Open Access

Introduction of a novel 18S rDNA gene arrangement along with distinct ITS region in the saline water microalga Dunaliella

  • Mohammad A Hejazi1Email author,
  • Abolfazl Barzegari1,
  • Nahid Hosseinzadeh Gharajeh1 and
  • Mohammad S Hejazi2
Contributed equally
Saline Systems20106:4

DOI: 10.1186/1746-1448-6-4

Received: 26 October 2009

Accepted: 8 April 2010

Published: 8 April 2010

Abstract

Comparison of 18S rDNA gene sequences is a very promising method for identification and classification of living organisms. Molecular identification and discrimination of different Dunaliella species were carried out based on the size of 18S rDNA gene and, number and position of introns in the gene. Three types of 18S rDNA structure have already been reported: the gene with a size of ~1770 bp lacking any intron, with a size of ~2170 bp consisting one intron near 5' terminus, and with a size of ~2570 bp harbouring two introns near 5' and 3' termini. Hereby, we report a new 18S rDNA gene arrangement in terms of intron localization and nucleotide sequence in a Dunaliella isolated from Iranian salt lakes (ABRIINW-M1/2). PCR amplification with genus-specific primers resulted in production of a ~2170 bp DNA band, which is similar to that of D. salina 18S rDNA gene containing only one intron near 5' terminus. Whilst, sequence composition of the gene revealed the lack of any intron near 5' terminus in our isolate. Furthermore, another alteration was observed due to the presence of a 440 bp DNA fragment near 3' terminus. Accordingly, 18S rDNA gene of the isolate is clearly different from those of D. salina and any other Dunaliella species reported so far. Moreover, analysis of ITS region sequence showed the diversity of this region compared to the previously reported species. 18S rDNA and ITS sequences of our isolate were submitted with accesion numbers of EU678868 and EU927373 in NCBI database, respectively. The optimum growth rate of this isolate occured at the salinity level of 1 M NaCl. The maximum carotenoid content under stress condition of intense light (400 μmol photon m-2 s-1), high salinity (4 M NaCl) and deficiency of nitrate and phosphate nutritions reached to 240 ng/cell after 15 days.

Background

Dunaliella is an unicellular halotolerant microalga with a great potential as transgenic bioreactor [1], and more significantly, food source and pharmaceuticals due to its ability to accumulate large amounts of carotenoids [2]. Isolation and identification of novel species and strains from natural habitats is the main purpose in the path of obtaining superior productive strains. On one hand due to environmental adaptation and lacking of a cell wall, a certain Dunaliella isolate may exhibit different morphological and physiological behaviour in different conditions [3]. On the other hand, wide geographic distribution of saline systems and required distinctive adaptations to these environments lead to extensive diversity of the organisms living in these systems [4]. In addition, slight molecular-based phylogenetic differences of Dunaliella species can reveal deep distinction in production of metabolites such as carotenoids [5]. Hence, molecular characterization provides an important tool for exploring biodiversity of Dunaliella and better understanding of its taxonomy.

Identification and classification of the organisms based on conserved and variable regions of 16S or 18S rDNA is a common procedure in taxonomy studies [6]. 18S rDNA gene has been used for molecular identification of different species of Dunaliella as eukaryotic microorganism [79]. Besides using intron sizing method, particular 18S rDNA fingerprint profiles were reported as an indicator for hyperproducer species [10]. Ribosomal spacer sequences, including ITS regions have been also frequently utilized for discrimination of genetic variation in green algae [1115]. Sequence comparison of the ITS region was utilized to predict genetic relatedness and to study phylogeny and taxonomy of Dunaliella [5, 15].

