Open access peer-reviewed chapter

Phytoremediation of Arsenic Contaminated Water Using Aquatic, Semi-Aquatic and Submerged Weeds

Written By

Dibakar Roy, Dasari Sreekanth, Deepak Pawar, Himanshu Mahawar and Kamal K. Barman

Submitted: 07 June 2021 Reviewed: 17 June 2021 Published: 07 August 2021

DOI: 10.5772/intechopen.98961

From the Edited Volume

Biodegradation Technology of Organic and Inorganic Pollutants

Edited by Kassio Ferreira Mendes, Rodrigo Nogueira de Sousa and Kamila Cabral Mielke

Chapter metrics overview

393 Chapter Downloads

View Full Metrics


Arsenic (As) is the one the most toxic element present in earth which poses a serious threat to the environment and human health. Arsenic contamination of drinking water in South and Southeast Asia reported one of the most threatening problems that causes serious health hazard of millions of people of India and Bangladesh. Further, use of arsenic contaminated ground water for irrigation purpose causes entry of arsenic in food crops, especially in Rice and other vegetable crops. Currently various chemical technologies utilized for As removal from contaminated water like adsorption and co-precipitation using salts, activated charcoal, ion exchange, membrane filtration etc. are very costly and cannot be used for large scale for drinking and agriculture use. In contrast, phytoremediation utilizes green plats to remove pollutants from contaminated water using various mechanisms such as rhizofiltration, phytoextraction, phytostabilization, phytodegrartion and phytovolatilization. A large numbers of terrestrial and aquatic weed flora have been identified so far having hyper metal, metalloid and organic pollutant removal capacity. Among the terrestrial weed flora Arundo donax, Typha latifolia, Typha angustifolia, Vetivaria zizinoids etc. are the hyper As accumulator. Similarly Eicchornea crassipes (Water hyacinth), Pistia stratiotes (water lettuce), Lemna minor (duck weed), Hyrdilla verticillata, Ceratophyllum demersum, Spirodella polyrhiza, Azola, Wolfia spp., etc. are also capable to extract higher amount of arsenic from contaminated water. These weed flora having As tolerance mechanism in their system and thus remediate As contaminated water vis-à-vis continue their life cycle. In this chapter we will discuss about As extraction potential of various aquatic and semi aquatic weeds from contaminated water, their tolerance mechanism, future scope and their application in future world mitigating As contamination in water resources.


  • Arsenic
  • Phytoremediation
  • Weed

1. Introduction

Arsenic (As) is the one the most toxic element present in earth which poses a serious health hazard to animal and human health. Generally arsenic is present in the earth crust in the form minerals, especially associated with iron pyrite and zinc ores. Arsenic contamination occurs through both by natural as well as anthropogenic processes [1]. Unlike other toxic heavy metals (Cadmium, mercury and chromium) arsenic contamination in environment predominately occurs through natural biogeochemical process [2] and some manmade activities play important role (triggering the process) in that process. Anthropogenic activities such as coal mining and burning smelting of As containing metal ores and other industrial activities are also responsible for distribution of arsenic in the environment [3]. Arsenic contamination of drinking water in South and Southeast Asia reported one of the most threatening problems that causes serious health hazard of millions of people of India and Bangladesh [4]. The source of As contamination in water in those countries were due to two different natural processes; oxidation of arsenopyrite minerals lies below ground water table due to water mining process and reduction of As containing iron hydroxides [5]. Arsenic exists in the nature in −3, 0, +3 and + 5 oxidation states and environmental forms include arsenious acids, arsenic acids, arsenites, arsenates, methylarsenic acid, dimethylarsinic acid, arsine, etc. Two inorganic forms are very common in natural waters: arsenite (AsO33−) and arsenate (AsO43−), referred to as arsenic (III) and arsenic (V). Pentavalent (+5) or arsenate species are AsO43−, HAsO42−, H2AsO4 while trivalent (+3) arsenites include As(OH)3, As(OH)4−, AsO2OH2− and AsO33−. The solubility of inorganic species depends on pH and redox potential of the environment and arsenite (As3+) is the most soluble form inorganic As. Pentavalent species or arsenate (As5+) predominate in oxygen rich aerobic environments, where as trivalent arsenites (As3+) dominant in moderately reducing anaerobic environments such as groundwater [4].

Arsenic concentration in drinking water reported more than 50 μg L−1 in many areas in the world [6], whereas maximum permissible limit set by World Health Organization (WHO) is 10 μg L−1. The use of arsenic contaminated ground water for irrigation purpose causes build up of As in soil and leads to entry of As in food crops, especially in rice and vegetables [7, 8]. This causes serious health hazard, in those As containing areas. In Southeast Asian countries like Bangladesh, Eastern parts of India (West Bengal and Bihar) and Vietnam, rice is consumed as major staple food and is very efficient in As translocation in grains [9]. Thus rice crop play a major pathway for As entry in human body living in those contaminated areas apart from drinking water. Thus remediation of arsenic contaminated water is important for environmental point of view. Various technologies are for remediation of arsenic contaminated water like ion exchange, electro dialysis, membrane filtration, adsorption and coagulation-flocculation generates lot of arsenic enriched waste. That waste material generally dumped or disposed in nearby surroundings, from where arsenic can also come back to soil and water by leaching thus making system susceptible to arsenic contamination. Along with above mentioned problem, huge cost is involved in this existing arsenic remediation technology. That necessitates finding out an alternate low cost technology which can take care of arsenic contaminated water.

Phytoremediation is an alternate and low cost technology that utilizes green plant to extract arsenic from water and store it vegetative cells. Phytoremediation process includes phytoextraction, phytostabilization, phytovolatilization, phytotransformation, and rhizofiltration [10]. Researchers find out that plants uptake arsenic by roots through phosphate uptake pathway and transfer it their above ground parts (shoot and leave). But how much amount of arsenic translocated from source (water) to sink (plant parts) depends on phytoremediation efficiency of the plant concern. However, more than 90% of total arsenic accumulated into the plant is stored in roots.

