

The authors declare that they do not have any conflict of interests with the content of the paper.


The authors thank Drs. Matthew Levy and Sonald Duclaire, Department of Biochemistry, Albert Einstein College of Medicine, for training them with the filter binding assay and their thoughtful discussions on selection of aptamers. This study was supported by Federal Funds from the National Institute of Allergy and Infectious Diseases, National Institutes of Health, under Award nos. AI083369 and AI082079. A. Sheoran was also supported by the Usen Family Career Development Award. The content is solely the responsibility of the authors and does not necessarily represent the official views of the National Institute of Allergy and Infectious Diseases or the National Institutes of Health.


  1. P. Boerlin, S. A. McEwen, F. Boerlin-Petzold, J. B. Wilson, R. P. Johnson, and C. L. Gyles, “Associations between virulence factors of Shiga toxin-producing Escherichia coli and disease in humans,” Journal of Clinical Microbiology, vol. 37, no. 3, pp. 497–503, 1999. View at: Google Scholar
  2. P. M. Griffin and R. V. Tauxe, “The epidemiology of infections caused by Escherichia coli O157:H7, other enterohemorrhagic E. coli, and the associated hemolytic uremic syndrome,” Epidemiologic Reviews, vol. 13, no. 1, pp. 60–98, 1991. View at: Google Scholar
  3. D. V. Milford, C. M. Taylor, B. Guttridge, S. M. Hall, B. Rowe, and H. Kleanthous, “Haemolytic uraemic syndromes in the British Isles 1985–8: association with verocytoxoin producing Escherichia coli. Part 1: clinical and epidemiological aspects,” Archives of Disease in Childhood, vol. 65, no. 7, pp. 716–721, 1990. View at: Google Scholar
  4. S. M. Ostroff, P. I. Tarr, M. A. Neill, J. H. Lewis, N. Hargret-Bean, and J. M. Kobayashi, “Toxin genotypes and plasmid profiles as determinants of systemic sequelae in Escherichia coli O157:H7 infections,” The Journal of Infectious Diseases, vol. 160, no. 6, pp. 994–998, 1989. View at: Google Scholar
  5. A. W. Friedrich, M. Bielaszewska, W.-L. Zhang et al., “Escherichia coli harboring Shiga toxin 2 gene variants: frequency and association with clinical symptoms,” The Journal of Infectious Diseases, vol. 185, no. 1, pp. 74–84, 2002. View at: Publisher Site | Google Scholar
  6. H. Russmann, H. Schmidt, J. Heesemann, A. Caprioli, and H. Karch, “Variants of Shiga-like toxin II constitute a major toxin component in Escherichia coli O157 strains from patients with haemolytic uraemic syndrome,” Journal of Medical Microbiology, vol. 40, no. 5, pp. 338–343, 1994. View at: Google Scholar
  7. S. Tzipori, A. Sheoran, D. Akiyoshi, A. Donohue-Rolfe, and H. Trachtman, “Antibody therapy in the management of Shiga toxin-induced hemolytic uremic syndrome,” Clinical Microbiology Reviews, vol. 17, no. 4, pp. 926–941, 2004. View at: Publisher Site | Google Scholar
  8. M. E. Fraser, M. Fujinaga, M. M. Cherney et al., “Structure of Shiga toxin type 2 (Stx2) from Escherichia coli O157:H7,” The Journal of Biological Chemistry, vol. 279, pp. 27511–27517, 2004. View at: Google Scholar
  9. H. Ling, A. Boodhoo, B. Hazes et al., “Structure of the Shiga-like toxin I B-pentamer complexed with an analogue of its receptor Gb3,” Biochemistry, vol. 37, no. 7, pp. 1777–1788, 1998. View at: Publisher Site | Google Scholar
  10. H. Shimizu, R. A. Field, S. W. Homans, and A. Donohue-Rolfe, “Solution structure of the complex between the B-subunit homopentamer of verotoxin VT-1 from Escherichia coli and the trisaccharide moiety of globotriaosylceramide,” Biochemistry, vol. 37, no. 31, pp. 11078–11082, 1998. View at: Publisher Site | Google Scholar