18S rDNA gene in Dunaliella genus contains relatively conserved region of exon(s) and variable region of intron(s). It is worth nothing that some species don't have any intron. Wilcox et al. (1992) declared that the type of introns present in the genus Dunaliella belongs to group I [16]. Different secondary structure of group I introns makes it distinguished from those of group II and III introns [17]. Group I introns display widespread but irregular distribution in the organisms [18]. These introns are frequently present in lower eukaryotes, especially algae and fungi [19, 20]. Since nuclear rDNAs are heritable, group I introns can be used as phylogenetic markers [20]. Olmos et al. (2000 and 2002) [7, 8] designed and used conserved primers (directed to exon region of 18S rDNA) and species-specific primers (directed to the introns of 18S rDNA) to identify some species. Based on these studies, some intron arrangements in 18S rDNA region were identified in different species of Dunaliella. They reported that 18S rDNA gene of D. tertiolecta (~1770 bp) lacks any intron, 18S rDNA gene of D. salina (~2170 bp) has just one intron after the first exon at 5' terminus that we call as intron 1. 18S rDNA gene in both species D. parva and D. bardawil (~2570 bp) possess two introns; one after the first exon at 5' terminus and the other after the second exon at 3' terminus that we name them as introns 1 and 2, respectively. More recently partial sequence of D. viridis 18S rDNA gene (GenBank: DQ009776) has been submitted with a size of 2494 bp in NCBI [21]. D. viridis has a longer intron compared to the introns 1 and 2, after the first and before the second exon, again at 5' terminus. We name this intron as intron 3. As molecular aspects of these microorganisms have not been studied enough, and so little is known about the different types of intron arrays, there is possibility of revealing diverse structure of 18S rDNA region. This may lead to discovery of new species/subspecies. This research was conducted to study the structure of 18S rDNA gene in one of the Iranian isolates of Dunalilla. The investigation was accompanied by studying ITS region simultaneously. 18S rDNA and ITS region of this isolate were submitted at NCBI by accession numbers of EU678868 and EU927373, respectively.

Results and Discussion

PCR Amplification of 18S rDNA gene

DNA extraction was performed when the cell density of liquid culture was approximately 8 × 103 cell/ml. In order to confirm the genus of the isolate, PCR amplification of 18S rDNA gene was performed using MA1-MA2 primers. These primers allow amplification of almost full length of 18S rDNA in different Dunaliella species. In addition, to investigate the species level of our isolate, PCR amplification was carried out using the species-specific primers. PCR amplification with MA1-MA2, resulted in production of a ~2170 bp DNA band (Figure 1). The amplification with species-specific primers of DSs-MA2, DPs-MA2 and DBs-MA2 created no DNA fragment.
Figure 1

Amplification with conserved primers of MA1-MA2. The PCR product was analyzed by electrophoresis using 1% agarose gel and marked using 1 kb DNA ladder (Fermentas Co.).

Using MA1-MA2, the presence of the DNA amplicon confirmed the genus of our isolate as Dunaliella. Concerning the species of Dunaliella, it is reminded that D. tertiolecta, D. salina, D. parva and D. bardawil produce ~1770, ~2170, ~2570 and ~2570 bp DNA fragments with these primers, respectively [7, 8]. Based on the submitted sequence of D. viridis (GenBank: DQ009776), 18S rDNA band size of about 2500 bp is expected using these primers. As shown in figure 1, the size of the amplified DNA was similar to 18S rDNA size of two 19/3 and 19/18 strains of D. salina.

Moreover, according to Olmos et al. (2000 & 2002) DSs-MA2 should amplify a DNA fragment of ~750 bp in D. salina, DPs-MA2 should produce DNA amplicon with the size of ~1050 bp in D. parva and DBs-MA2 should amplify a fragment of ~1000 bp in D. bardawil. Because D. tertiolecta lacks any intron, no DNA amplicon is expected with species-specific primers. Taken these results together, although the size of 18S rDNA gene was similar to that of D. salina, creation of no PCR product with any of species-specific primers including DSs-MA2 suggests that 18S rDNA profile in our isolate is different from the others studied so far.

RFLP and Sequence analysis of 18S rDNA gene

The accuracy of the discrepancy from D. salina was approved by RFLP analysis. The restriction patterns of 18S rDNA gene of the isolate ABRIINW-M1/2 exhibited different polymorphism (data not shown) comparing with both strains of D. salina 19/3 and 19/18. When digested with Taq I, 18S rDNA of our isolate was cut into 5 restricted fragments, while in both standard D. salina samples 4 different fragments were produced.