The plants utilized for phytoremediation have some criteria like (1) plant have higher specific growth rate under contaminated environment, (2) higher translocation capability of the toxic element concerned [11]. Metal translocation capability depends on factors like (1) bio concentration factor (BCF) and (2) translocation factor (TF). Plants having BCF >1 are ideal for Phytoremediation. Chinese brake fern (Pteris vittata) is the most promising plant for phytoremediation of arsenic from contaminated soil [12]. For instance, plants species like water hyacinth (Eichhornia crassipes), duck weed (Lemma minor, Spirodela polyrhiza and Wolfia globosa), water lettuce (Pistia stratiotes) and fern (Azolla pinnata) have been successfully utilized for arsenic removal from water purpose by many researchers [13, 14, 15]. Among the semi aquatic weeds. Apart from these free floating aquatic weed flora such as Arundo donax, Vetivaria sp., and Alternanthera philoxeroides had been successfully utilized for remediation of As contaminated water [16, 17]. In this chapter we are going to discuss about arsenic removal potential of various aquatic and semi aquatic weeds along with their future use for phytoremediation purpose.


2. Phytoremediation pathways

The terminology “Phytoremediation” consists of two words, “Phyto” means “green plants” and “remediation” means “curative measures or restoration”. The word “phytoremediation” was first given by Chaney [18]. In phytoremediation process, generally green plants are used which uptake toxic chemical substances (such as heavy metals and metalloids, pesticide residues etc.) from contaminated sites (soil and water) by various mechanisms and remove them from environment. Various crop and weed plants are found to be suitable for phytoremediation purpose. But research results indicated that weed flora had higher phytoremediation potential than cultivated crops (Example- Brassica sp). There are various pathways of phytoremediation process such as, rhizofiltration, phytoaccumulation or phytoextraction, phytostabilization, phytodegradation or phytotransformation and phytovolatilization etc.

  • Rhizofiltration: Plants uptake toxics substances by their roots through adsorption or absorption process and sequester in their root system. Aquatic plants mainly exhibited this process.

  • Phytoaccumulation or phytoextraction: Plants uptake toxic substances by their root system and translocated to other plant parts such as stem and leave or other modified plant parts. This mechanism mainly exhibited this process are suitable for remediation of contaminated soil.

  • Phytostabilization: In this process, plants restrict movement of toxic substances in soil or water, thus reduced their availability to plants. In this method, plants do not uptake toxic substances from environment. Rather, plants secrets some root exudates or photochemicals which form stable chemical bond with toxic substances and increases its stability in environments.

  • Phytodegradation or Phytotransformation: In this process, plants uptake toxic substance from soil or water and degrade these primary toxic substances into nontoxic forms. A large number of metabolic and physiological factors are involved in this process.

  • Phytovolatilization: Plant uptake toxic substances by their root system and translocated to their aerial plant parts especially in leaves; and release toxic substances in the form of vapor which may not be toxic as their primary source.

Apart from this there are some other terminologies often used in phytoremediation process are bioconcentration factor (BCF) and translocation factor (TF).

BCF = toxic substance uptake by plant/toxic substance present in environment (soil or water).

TF = toxic substance present in shoot or stem/toxic substance present in roots or.

Toxic substance present in leaves/Toxic present in shoot or stem.

For, Hyper accumulator plants both BCF and TF is >1 is desired. In other words, plants suitable for phytoremediation, BCF >1 is always desirable. But for aquatic weeds, as their dominant pathways is rhizofiltration; their toxic substances BCF >1 but TF for root to shoot or shoot to leaves is <1.


3. Potential of various aquatic plants for phytoremediation

3.1 Phytoremediation by free floating aquatic weeds

Eichhornia crassipes:Eichhornia crassipes is commonly known as water hyacinth, a free-floating perennial aquatic plant native to tropical and sub-tropical South America, and is now wide spread in all tropic climates. The genus Eichhornia comprises seven species of water hyacinth among which E. crassipes is the most common and have been reported to grow very first. However, its enormous biomass production rate, high tolerance to pollution and absorption capacity of heavy-metal and nutrient qualify it for use in wastewater treatment [19].

The capability of removing arsenic from contaminated water was earlier observed by Misbahuddin and Fariduddin [20] and they observed that water hyacinth can removes arsenic from water within 3–6 hr. exposure time. Amount of arsenic removed depends on number of the plant used, exposure time, presence of air and sunlight. They concluded that whole plants were more effective than fibruous roots alone. It was observed that dried roots of water hyacinth can rapidly reduces As content in contaminated water within below WHO recommended critical level (<10 μg Lg−1) [21]. A fine powder was prepared from dried roots of water hyacinth plants (obtained from Dhaka, Bangladesh) removed more than 93% arsenite and 95% of arsenate from a solution containing As @ 200 μg L−1 within 1 hr. exposure time [21]. Higher biomass production ability of water hyacinth allow it to remove As at higher rate (600 mg As ha−1 day−1) and greater efficiency (17%) compared to lower biomass producing aquatic macrophytes such as lesser duck weed (Lemna minor) which removed As at lower rate (140 mg As ha−1 day−1) and lesser efficiency (5%); though there was no difference in bioaccumulation capacity [13]. Similarly better As extraction capacity of water hyacinth (80%) compared to Lemna minor and Spirodella Polyrhiza from tropical coalmine effluent was also been reported [22] from India. Unlike lower biomass producing aquatic macrophytes, water hyacinth poses better As extraction ability compared to higher biomass producing vetivar grass [23]. Not only higher biomass, higher reproduction ability also plays an important role in As phytoremediation by water hyacinth. Water hyacinth was a suitable phytoremediation agent when As present in contaminated water at lower concentrations. When As was provided at lower concentrations @ 1 and 2 mg L−1, water hyacinth removed 90 and 65% of total As from contaminated solutions (1 and 2 mg L−1 respectively) provided respectively within 7 days [24] and maximum As stored in roots. Water hyacinth can extract higher amount As from contaminated water but their presence in water bodies reduces dissolved oxygen content (DOC), which makes its application for a larger water bodies a problematic pathway which needs to be taken care.