  11. C. A. Lingwood, H. Law, S. Richardson et al., “Glycolipid binding of purified and recombinant Escherichia coli produced verotoxin in vitro,” The Journal of Biological Chemistry, vol. 262, no. 18, pp. 8834–8839, 1987. View at: Google Scholar
  12. T. Waddell, S. Head, M. Petric, A. Cohen, and C. Lingwood, “Globotriosyl ceramide is specifically recognized by the Escherichia coli verocytotoxin 2,” Biochemical and Biophysical Research Communications, vol. 152, no. 2, pp. 674–679, 1988. View at: Google Scholar
  13. C. A. Lingwood, “Role of verotoxin receptors in pathogenesis,” Trends in Microbiology, vol. 4, no. 4, pp. 147–153, 1996. View at: Publisher Site | Google Scholar
  14. Y. Endo, K. Tsurugi, T. Yutsudo, Y. Takeda, T. Ogasawara, and K. Igarashi, “Site of action of a Vero toxin (VT2) from Escherichia coli O157:H7 and of Shiga toxin on eukaryotic ribosomes. RNA N-glycosidase activity of the toxins,” European Journal of Biochemistry, vol. 171, no. 1-2, pp. 45–50, 1988. View at: Google Scholar
  15. S. K. Saxena, A. D. O'Brien, and E. J. Ackerman, “Shiga toxin, Shiga-like toxin II variant, and ricin are all single-site RNA N-glycosidases of 28 S RNA when microinjected into Xenopus oocytes,” The Journal of Biological Chemistry, vol. 264, no. 1, pp. 596–601, 1989. View at: Google Scholar
  16. L. H. Lauridsen and R. N. Veedu, “Nucleic acid aptamers against biotoxins: a new paradigm toward the treatment and diagnostic approach,” Nucleic Acid Therapeutics, vol. 22, no. 6, pp. 371–379, 2012. View at: Publisher Site | Google Scholar
  17. C. Tuerk and L. Gold, “Systemic evolution of ligands by exponential enrichment: RNA ligands to bacteriophage T4 DNA polymerase,” Science, vol. 249, no. 4968, pp. 505–510, 1990. View at: Google Scholar
  18. A. D. Ellington and J. W. Szostak, “In vitro selection of RNA molecules that bind specific ligands,” Nature, vol. 346, no. 6287, pp. 818–822, 1990. View at: Publisher Site | Google Scholar
  19. M. Famulok, J. S. Hartig, and G. Mayer, “Functional aptamers and aptazymes in biotechnology, diagnostics, and therapy,” Chemical Reviews, vol. 107, no. 9, pp. 3715–3743, 2007. View at: Publisher Site | Google Scholar
  20. S. M. Nimjee, C. P. Rusconi, and B. A. Sullenger, “Aptamers: an emerging class of therapeutics,” Annual Review of Medicine, vol. 56, pp. 555–583, 2005. View at: Publisher Site | Google Scholar
  21. M. Fan, S. R. McBurnett, C. J. Andrews, A. M. Allman, J. G. Bruno, and J. L. Kiel, “Aptamer selection express: a novel method for rapid single-step selection and sensing of aptamers,” Journal of Biomolecular Techniques, vol. 19, no. 5, pp. 311–319, 2008. View at: Google Scholar
  22. A. Donohue-Rolfe, D. W. K. Acheson, A. V. Kane, and G. T. Keusch, “Purification of Shiga toxins and Shiga-like toxin I and II by receptor analog affinity chromatography with immobilized P1 glycoprotein and production of cross-reactive monoclonal antibodies,” Infection and Immunity, vol. 57, no. 12, pp. 3888–3893, 1989. View at: Google Scholar
  23. J. Ruckman, L. S. Green, J. Beeson et al., “2′-fluoropyrimidine RNA-based aptamers to the 165-amino acid form of vascular endothelial growth factor (VEGF165): inhibition of receptor binding and VEGF-induced vascular permeability through interactions requiring the exon 7-encoded domain,” The Journal of Biological Chemistry, vol. 273, no. 32, pp. 20556–20567, 1998. View at: Publisher Site | Google Scholar