18S rDNA sequencing was performed in order to obtain detailed information regarding the structure of this region in our isolate. The sequence of our isolate along with those of other Dunaliella species were aligned multiply (Figure 2). Due to the lack of any intron in D. tertiolecta 18S rDNA gene, this species was excluded from the figure and further analysis. As seen in figure 2, our isolate (ABRIINW-M1/2) lacks a fragment composed of 414 nucleotides extended from 1164 to 1578 corresponding to the intron 1. Moreover, the gene of our isolate possesses a variable region of 440 nucleotides at 3' terminus starting from about nucleotide 2195. Numbering was conducted according to the 18S rDNA sequence of D. parva with accession number of M62998. Lack of intron 1 and presence of intron 2 in our isolate discriminate the isolate from D. salina which contains only intron 1, as we already discussed in the introduction. It should be noted that according to DNA alignment, partially submitted 18S rDNA sequence of D. peircei (strain UTEX LB 2192, GenBank: DQ009778) whose fingerprint profile was unpublished includes a corresponding region extending from about 1164 to 1580, in the same position as the intron of D. salina.
Figure 2

18S rDNA sequence alignment of Dunaliella sp. ABRIINW-M1/2 and other Dunaliella species. Data for other species were gathered from NCBI. The conserved regions of the gene are demonstrated in different colour (red).

D. parva and D. bardawil contain both intron 1 and intron 2 with a 18S rDNA length of about 2570 nucleotides. This is while, our isolate lacks intron 1 and harbours a 18S rDNA with a size of about 2170 nucleotides. Therefore, the isolate would be different from D. parva and D. bardawil.

D. viridis contains only one longer intron compared with introns 1 and 2. It is settled after the first and before the second exon in a position near to 5' terminus with a size of about 810 nucleotides. Accordingly, the isolate does not belong to the species of D. viridis, either. The position and arrangement of introns in different forms is depicted in Figure 3.
Figure 3

Diagram showing the position of intron insertions in 18S rDNA gene of Dunaliella species. 18S rDNA arrangement is demonstrated in 5 group based on the insertion site of introns. The names of the species wich have the corresponding type of arrangement is written in left side.

18S rDNA sequence of our isolate was submitted at NCBI by the name of Dunaliella sp. ABRIINW-M1/2 and accesion number of EU678868. ABRIINW stands for Agricultural Biotechnology Institute of Iran, Northwest and West region where this research was performed in.

All cluster analyses using Neighbor Joining (NJ), Unweighted Pair Group Method with Arithmatic Mean (UPGMA), Maximum Parsimony (MP) and Minimum Evolution (ME) of MEGA4 showed similar clade arrangement. They strongly supported (88-93% bootstrap values) the branch including Dunaliella sp. ABRIINW-M1/2 differing from other taxa. Figure 4 shows the result of bootstrap analysis of NJ tree. All sequences in the dendrogram were divided into three lineages of A, B and C. As seen in the figure, Dunaliella sp. ABRIINW-M1/2 appeared as individual entity (clade B) differing from two strains (19/3 and 19/18) of D. salina and D. peircei (clade A) with high bootstrap value (93%). The cluster including clades A and B was divergent from clade C which is composed of D. viridis, D. bardawil and D. parva.
Figure 4

Phylogram based on 18S rDNA gene for the species of Dunaliella and Dunaliella sp. ABRIINW M1/2. The tree is constructed using neighbor-joining method. Bootstrap values were calculated from 1000 replicates.

In the next step, the intron location of various Dunaliella species were marked and they were aligned seperately (Figure 5). This analysis showed that the intron of Dunaliella sp. ABRIINW-M1/2, displayed the highest similarity of 79% and 83% with intron 2 present in D. parva and D. bardawil.
Figure 5

18S rDNA intron alignment of Dunaliella sp. ABRIINW-M1/2 and other Dunaliella species. Data for other species were gathered from NCBI. The conserved regions of the gene are demonstrated in different colour (red).