Pistia stratiotes: Pistia stratiotes is commonly called as water lettuce There are many previous studies indicated that Pistia stratiotes capable of removing toxic heavy metals from contaminated water [25, 26, 27], but there were few studies was done on As uptake by water lettuce. Earlier a field study carried out using P. stratiotes and results showed that Pistia stratiotes can remove As from contaminated water, along with higher bioconcentration factor (BCF) for root (8632) vis-à-vis lower BCF for leaf (2342) [28]. In a laboratory study it was demonstrated that maximum As removal efficiency of P. stratiotes was found at pH 6.5 and Pistia removed 87.5% of the metalloid provided in the solution [29]. From Laboratory study it was revealed that P. stratiotes can accumulate As efficiently when As was provided at lower concentrations, though total As uptake was increased with increase in As concentration in the solution [30]. Arsenite accumulation in P. Stratiotes was found more in root and less in leaves like water hyacinth. Arsenic accumulation in roots and leaves were respectively 1120 and 31.60 μg g−1 DW respectively when 10 μM As (As3+) solutions are employed [31]. When higher concentration of As solutions used (>20 μM), As toxicity symptoms like chlorosis, suppressed growth, lower photosynthetic rate, suppressed enzymatic activities and increased cell damage were observed in P. stratiotes [30, 31].

Lemna, Spirodella and Wolfia: Weeds belongs to Lemna, Spirodella and Wolfia are generally known as Duckweeds. Duckweeds are small free-floating aquatic weed plants which generally found in water bodies, mainly comprises of four genera, Lemma, Spirodela, Wolfia, and Wolfiella, and of 34 species. Among these Lemna, Spirodela, and Wolfia have been widely reported to accumulate arsenic from contaminated water [13, 32, 33, 34]. Research studies indicated that, total As accumulation in Lemna gibba was more in field condition compared to laboratory conditions due to higher exposure time in field condition [32]. However higher accumulation of As in plant parts is not always correlated with bio-concentration factor (BCF). It was found that total As accumulation plant parts may be higher in field condition, but higher BCF was obtained at laboratory conditions [32] due to better availability of external nutrients.

However nutrients like phosphate addition may suppressed As uptake by duckweeds as both phosphorus and arsenic belongs same group-V(b) element family in periodic table [33]. In most of the phytoremediation study carried out in laboratory condition, As is provided either in the form of arsenite (As3+) or arsenate (As5+). But some studies included dimethyl arsenic acid (DMAA), an organic form of arsenic for evaluation of As phytoremediation potential of duckweed species. In a lab study, Spirodela polyrhiza was exposed to two forms of As species, arsenate and DMAA with concentrations ranged from 1, 2, and 4 μM and their interaction with phosphate (100 to 500 μM) was studied [33]. Results obtained showed that arsenate uptake was affected by higher phosphate concentrations whereas DMAA uptake was not influenced by phosphate concentration indicating that Spirodela polyrhiza had separate mechanisms for DMAA uptake. Duckweeds showed contrasting As uptake behavior when provided in two separate inorganic forms (As5+ vs. As3+) and maximum As uptake was reported with arsenite form (As3+) [34]. Spirodela polyrhiza extracted 17408 and 8674 μg g−1 As (dry weight basis) respectively from solutions containing As in the form of As3+ and As5+ (64 μM As each) respectively within 6 days [34]. Maximum amount of As extracted by duckweeds is still questionable and it is varied with As exposure time, concentrations of As in contaminated solution, and research type (laboratory vs. field study). Spirodela polyrhiza reported to uptake 400 mg kg−1 As (dw basis) without showing any toxicity symptoms, but can accumulate up to 900 mg kg−1 As (dw basis) when subjected to 320 μM ml−1 As containing solutions [35]. Under natural condition, Lemna minor was found to accumulate 430 mg kg−1 As (dry weight basis) under As contaminated environment [36]. There are few studies on As uptake by Wolfia globosa (rootless duckweed). Wolfia globosa had been reported to extract more than 1000 mg kg−1 (frond dry weight basis) from contaminated water [37]. Like other duckweeds, Wolfia globosa also uptake more arsenite form compared to arsenate form [37]. Later studies confirmed that Wolfia globosa produced phytochelatins which played an important role minimizing toxic effects of As in their body parts [38]. These above cited studies showed that Lemna minor, Spirodela polyrhiza and Wolfia globosa are suitable for phytoremediation of As from contaminated water.

Salvinia: Salvinia is a floating fern belongs to genus salviniaceae, commonly called as butterfly fern. The genus salviniaceae contains 12 different species, out of them only 3 had been investigated for As phytoremediation were namely Salvinia molesta, Salvinia minima and Salvinia natans [39, 40, 41]. Salvinia minima have been reported as an efficient scavenger of Pb (34 mg g−1 dw) and less efficient remover of As (0.05 mg g−1) from contaminated medium and uptake of both Pb and As increased with exposure time duration and concentration of the element in the medium concerned [40]. The plant showed toxicity symptoms when As3+ concentration was more than 100 μM and tolerates up to 300 μM. Addition of phosphate in solution, reduced As uptake of as occurred in other aquatic weed plant also been recorded in their study. Similarly negative impact of phosphate and iron on As uptake by Salvinia natans was observed [41]. Phosphate addition reduced As uptake when provided in the from arsenate (As5+), in contrast no impact when As was provided in the form of DMAA. Like other aquatic weeds (Eicchornia, Pistia and Spirodela), Salvinia molesta also showed As toxicity upon exposure to higher concentration. To counter As stress, antioxidant enzyme activities and reactive oxygen species (ROS) were increased in floating leaves [39]. These studies indicated that Salvinia can play an important role for As phytoremediation as it had own defense mechanism.

Azolla: Azolla is a small, free floating aquatic fern commonly found in paddy fields, ponds, river and lakes. There are numerous studies carried out globally showed that Azolla can remediate heavy metal toxicity from contaminated water [42, 43, 44]. But studies on As phytoremediation capability of azolla were scarce. In As contaminated area of Bangladesh, Mahmud et al. [45] evaluated 49 different plant species for As uptake and BCF; found that Azolla pinnata along with Eichhornia crassipes and Spirodella polyrhiza showed higher BCF and TF in paddy field. Among 49 plant species, Azolla pinnata showed highest BCF 10.92 indicated its suitability to reduce As uptake by paddy plants in field condition. A study using Azolla conducted in China using 50 different strains of Azolla spp. based on their uptake and speciation [46]. As uptake was ranged from 29 to 397 mg kg−1; A. caroliniana accumulated maximum As followed by A. macrophylla and minimum accumulation was associated with A. filiculoides when all strains were grow in 50 μM As5+ solution for 10 days (Figure 1). Arsenic speciation in followed in the order of arsenate (As5+) > arsenite (As3+) > DMAA and MMAA accounting 50–60, 25–40 and 1–5% of total arsenic in A. caroliniana respectively. In contrast, asrenite (As3+) was dominant As species in A. filiculoides governs 55–69% of total As [46]. Another study was conducted on phytoremediation of As by A. caroliniana wild using various As concentrations (0, 0.25, 0.5, 1.0 and 1.5 mg L−1) and impact of As exposure on plant enzymatic properties were investigated [47]. Maximum As uptake (386 mg kg−1) was reported at highest As concentration (1.5 mg kg−1). It was observed that peroxidases, glutathione reductase, catalase and superoxide dismutase activities were enhanced at lower As doses and reduced at higher doses. In exposure to higher As concentration, thiol content and anthocyanin production were increased and correlated with higher As uptake.