  24. R. Padilla and R. Sousa, “A Y639F/H784A T7 RNA polymerase double mutant displays superior properties for synthesizing RNAs with non-canonical NTPs,” Nucleic Acids Research, vol. 30, no. 24, article e138, 2002. View at: Google Scholar
  25. L. V. Gening, S. A. Klincheva, A. Reshetnjak, A. P. Grollman, and H. Miller, “RNA aptamers selected against DNA polymerase β inhibit the polymerase activities of DNA polymerases β and κ,” Nucleic Acids Research, vol. 34, no. 9, pp. 2579–2586, 2006. View at: Publisher Site | Google Scholar
  26. A. Berezhnoy, C. A. Stewart, J. O. Mcnamara II et al., “Isolation and optimization of murine IL-10 receptor blocking oligonucleotide aptamers using high-throughput sequencing,” Molecular Therapy, vol. 20, no. 6, pp. 1242–1250, 2012. View at: Publisher Site | Google Scholar
  27. S. D. Jhaveri and A. D. Ellington, “In vitro selection of RNA aptamers to a protein target by filter immobilization,” in Current Protocols in Molecular Biology, chapter 9, unit 9.3, 2001. View at: Google Scholar
  28. A. S. Sheoran, S. Chapman-Bonofiglio, B. R. Harvey et al., “Human antibody against Shiga toxin 2 administered to piglets after the onset of diarrhea due to Escherichia coli O157:H7 prevents fatal systemic complications,” Infection and Immunity, vol. 73, no. 8, pp. 4607–4613, 2005. View at: Publisher Site | Google Scholar
  29. G. Krautz-Peterson, S. Chapman-Bonofiglio, K. Boisvert et al., “Intracellular neutralization of Shiga toxin 2 by an A subunit-specific human monoclonal antibody,” Infection and Immunity, vol. 76, no. 5, pp. 1931–1939, 2008. View at: Publisher Site | Google Scholar
  30. L. C. Bock, L. C. Griffin, J. A. Latham, E. H. Vermaas, and J. J. Toole, “Selection of single-stranded DNA molecules that bind and inhibit human thrombin,” Nature, vol. 355, no. 6360, pp. 564–566, 1992. View at: Publisher Site | Google Scholar
  31. K. A. Marshall and A. D. Ellington, “In vitro selection of RNA aptamers,” Methods in Enzymology, vol. 318, pp. 193–214, 2000. View at: Google Scholar
  32. R. Stoltenburg, C. Reinemann, and B. Strehlitz, “SELEX—a (r)evolutionary method to generate high-affinity nucleic acid ligands,” Biomolecular Engineering, vol. 24, no. 4, pp. 381–403, 2007. View at: Publisher Site | Google Scholar
  33. S. Klussmann, The Aptamer Handbook: Functional Oligonucleotides and Their Applications, Wiley-VCH, 2006.
  34. B. Hall, S. Arshad, K. Seo et al., “In vitro selection of RNA aptamers to a protein target by filter immobilization,” in Current Protocols in Molecular Biology, chapter 9, unit 9.3, pp. 1–27, 2010. View at: Google Scholar
  35. C. Mannironi, A. di Nardo, P. Fruscoloni, and G. P. Tocchini-Valentini, “In vitro selection of dopamine RNA ligands,” Biochemistry, vol. 36, no. 32, pp. 9726–9734, 1997. View at: Publisher Site | Google Scholar
  36. A. Geiger, P. Burgstaller, H. von der Eltz, A. Roeder, and M. Famulok, “RNA aptamers that bind L-arginine with sub-micromolar dissociation constants and high enantioselectivity,” Nucleic Acids Research, vol. 24, no. 6, pp. 1029–1036, 1996. View at: Publisher Site | Google Scholar
  37. B. Hall, J. M. Micheletti, P. Satya, K. Ogle, J. Pollard, and A. D. Ellington, “Design, synthesis, and amplification of DNA pools for in vitro selection,” Current Protocols in Nucleic Acid Chemistry, chapter 9, unit 9.2, 2009. View at: Google Scholar

Copyright © 2014 Sreerupa Challa et al. This is an open access article distributed under the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original work is properly cited.

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