In order to better investigate the similarity of intron regions, phylogenetic tree was calculated using neighbor-joining (NJ). The result of bootstrap analysis of NJ tree is displayed in Figure 6. The intron sequences were clustered in two separate groupings. The intron of D. salina 19/3 and D. salina 19/18 together with the corresponding region in D. peircei showed homology with the clade containing intron 1 of D. parva and D. bardawil which has lineage with D. viridis. The single intron of ABRIINW-M1/2 was grouped with intron 2 of D. bardawil and D. parva. These results further approved the novelty of the gene arrangement.
Figure 6

Phylogram based on the intron of 18S rDNA gene for the species of Dunaliella and Dunaliella sp. ABRIINW M1/2. The first and second introns of the species D. parva and D. bardawil are represented with 1 and 2, respectively. The tree is constructed using neighbor-joining method. Bootstrap values were calculated from 1000.

PCR amplification and sequence analysis of ITS region

In addition to 18S rDNA gene, we PCR ampified and sequenced Internal Transcribed Sequence (including ITS1, 5.8 rDNA and ITS2) of our isolate to assess the diversity with other members of Dunaliella genus. PCR amplification of ITS region resulted in production of a single band with a size of ~700 bp (Figure 7) similar to its size in the other species. This length was expected as it was found that ITS region in Dunaliella does not show the length variation at intra- or interspecific level (10). Then the sequence was aligned with 16 different strains (table 1) whose ITS sequences were fully recorded at NCBI including the outgroup of Ch. reinhardtii (Figure 8). ITS nucleotide sequence of Dunaliella sp. ABRIINW-M1/2 exhibited various similarities ranging from 78-88% with others. It showed the highest and lowest similarity with D. viridis and D. salina Ds18S3, respectively. Since ITS sequence of D. peircei was submitted as separate sets of ITS1 and ITS2 and they didn't show any significant similarity with the corresponding regions of the others, it was excluded from the analysis. The ITS sequence of Dunaliella sp. ABRIINW-M1/2 was registered with accession number of EU927373 in NCBI database.
Figure 7

ITS amplification with the primers of AB1-AB2. The PCR product was analyzed by electrophoresis using 1% agarose gel and marked using 1 kb DNA ladder (Fermentas Co.).

Table 1

List of Dunaliella strains investigated in this study

Dunaliella strains

Accession NO. (18S rDNA)

Accession NO. (ITS region)

Dunaliella sp. ABRIINW-M1/2

EU678868

EU927373

Dunaliella bardawil

AF150905

DQ116744

Dunaliella parva

M62998

DQ116746

Dunaliella salina strain CCAP 19/3

EF473743

EF473744

Dunaliella salina strain CCAP 19/18

EF473745

EF473746

Dunaliella viridis strain CONC002

DQ009776

DQ377098

Dunaliella peircei strain UTEX LB 2192

DQ009778

 

Dunaliella salina SAG 42.88

 

EF473741

Dunaliella salina Ds18S3

 

FJ360758

Dunaliella salina Ds18S1

 

FJ360756

Dunaliella salina Dsge

 

EF473732

Dunaliella tertiolecta CCAP 19/27

 

EF473748

Dunaliella tertiolecta ATCC 30929

 

EF473742

Dunaliella tertiolecta SAG 13.86

 

EF473738

Dunaliella tertiolecta Dtsi

 

EF473730

Dunaliella primolecta

 

DQ116745

Dunaliella sp. hd10

 

DQ116747

Chlamydomonas reinhardtii

AB511836

AB511842

Figure 8

ITS (ITS1, 5.8 rDNA and ITS2) sequence alignment of Dunaliella sp. ABRIINW-M1/2 and other Dunaliella species. Data for other species were gathered from NCBI.