Figure 1.

Arsenic uptake pattern in different Azolla sp. (adapted from Zhang et al., 2009).

3.2 Phytoremediation of arsenic by semi aquatic weeds

Some semi aquatic weed such as Alternathera philoxeroides, Arundo donax, Vetivaria Zizinoids, Typha latifolia, Phragmites spp. and Canna spp. had been widely reported to accumulate As in their body parts from contaminated soils and water [16, 17, 48, 49, 50, 51]. Alternanthera philoxeroides had potential to extract As from contaminated water and stored in root system [52, 53]. Reports from previous studies indicates that As accumulation in A. philoxeroides followed in the order of root > stem > leaf and average BCF for root ranged from 106 to 191, when exposed to various doses of As containing solutions (1, 2 and 5 mg kg−1) under laboratory condition [52]. Under natural condition, Alternanthera philoxeroides observed to uptake 12.94 mg kg−1 total As dw from pulp paper industry water with average BCF- 3.58 and TF-0.51 [53]. Higher BCF under laboratory condition observed due to used of higher As containing solution and availability of external nutrients for weed plants which may trigger As uptake through phosphate uptake pathway.

Arundo donax is a perennial semi aquatic weed mostly found in submerged condition offer a tremendous potential to uptake As from contaminated water. Earlier research work showed that Arundo donax can grow efficiently up to 50–600 μg L−1 As concentration without showing any toxicity symptom and maximum As uptake, BCF (15), TF (4.93) were recorded at 600 μg L−1 [16]. Toxicity symptoms appeared when plants were exposed to solutions containing 1000 μg L−1 As [16]. Further, combined use of plant growth promoting rhizobacteria (PGPR) such as Stenotrophomonas maltophilia and Agrobacterium sp. increased bioaccumulation of As in roots of Arundo donax plant upon exposure to higher concentration As (20 mg kg−1) and enhanced overall phytoremediation efficiency of Arundo donax in presence of PGPR bacteria [51]. The As accumulation in Phragnites austratlis followed in the order of roots > rhizomes > leaves and maximum total As uptake was registered 32.5 mg kg−1 [54].V. zizinoids, another semi aquatic weed reported to be capable of extracting As from contaminated water [17, 55]. In a hydroponic study (21 days), root to shoot As uptake it was increased with increase in As concentrations by V. zizinoids can uptake [17]. The BCF and TF for As were 10 and 0.86 indicates that V. zizinoids was an As hyper accumulator and stored higher proportion of As in their root system. Combined use of arbuscular mycorrhizal fungi (Glomus spp.) enhanced As uptake capability and growth of vetivar grass (Chrysopogon zizanioides) [55]. Typha latifolia also had the potential to uptake higher proportion of As from contaminated environment (soil), but most of the studies conducted using Typha latifolia were focused in soil. Most of the studies showed that semi aquatic weeds store more As in their root system and lower in upper vegetative parts. Higher plant vigor, higher As extraction capacity and perennial nature make them suitable phytoremediation agent for constructed wetland system. Combined use of submerged weeds like Hydrilla, Ceratophyllum, Potamogeton along with semi aquatic weeds (Arundo donax, Vetivaria zizinoids, Phragmites spp. and Typha sp.) and PGPR like VAM, As oxidizing bacteria may be highly useful to treat and remediate As contaminated water in constructed wetland system. Semi aquatic weeds are highly efficient when As present in higher concentrations and when As concentration in the system become lower submerged weeds come to play their role, as they are highly efficient As remover at lower concentrations. Again use PGPR will increase overall phytoremediation efficiency. Future research may be undertaken in these aspects for better information and output.

3.3 Phytoremediation by submerged aquatic weeds

Among the submerged aquatic weeds Hydrilla verticillata, Ceratophyllum dermersum, Potamageton crispus, Valisnaria natans, Eleocharis acicularis and Elodea Canadensis widely reported by many researchers to extract As from contaminated water. Studies conducted in laboratory and field conditions indicated that Hydrilla verticillata, and Ceratophyllum demersum can uptake higher proportion of As from contaminated water depending on exposure time and concentration of metalloid [22, 56, 57]. Unlike Spirodela polyrhiza, Hydrilla verticillata also uptake more arsenite (As3+) form rather arsenate (As5+) form [50]. Under simulated field condition (aquatic pond) Hydrilla verticillata alone removed sum total 8546 μg (348 μg g−1) of As from contaminated water (As concentration 1500 μg L−1) which is 72% of the total arsenic supplied [56]. Ceratophyllum demersum reported to accumulate 76 μg g−1 in 4 days and and As accumulation further increased to 201 μg g−1 in 7 days when exposed to 50 μM As solutions [22]. Maximum As accumulation by Ceratophyllum was recorded 525 μg g−1 dw when subjected to with 250 μM As5+ solution for 7 days [22]. Uptake of As by Ceratophyllum demersum depends on species of As present (As3+ vs. As5+) and pH of the medium. Maximum uptake of As3+ by Ceratophyllum was reported at pH 6.5 [58]. This variation in selective uptake of As species largely depends on uptake pathways and plant metabolism.