In order to study phylogenetic relationship between our isolate and the other Dunaliella species based on ITS region, different algorithms available at MEGA4 were utilized. Figure 9 shows the corresponding dendrogram established by NJ. As expected the outgroup, Ch. reinhardtii was the divergent from other taxa related to Dunaliella species. The cluster analysis of 16 taxa including our isolate demonstrated their association into four clades. Clade A contains all strains of D. tertiolecta (CCAP 19/27, ATCC 30929, SAG 13.86 and Dtsi), two strains of D. salina (SAG 42.88 and Dsge), D. primolecta, D. parva, D. bardawil and Dunaliella sp. hd10. Clade B consists of two strains of D. salina Ds18S1 and D. salina Ds18S3. Clade C includes two other strains of D. salina (CCAP 19/3 and CCAP 19/3) with weak bootstrap value of 50%. The isolate of our interest, Dunaliella sp. ABRIINW-M1/2 appeared in clade D together with D. viridis strain CONC002 (bootstrap value: 83%). The tree supported the split between this clade (D) and all other taxa included in clades A, B and C.
Figure 9

Dendrogram showing the relationship among Dunaliella sp. ABRIINW-M1/2 and species of Dunaliella. The tree is based on ITS region and was constructed using the neighbor-joining method. Bootstrap values were calculated from 1000.

Salt tolerance and carotenoid production ability

Salt tolerance and growth experiments showed that our isolate can grow at different salinity levels ranging from 0.5 to 4 M NaCl but the highest cell concentration was obtained at 1 M NaCl (14.4 × 108 cell/ml).

The carotenoied content of the cells, cultivated under stress condition of high light intensity (400 μmol photon m-2 s-1), high salinity (4 M NaCl) and nutrient limitation (deficiency of KNO3 and KH2PO4), was measured on days 12, 15 and 21. The carotenoid content of the cells reached to the maximum amount of 240 ng/cell after 15 days and remained constant till day 21.

Conclusion

This work demonstrates a new 18S rDNA arrangement in Dunaliella genus. Although the size of 18S rDNA is similar to that of D. salina, position and nucleotide structure of the intron is clearly different. The isolate differs from D. bardawil and D. parva by the size of 18S rDNA and number of the introns. Likewise, it varies from D. viridis in terms of 18S rDNA gene length, and the size and position of the intron. Further, analysis of ITS region sequence indicated that this region in our isolate shows similarity ranging from 78-88% with those of previously known species. Based on the phylogenetic analysis, this isolate with its closest related taxon of D. viridis was divergent from all other taxa. Thereupon, the reported sequences are considered as novel 18S rDNA arrangement and distinct ITS region. Optimum growth of this isolate occurred at 1 M NaCl and Maximum total carotenoid was measured as 240 ng/ml. However, complementary morpho-physiological studies of the isolate are needed to elucidate if the isolate is a new species/subspecies.

Materials and methods

Dunaliella isolation and culture condition

Sampling was attempted from Maharlou saline lake of Iran. 10 ml of the specimens were cultivated in a liquid medium described by Hejazi and Wijffles [22] containing 9% NaCl. Dunaliella single clonies were obtained by spreading the liquid culture on the solidified medium containing 1.8% Agar. Then each single clony was cultured in 50 ml liquid medium. The culture was incubated at 26°C and irradiance of of 80 μmol photon m-2 s-1 in the photoperiod of 16: 8 (L: D). Two strains of 19/3 and 19/18 D. salina were obtained from CCAP (Culture Collection of Algae and Protozoa) as standard strains of D. salina.

Genomic DNA extraction

DNA extraction was conducted according to the protocol developed in our laboratory: 1.5 microlitre of the green algae culture was centrifuged for 5 min at 5000 rpm, and supernatant was discarded. The micoalgal cells were suspended in the lysis buffer containing CTAB 10 g/l, NaCl 80 g/l, Trise 12 g/l, EDTA 7 g/l, LiCl 2 g/l, PVP 2 g/l and shaked to be well mixed. After incubation at 60°C for 10 min, the mixture was centrifuged for 5 min at 10,000 rpm. Then equal volume of Chloroform-isoamylalcohol (24:1) was added and again centrifuged for 5 min at 12000 rpm. Upperphase supernatant was transferred into a new tube and genomic DNA was precipitated by addition of equal volume of isopropanol. The tube was kept for 10 min at -20°C, then centrifuged at 13000 rpm for 5 min. Supernatant was discarded and the DNA pellete was finally washed twice using ethanol 70%.

PCR amplification of 18S rDNA

To amplify 18S rDNA gene, two conserved primers called MA1 and MA2, corresponding to conserved regions of 5' and 3' termini, respectively, were used as forward and reverse primers [7]. PCR reactions were performed in 50 μl containing 20 ng genomic DNA in TE (Tris/EDTA) buffer, pH 8 [23] and 50 ng of the primers using 1× PCR Master Kit (CinnaGen PCR Masster Kit, Cat. No. PR8250C). Amplification was performed using 32 cycles in a TECHNE Thermal Cycler (Model: FTGRAD2D). The amplification was achieved according to the method described by Olmos et al. (2000).

Based on the differences in the number and sequence of introns in various Dunaliella species, Olmos et al. (2000 & 2002) designed three species-specific primers of DSs (5'-GCAGGAGAGCTAATAGGA-3'), DPs (5'-GTAGAGGGTAGGAGAAGT-3') and DBs (5'-GGGAGTCTTTTTCCACCT-3') for descrimination of the species. Primer DSs is directed to the single intron of D. salina. Primers DBs, DPs are directed to the second intron of D. parva and second intron of D. bardawil, respectively. They were used as forward primers along with the primer MA2 as reverse primer for species identification according to the method suggested by Olmos et al. (2002).

PCR amplification of ITS region

To design primers for ITS region, including ITS1, 5.8S rDNA and ITS2, full ITS sequence of 6 strains namely Dunaliella bardawil DQ116744, Dunaliella parva DQ116746, Dunaliella salina CCAP 19/3 EF473744, Dunaliella salina CCAP 19/18 EF473746, Dunaliella tertiolecta CCAP 19/27 EF473748 and Dunaliella viridis CONC 002 DQ377098 were imported to Oligo5 program. Two primers of AB1 (5'-AATCTATCAATAACCACACCG-3') and AB2 (5'-TTTCATTCGCCATTACTAAGG-3') were designed according to conserved sequences flanking ITS region in Dunaliella species. These primers cover nucleotides 1-21 of ITS1 and 80-100 of 28S rDNA gene, respectively. The target sequence was amplified in total mixture volume of 50 μl in above mentioned condition. PCR amplification was carried out as follows: 5 min at 95°C as initial denaturing time, 35 cycles of 94°C for 1 min, 57°C for 50 sec and 72°C for 1 min followed by final extention step of 72°C for 10 min.

Restriction Fragment Length Polymorphism (RFLP) of amplified 18S rDNA gene

For preliminary assessment of the sequence difference in certain isolates/species which were assumed to be correlated, the PCR products of the relevant samples were exposed to restriction endonuclease of Taq I. According to the protocol of manufacters (Germany, Fermentase), 250 ng of the product was digested with 5 U of the enzyme in 37 C for 3 hours. Restriction fragments were resolved through 2% agarose gel and were stained by ethidium bromide.

Purification and sequencing of PCR products

PCR amplicons were purified using PCR purification kit (Roche) according to the manufacturer's instructions. Then, the purified products were sequenced by Macrogen company (Korea). Using BLAST software, the determined sequences were compared with the sequences deposited in NCBI GenBank as 18S rDNA and ITS regions of different Dunaliella species.

Phylogenetic analysis of sequences

To analyze the phylogeny of the isolated Dunaliella, alignment of the sequences was performed with the sequences of different Dunaliella species which were submitted in NCBI database as complete sequence (table 1). Multiple alignment was performed using Expasy, Multalin [At GENOTOUL BIOINFO] website. Four algorithms available at MEGA4 ver. 4: Neighbour-Joining (NJ), Unweighted Pair Group Method with Arithmatic Mean (UPGMA), Maximum Parsimony (MP) and Minimum Evolution (ME) were employed to construct phylogenetic relationships. Using NJ, the evolutionary distances were computed using the Maximum Composite Likelihood model and reliability of the branches was assessed by bootstrapping the data with 1000 replicates. Phylogenetic studies included Chlamydomonas reinhardtii (GenBank: AB511836 and AB511842 for 18S rDNA and ITS region, respectively) as the outgroup.