In natural conditions, submerged weeds grow in water bodies in association with floating macrophytes. Use of Combinations of submerged and floating weeds found more effective for phytoremediation purpose than submerged and floating weeds alone. Research work carried out using Hydrilla, Certophyllum, lemna and Wolfia at various combinations showed that Ceratophyllum + lemna combination (3326 μg) combination removed maximum total As followed by Hydrilla + Wolfia (1896 μg) (Figure 2). When the contribution of single plant considered, contribution of Hydrilla is more than 50% [56]. Arsenic phytoextraction potential of five different submerged weeds namely Ceratophyllum dermersum, Potamageton crispus, Myriophyllum spicatum, Hydrilla verticillata and Vallisneria natans were compared under natural As contaminated environement [59]. Results showed that all plants accumulated more 1000 mg kg−1 dw As; highest and lowest As accumulation and BCF were associated with Vallisneria natans (BCF- 361) and Ceratophyllum dermersum (BCF- 221) [59]. Similarly ability of potamogeton spp., Myriophyllum spp. and Valisnaria app to uptake As from contaminated water were also been reported by many authors [60, 61, 62]. Arsenic uptake by various types of aquatic, semi-aquatic and submerged weeds has been outlined in Table 1.

Figure 2.

Arsenic uptake comparison between various weed plants (Hydrilla, Ceratophyllum, Wolffia, Lemna and Eicchornia) grown in singly or in various combinations upon arsenic exposure for 30 days (adapted from Srivastava et al., 2014).

Name of the plantsKey findingsReference
Eichhornia crassipesRemoved 600 mg As ha−1 day−1 within 21 days with 18% removal efficiency when As was applied @ 0.15 mg L−1[13]
Lemna minorRemoval rate 140 mg As ha−1 day−1 within 21 days with 5% removal efficiency when As was applied @ 0.15 mg L−1[13]
Removed relatively higher As3+ (17408 μg g−1) and lower As5+ (8674 μg g−1As) from As containing solutions (64 μM As each)[35]
Pistia stratiotesAccumulates 1120 μg g−1 As in roots and 31.60 μg g−1 As in leaves (dry weight basis) from 10 μM As containing solution[31]
Salvinia natansAccumulates 50 μg g−1 As in roots[41]
Hydrilla verticillataRemoved sum total 8546 μg (348 μg g−1) of As from contaminated water (As concentration 1500 μg L−1)[49]
Ceratophyllum demersumAccumulates 525 μg g−1 (dry weight baisis) from 250 μM As5+ solution for 7 days[22]
Potamogeton crispusAccumulates 1000 mg kg−1 (dry weight basis) from As contaminated environment[52]
Myriophyllum spicatumAccumulates 1000 mg kg−1 (dry weight basis) from As contaminated environment[52]
Vallisnaria natansAccumulates 1000 mg kg−1 (dry weight basis) from As contaminated environment[52]
Alternanthera philoxeroidesExtract 12.94 mg kg−1 total As (dry weight basis) from pulp paper industry effluents[61]
Arundo donaxAccumulates As at the rate 9 mg kg−1 with TF = 4.93 and BF = 15.00 for the arsenic containing solution 600 μg L−1.[16]
Phragnites austratlisAccumulates 32.5 mg kg−1 As in root[62]

Table 1.

Phytoremediation ability of various aquatic and semi aquatic weeds.


4. Mechanisms of arsenic uptake and detoxification in aquatic weeds

4.1 Mechanisms of arsenic uptake in aquatic macrophytes

Three pathways for arsenic uptake in marine macrophytes have been described – (i) active uptake through phosphate uptake transporters, (ii) passive uptake through aquaglyceroporins, and (iii) physicochemical adsorption on root surfaces. Plants mainly uptake As(V) through phosphate uptake transporters [63, 64]. As(III), DMAA and MMAA gets into the plants by passive mechanism through the aquaglyceroporin channels [64].

4.1.1 Active uptake through phosphate uptake transporters

As(V) and phosphate are chemical analogs, and compete for uptake carriers in the plasmalemma [65]. As a result, as the phosphate content rises, more As (V) is required to be desorbed in the solution. Mkandawire and Dudel. [32] and Rahman et al. [33] showed that As (V) is taken up by aquatic plants through the phosphate uptake pathway, it competes with phosphate for uptake in tissues of L. gibba L. and S. polyrhiza L.

4.1.2 Passive uptake through aquaporins/aquaglyceroporins

Physiological studies indicate that these arsenic species are transported in rice through aquaporins /aquaglyceroporins via passive uptake mechanisms [66, 67]. Molecular studies revealed that Nodulin26-like intrinsic membrane proteins (NIPs), one of the major subfamilies of aquaporins transporters that promote the transport of neutral molecules like water, glycerol, and urea, are responsible for transporting As(III) into rice roots [68]. Aquaporins and aquaglyceroporins are two of three subfamilies of water channel proteins (WCPs), the transmembrane proteins that have a specific three-dimensional structure with a pore that permeates water molecules [69], which are permeable to water, glycerol, and/or other small, neutral molecules. Glycerol and As(III) compete for uptake in rice (Oryza sativa L.), indicating that this arsenic species is carried via the plasma membrane by aquaporins/ aquaglyceroporins [67].

4.1.3 Physicochemical adsorption on root surfaces

Arsenic is adsorbing and accumulating on the surfaces of aquatic plants due to suspended iron oxides (Fe-plaque). Robinson et al. [70] discovered a strong association between arsenic and iron concentrations in aquatic plants, which is believed to be due to arsenic adsorption on plant surfaces’ iron oxides. Rahman et al. [14] investigated arsenic species adsorption on precipitated iron oxides on S. polyrhiza L. roots/fronds and revealed a strong association between arsenic and iron concentrations in tissues when the plant was exposed to As (V). There was no association between arsenic and iron in plant tissue when S. polyrhiza L. was exposed to As (III), DMAA, and MMAA.As (V) is primarily adsorbed on precipitated iron oxides on the roots of aquatic plants and deposited by a physicochemical adsorption process, according to the findings.

4.2 Arsenic metabolism and detoxification in aquatic macrophytes

Arsenic occurs primarily as As (V) in an oxic environment and as As (III) in a reduced environment [64]. In plants, As (V) and phosphate share the same transporter, while As(III) enters plant cells through NIPs’aquaporins [57, 64]. Because of their distinct molecular properties, these two types of arsenic elicit different biochemical responses in aquatic plants [71]. As (V) has no affinity for thiol ligands, while As(III) has a strong affinity for peptides with sulfhydryl (-SH) groups, such as glutathione (GSH) and phytochelatins (PCs) [64, 72]. Even though plants had been exposed to As, arsenic speciation in plant tissues indicates that arsenic is primarily present in the As(III) oxidation state (V).This suggests that As(V) is effectively reduced to As(III) in plant cells after uptake, and that most plants have high As(V) reduction competence [64]. The reduction of As(V) to As(III) is mediated by GSH [73] and by enzyme [74], which is thought to be a detoxification mechanism of the plants. As(V) and As(III) have been shown to generate reactive oxygen species (ROS) within cells when they are taken up [75], and plants counteract the generation of ROS by various enzymes and cellular compounds [76]. The GSH can act as an antioxidant and is required for the synthesis of Phytochelatins which are required for metalloid chelation [71].