Salt tolerance and carotenoid production ability

To determine the optimum growth rate, the isolate of our interest was grown at five different concentrations of NaCl (0.5, 1, 2, 3 and 4 M). The flasks were maintained at 26°C and of 80 μmol photon m-2 s-1 in 16 h light: 8 h dark cycle. Growth behaviour of the isolate was measured every two days using a Neubaur haemocytometer.

For determination of carotenoid content, the described liquid medium was prepared with 4 M NaCl. Further, the cultures were exposed to deficiency of nitrate (KNO3) and phosphate (KH2PO4). The flasks were shaked and maintained at constant high light intensity of 400 μmol photon m-2 s-1. The stress condition was considered to obtain the maximum carotenoid production. Both optimum growth salinity and carotenoid studies were conducted in triplicate samples.

Carotenoid extraction was carried out after 12, 15 and 21 days cultivation. Its concentrations were deternined spectrophotometrically according to the method descrýbed by Hejazi et al. [24].

Notes

Declarations

Acknowledgements

This study was financially supported by Agricultural Biotechnology Research Institute of Iran (ABRII). The authors thank ABRII for the support.

Authors’ Affiliations

(1)
Branch for the Northwest and West Region, Agricultural Biotechnology Research Institute of Iran (ABRII)
(2)
Pharmacy faculty, Tabriz University