The mechanism of arsenic accumulation and detoxification was studied by many others in aquatic plant H. verticillata [57, 71]. In the presence of As (III) or As(V), H. verticillata enhanced the biosynthesis of thiols such as PCs, and increased antioxidant enzyme activity. Although the levels of thiolic compounds such as NP-SH, cysteine, GSH, and oxidized glutathione (GSSG) were significantly enhanced in H. verticillata upon exposure to both As(III) and As(V), As(III) was found to enhance the activities of cysteine synthase and c-glutamylcysteine synthetase and the amount of cysteine and GSH to higher levels than As(V) . The analysis of PCs indicates that the accumulation of PC1 and PC2 in H. verticillata was enhanced with the increase of both As(III) and As(V) concentrations [71]. Thus, during As (III) and As(V) stress, phytochelatins and antioxidant systems in H. verticillata react differently, which is considered to be the plant’s detoxification mechanism.


5. Biotechnological interventions for phytoremediation

Plants have been utilized for phytoremediation of toxic metals and metalloids, however due to heavy metal phytotoxicity to plants; this process has been slow and largely rendered ineffective [77]. Natural heavy metal hyperaccumulators are also available, however, they are limited to specific geo-climatic conditions and also lack the crucial biomass required for efficient phytoremediation. Phytoremediation has a lot of potential using genetic engineering technologies to improve plant tolerance and heavy metal accumulation. Furthermore, various new studies using omics technologies such as genomics, transcriptomics, proteomics, and metabolomics to elucidate the genetic determinants and pathways involved in heavy metal and metalloid tolerance in plants have been identified. Presently there are three main biotechnological approaches for the phytoremediation of heavy metals and metalloids are currently being used to engineer plants for phytoremediation of heavy metals and metalloids: (1) manipulating metal/metalloid transporter genes and uptake systems; (2) enhancing metal and metalloid ligand production; (3) conversion of metals and metalloids to less toxic and volatile forms [78] (Figure 3).

Figure 3.

Potential biotechnological strategies for phytoremediation. Heavy/toxic metals can be mobilized and transported (influx) into roots through plasma membrane transporters. They can then be transported (efflux) out of the roots into the xylem and translocated into the shoots. At this stage, plant tolerance to toxic elements may be enhanced through manipulation of influx/efflux transporters or by increasing the levels of ligands/chelators. Volatilization of the toxic elements can be achieved through enzymes that modify these toxic elements. Chelators or efflux transporters can also be used to export the toxic elements out of the cytosol and into vacuoles or the cell wall. Adapted from Dhankher et al. (2011).

5.1 Manipulating metal/metalloid transporter genes and uptake system

Enhanced heavy metal tolerance and bioaccumulation has been attained in different plant species by genetic manipulation of metal transporter genes. For example, the overexpression of full length NtCBP4 (plasma membrane channel protein) in Nicotiana tabacum showed Pb2+ hypersensitivity and enhanced accumulation of Pb2+ in the genetically manipulated plants. However, the overexpression of a truncated version of NtCBP4 generated by deletion of its C-terminal, calmodulin- binding domain and part of the putative cyclic nucleotide- binding domain showed improved tolerance to Pb2+ and less accumulation of Pb2+ [79]. Nicotiana tabacum plants expressing CAX2 (calcium exchanger 2) gene accumulated more Ca2+, Mn2+ and Cd2+ and also showed enhanced tolerant to elevated Mn2+. It was also observed that overexpression of CAX2 gene in Nicotiana tabacum increased Mn2+ and Cd2+ transport in the root tonoplast vesicles in the transgenic plants [80]. Moreover, T-DNA mutants of the Arabidopsis CNGC1 (cyclic nucleotide- gated ion channel 1) gene, that encodes a homologous protein to NtCBP4, also showed Pb2+ hypersensitivity and enhanced accumulation of Pb2+ in the genetically manipulated plants. These findings suggest that NtCBP4 and AtCNGC1 play an important role in the transport pathway of Pb2+ [79, 81]. The overexpression of yeast YCF1 (Yeast Cadmium Factor 1) gene in Arabidopsis thaliana resulted in enhanced accumulated higher amounts and tolerance to Pb2+ and Cd2+ metals in plants [82].

Recent research findings have revealed arsenite is transported in plants by proteins belonging to the aquaporins [83, 84]. It is observed that in efficient arsenic hyperaccumulators such as Pteris vittata has highly well-organized system of arsenic translocation from root to shoot tissues [85, 86], However, most non-hyperaccumulators show low mobility rate compared to P. vittata, also variable Arsenic mobility rate is observed among different plant species, suggesting that it is controlled by genes. Arsenic loading to the xylem is a critical stage in arsenic translocation from root to shoot, however it is a poorly known mechanism. Ma et al. [87, 88] has identified and characterized Lsi2 gene encoding an efflux protein, plays an important role in loading arsenite into the xylem. Mutation in Lsi2 gene caused about 50% reduction in arsenic accumulation in the shoot. The Lsi2 gene is a homolog of the E. coli ArsB gene, an As (III)/H+ exchanger that confers bacterial arsenite tolerance [89].

Genome-wide gene expression analysis in Oryza sativa roots treated with different heavy metals and metalloids; As(V), Cr(VI), Pb, and Cd, showed numerous differentially expressed genes as well as unique genes. Various genes belonging to different transporter families were identified [90]. Recently Wang et al. [91], has identified genes for Cu tolerance in the Paeonia ostii with the help of de novo transcriptome sequencing approach. Such genes may further be transferred to crop plants for enhancing heavy metal tolerance. Therefore, strategies of developing transgenic plants for arsenic (As) phytoremediation include enhancing plant uptake for phytoextraction, decreasing plant uptake, improving the plants’ tolerance to As contamination, and increased methylation for enhanced food safety.

5.2 Enhancing metals and metalloids ligand production

Complexation of Arsenic with phytochelatins (PCs), or metallothionein (MTs) or glutathione (GSH) is an proficient way to detoxify As(III), since these complexes are sequestered in the vacuoles, this process is catalyzed by the homologs of multidrug resistance proteins (MRPs) [92, 93]. Enhancing the accumulation or synthesis of PCs and/or GSH and/or MTs may be one way to increase phytoremediation of arsenic. The overexpression of PCS in Brassia juncea enhanced its tolerance to arsenic but no significant increase arsenic accumulation was observed, this may be due to the fact that PC synthesis is also limited by the production of GSH [94]. The overexpression of AtPCS1 and GSH1genes, that encode g-glutamylcysteine synthetase (g-ECS), the rate-limiting step in GSH biosynthesis, individually in Arabidopsis thaliana increased both arsenic tolerance and as well as accumulation [95].

Arsenic (As) tolerance in plants can also be increased by modifying GSH and PCs. Dhankher et al. [96] transferred and co-expressed two bacterial genes, E. coli arsenate reductase (arsC) and γ-glutamylcysteine synthetase (γ-ECS), in Arabidopsis thaliana, the transgenic plants grown in the presence of 125 μM sodium arsenate accumulated threefold more arsenic in the aboveground biomass and showed almost 17-fold higher biomass than wild type WT plants. The overexpression of AtPCS1 under constitutive promoter in A. thaliana enhanced tolerance to arsenate but failed to enhance arsenic accumulation [97]. These studies showed that manipulation of genes for increasing the production of metal chelation agents hold great potential for improving heavy metal and metalloid tolerance and accumulation in plants.

The de novo transcriptome sequencing analysis in Raphanus sativus L. roots under cadmium stress was carried out to discover differentially expressed genes and microRNAs (miRNAs) involved in Cd-responsive regulatory pathways. Various candidate genes encoding PCs, GSHs, and MTs; and other genes belonging to zinc iron permease (ZIPs) and ABC transporters were identified [98]. Likewise, in de novo transcriptome analysis in radish roots under chromium stress, showed that 1561 unigenes down-regulated and 1424 unigenes were up-regulated, various transcription factors such as Chromium stress-responsive genes involved in chelate compounds, signal transduction and antioxidant biosynthesis were discovered [99]. Such candidate genes can further be transferred into the crop plants to enhance heavy metal tolerance as well as accumulation.

5.3 Conversion of metals and metalloids to less toxic and volatile forms

There are several reports for developing phytoremediation strategies for heavy metals with the help of biotechnological interventions by conversion of these metals to less toxic and volatile forms. It is observed that many organisms, including bacteria, fungi, and animals, methylate arsenic. Methylated arsenic have been discovered in several plant species, including rice grain [100, 101], and suggest that this is the process is a result of endogenous methylation by the plants themselves. The final product of this pathway is the gas trimethylarsine (TMAs(III)), that can be volatilized from the plant. Qin et al. [102] have cloned a gene encoding an As(III)-S-adenosylmethionine methyltransferase (arsM) from the soil bacterium Rhodopseudomonas palustris. Expression of the arsM gene in an arsenic-sensitive strain of E. coli that resulted in the biosynthesis of several methylated forms of arsenic, including volatile TMAs(III) and conferred arsenic tolerance in the plants. These findings show that the expression of the single methyltransferase (arsM) gene is sufficient to produce both volatilization and tolerance to arsenic (As). A gene for an ArsM homolog in a primitive plant, the eukaryotic alga Cyanidioschyzon merolae has been idenfied [103]. Cells expressing CmArsM methylates As(III), as like the purified enzyme. In a rice microarray study, a putative gene annotated as a methyltransferase was found to be upregulated upon exposure to arsenate in the growth solution [104]. These findings indicate the possibility of engineering arsenic volatilization for the phytoremediation of arsenic-contaminated water and soil and also to improve the safety of the food supply.


6. Conclusions

Contamination of soils and water by arsenic is one the serious threat for food security and human health in throughout the world. Some severe skin and other diseases occur due to continuous consumption of As contaminated foods and water. This necessitates a suitable technology to handle arsenic contaminated water carefully, so that above mentions points can be satisfied. Phytoremediation of arsenic contaminated water by aquatic and semi aquatic weeds offers low cost, economically feasible and eco-friendly technology to remove arsenic from contaminated water for long term. Some weeds have tremendous potential to accumulate higher amount of arsenic in their plant parts such as Eichhornia crassipes, Hydrilla verticillata, Spirodella polyrhiza, Arundo donax and Vetivaria spp. More specifically semi aquatic weeds like Arundo donax and Vetivaria sp. (perennial) can be used with in combination with Eicchornia, Spirodella and Hydrilla to remove arsenic more efficiently from treatment tanks or constructed wetland system. Although management of plant biomass will be another concern for disposal, but these plant materials can be used for making fiber (water hyacinth), handcraft items (Arundo and Typha stems) and biofuel purpose. Moreover, with advancement of molecular genetics in future As tolerance genes can be transferred to food crops (specially rice) which can store huge amount of As in their roots or very low transfer co-efficient from root to grain so that transgenic rice crops will able to grow using As contaminated water and contribute in food security in upcoming days.