References

  1. Xue L, Pan W, Jiang G, Wang J: Transgenic Dunaliella salina as a bioreactor. United States Patent 7081567. 2001Google Scholar
  2. Borowitzka MA, Borowitzka LJ: Dunaliella. Micro-algal Biotechnology. Edited by: Borowitzka MA, Borowitzka LJ. 1988, Cambridge: Cambridge University Press, 27-58.Google Scholar
  3. Oren A: A hundred years of Dunaliella research: 1905-2005. Saline Systems. 2005, 1: 1-14. 10.1186/1746-1448-1-2.View ArticleGoogle Scholar
  4. Abatzopoulos TJ, Beardmore JA, Clegg JS, Sorgeloos P: Artemia: Basic and Applied biology. 2002, Kluwer Academic PublishersView ArticleGoogle Scholar
  5. Gómez PI, Gonzaléz MA: Genetic variation among seven strains of Dunaliella salina (Chlorophyta) with industrial potential, based on RAPD banding patterns and on nuclear ITS rDNA sequences. Aquaculture. 2004, 233: 149-162. 10.1016/j.aquaculture.2003.11.005.View ArticleGoogle Scholar
  6. Olsen GJ, Lane DJ, Giovannoni SJ, Pace NR: Microbial ecology and evolution: a ribosomal RNA approach. Annu Rev Microbiol. 1986, 40: 337-365. 10.1146/annurev.mi.40.100186.002005.View ArticleGoogle Scholar
  7. Olmos J, Paniagua J, Contreras R: Molecular identification of Dunaliella sp. utilizing the 18S rDNA gene. Lett Appl Microbiol. 2000, 30: 80-84. 10.1046/j.1472-765x.2000.00672.x.View ArticleGoogle Scholar
  8. Olmos-Soto J, Paniagua-Michel J, Contreras PR, Trujillo L: Molecular identification of beta carotene hyper-producing strains of Dunaliella from saline environments using species-specific oligonucleotides. Biotech Lett. 2002, 24: 365-369. 10.1023/A:1014516920887.View ArticleGoogle Scholar
  9. Raja R, Iswarya SH, Balasubramanyam D, Rengasamy R: PCR-identification of Dunaliella salina (Volvocales, Chlorophyta) and its growth characteristics. Microbiol Res. 2007, 162: 168-176. 10.1016/j.micres.2006.03.006.View ArticleGoogle Scholar
  10. Olmos J, Ochoa L, Paniagua-Michel J, Contreras R: DNA fingerprinting differentiation between beta carotene hyperproducer strains of Dunaliella from around the world. Saline Systems. 2009, 5: 5-10.1186/1746-1448-5-5.View ArticleGoogle Scholar
  11. Coleman AW, Suarez A, Goff LJ: Molecular delineation of species and syngens in volvocacean green algae (Chlorophyta). J Phycol. 1994, 30: 80-90. 10.1111/j.0022-3646.1994.00080.x.View ArticleGoogle Scholar
  12. Coleman AW, Mai JC: Ribosomal DNA ITS-1 and ITS-2 sequence comparisons as a tool for predicting genetic relatedness. J Mol Evol. 1997, 45: 168-177. 10.1007/PL00006217.View ArticleGoogle Scholar
  13. González MA, Gómez PI, Montoya R: Comparison of PCR-RLFP analysis if the ITS region with morphological criteria of various strains of Dunaliella. J Appl Phycol. 1999, 10: 573-580. 10.1023/A:1008035422784.View ArticleGoogle Scholar
  14. González F, Coleman AW, Gómez PI, Montoya R: Phylogenetic relationship among various strains of Dunaliella (Chlorophyceae) based on nuclear ITS rDNA sequences. J Phycol. 2001, 37: 604-611. 10.1046/j.1529-8817.2001.037004604.x.View ArticleGoogle Scholar
  15. Gómez P, Gonzaléz M: Genetic polymorphism in eight Chilean strains of the carotenogenic microalga Dunaliella salina Teodoresco (Chlorophyta). Biol Res. 2001, 34: 23-30. 10.4067/S0716-97602001000100012.View ArticleGoogle Scholar
  16. Wilcox LW, Lewis LA, Fuerst PA, Floyd GL: Group I introns within nuclear-encoded small-subunit rRNA gene of three green algae. Molec Biol Evol. 1992, 9: 1103-1118.Google Scholar
  17. Paquin B, Shub DA: Introns: Group I Structure and Function. 2001, Encyclopedia of Life Sciences, Nature Publishing Group, LondonGoogle Scholar
  18. Dujon B: Group I introns as mobile genetic elements: facts and mechanistic speculations. Gene. 1989, 82: 91-114. 10.1016/0378-1119(89)90034-6.View ArticleGoogle Scholar
  19. Johansen S, Muscarella DE, Vogt VM: Insertion elements in ribosomal DNA. Ribosomal RNA: structure, evolution, processing and function in protein biosynthesis. Edited by: Zimmermann RA, Dahlberg AE. 1996, CRC Press, 89-110.Google Scholar
  20. Hibbett DS: Phylogenetic evidence for horizontal transmission of Group I introns in the nuclear ribosomal DNA of mushroom-forming fungi. Mol Biol Evol. 1996, 13: 903-917.View ArticleGoogle Scholar
  21. National Center for Biotechnology Information: [http://www.ncbi.nlm.nih.gov/nuccore/63029919]
  22. Hejazi MA, Wijffles RH: Effect of light intensity on b-carotene production and extraction by Dunaliella salina in two-phase bioreactors. Bio Eng. 2003, 20: 171-175.Google Scholar
  23. Sambrook J, Fritsch EF, Maniatis T: Molecular Cloning: A Laboratory Manual. 1989, Cold Spring Harbor, Cold Spring Harbor Laboratory PressGoogle Scholar
  24. Hejazi MA, de Lamarliere C, Rocha JMS, Vermue M, Tramper J, Wijffels RH: Selective extraction of carotenoid from the alga Dunaliella salina with retention of the viability. Biotechnol Bioeng. 2002, 79 (1): 29-36. 10.1002/bit.10270.View ArticleGoogle Scholar

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© Hejazi et al; licensee BioMed Central Ltd. 2010

This article is published under license to BioMed Central Ltd. This is an Open Access article distributed under the terms of the Creative Commons Attribution License (http://creativecommons.org/licenses/by/2.0), which permits unrestricted use, distribution, and reproduction in any medium, provided the original work is properly cited.