  1. 1. Shukla A, Srivastava S. A review of phytoremediation prospects for arsenic contaminated water and soil. Phytomanagement of polluted sites. 2019 Jan 1:243-54
  2. 2. Bhattacharyya R, Chatterjee D, Nath B, Jana J, Jacks G, Vahter M. High arsenic groundwater: mobilization, metabolism and mitigation–an overview in the Bengal Delta Plain. Molecular and cellular biochemistry. 2003 Nov; 253(1):347-55
  3. 3. Shaji E, Santosh M, Sarath KV, Prakash P, Deepchand V, Divya BV. Arsenic contamination of groundwater: A global synopsis with focus on the Indian Peninsula. Geoscience Frontiers. 2020 Oct 1
  4. 4. Srivastava S, Suprasanna P, D’souza SF. Mechanisms of arsenic tolerance and detoxification in plants and their application in transgenic technology: a critical appraisal. International journal of phytoremediation. 2012 May 1;14(5):506-17
  5. 5. Saha D, Sahu S. A decade of investigations on groundwater arsenic contamination in Middle Ganga Plain, India. Environmental geochemistry and health. 2016 Apr 1;38(2):315-37
  6. 6. Mukherjee AB, Bhattacharya P, Jacks G, Banerjee DM, Ramanathan AL, Chandan M, Chandrashekharam D, Debashis C, Naidu R. Groundwater arsenic contamination in India: extent and severity. CSIRO Publishing; 2006
  7. 7. Tuli R, Chakrabarty D, Trivedi PK, Tripathi RD. Recent advances in arsenic accumulation and metabolism in rice. Molecular Breeding. 2010 Aug; 26(2):307-23
  8. 8. Spognardi S, Bravo I, Beni C, Menegoni P, Pietrelli L, Papetti P. Arsenic accumulation in edible vegetables and health risk reduction by groundwater treatment using an adsorption process. Environmental Science and Pollution Research. 2019 Nov; 26(31):32505-16
  9. 9. Awasthi S, Chauhan R, Srivastava S, Tripathi RD. The journey of arsenic from soil to grain in rice. Frontiers in Plant Science. 2017 Jun 20; 8:1007
  10. 10. Rahman MA, Hasegawa H. Aquatic arsenic: phytoremediation using floating macrophytes. Chemosphere. 2011 Apr 1;83(5):633-46
  11. 11. Nazir A, Malik RN, Ajaib M, Khan N, Siddiqui MF. Hyperaccumulators of heavy metals of industrial areas of Islamabad and Rawalpindi. Pak J Bot. 2011 Aug 1;43(4):1925-33
  12. 12. Ma LQ, Komar KM, Tu C, Zhang W, Cai Y, Kennelley ED. A fern that hyperaccumulates arsenic. Nature. 2001 Feb;409(6820):579-.579
  13. 13. Alvarado S, Guédez M, Lué-Merú MP, Nelson G, Alvaro A, Jesús AC, Gyula Z. Arsenic removal from waters by bioremediation with the aquatic plants Water Hyacinth (Eichhornia crassipes) and Lesser Duckweed (Lemna minor). Bioresource technology. 2008 Nov 1;99(17):8436-40
  14. 14. Rahman MA, Hasegawa H, Ueda K, Maki T, Rahman MM. Arsenic uptake by aquatic macrophyte Spirodela polyrhiza L.: Interactions with phosphate and iron. Journal of hazardous materials. 2008 Dec 30; 160(2-3):356-61
  15. 15. Roy C, Jahan M, Rahman S. Characterization and treatment of textile wastewater by aquatic plants (macrophytes) and algae. European Journal of Sustainable Development Research. 2018; 2(3):29
  16. 16. Mirza N, Mahmood Q, Pervez A, Ahmad R, Farooq R, Shah MM, Azim MR. Phytoremediation potential of Arundo donax in arsenic-contaminated synthetic wastewater. Bioresource technology. 2010 Aug 1;101(15):5815-9
  17. 17. Mirza N, Mubarak H, Chai LY, Yong W, Khan MJ, Khan QU, Hashmi MZ, Farooq U, Sarwar R, Yang ZH. The potential use of Vetiveria zizanioides for the phytoremediation of antimony, arsenic and their co-contamination. Bulletin of environmental contamination and toxicology. 2017 Oct;99(4):511-7
  18. 18. Chaney, R.L., 1983. Plant uptake of inorganic waste constituents. In: Parr, J.F.E.A. (Ed.), Land Treatment of Hazardous Wastes. Noyes Data Corp, Park Ridge, NJ, pp. 50-76
  19. 19. Ebel M, Evangelou MW, Schaeffer A. Cyanide phytoremediation by water hyacinths (Eichhornia crassipes). Chemosphere. 2007 Jan 1;66(5):816-23
  20. 20. Misbahuddin, M.I.R. and Fariduddin, A.T.M., 2002. Water hyacinth removes arsenic from arsenic-contaminated drinking water. Archives of Environmental Health: An International Journal, 57(6), pp.516-518
  21. 21. Al Rmalli SW, Harrington CF, Ayub M, Haris PI. A biomaterial based approach for arsenic removal from water. Journal of environmental monitoring. 2005;7(4):279-82
  22. 22. Mishra, V.K., Upadhyay, A.R., Pathak, V. and Tripathi, B.D., 2008. Phytoremediation of mercury and arsenic from tropical opencast coalmine effluent through naturally occurring aquatic macrophytes. Water, air, and soil pollution, 192(1), pp.303-314
  23. 23. Taleei MM, Ghomi NK, Jozi SA. Arsenic removal of contaminated soils by phytoremediation of vetiver grass, chara algae and water hyacinth. Bulletin of environmental contamination and toxicology. 2019 Jan 15;102(1):134-9
  24. 24. Islam A, Saha PK, Iqbal M, Islam MN, Nayeem M. Removal of arsenic by water hyacinth from arsenic contaminated water. Water Int. 2016;1(2):36-41
  25. 25. Rodrigues AC, do Amaral Sobrinho NM, dos Santos FS, dos Santos AM, Pereira AC, Lima ES. Biosorption of toxic metals by water lettuce (Pistia stratiotes) biomass. Water, Air, & Soil Pollution. 2017 Apr 1;228(4):156
  26. 26. Zhou YQ, Li SY, Shi YD, Lv W, Shen TB, Huang QL, Li YK, Wu ZL. Phytoremediation of Chromium and Lead Using Water Lettuce Pistia stratiotes L. InApplied Mechanics and Materials 2013 (Vol. 401, pp. 2071-2075). Trans Tech Publications Ltd
  27. 27. Odjegba VJ, Fasidi IO. Accumulation of trace elements by Pistia stratiotes: implications for phytoremediation. Ecotoxicology. 2004 Oct;13(7):637-46
  28. 28. Lee CK, Low KS, Hew NS. Accumulation of arsenic by aquatic plants. Science of the total environment. 1991 Apr 15;103(2-3):215-27
  29. 29. Basu A, Kumar S, Mukherjee S. Arsenic reduction from aqueous environment by water lettuce (Pistia stratiotes L.). Indian Journal of Environmental Health. 2003 Apr 1;45(2):143-50
  30. 30. Farnese FD, Oliveira JA, Lima FS, Leão GA, Gusman GS, Silva LC. Evaluation of the potential of Pistia stratiotes L.(water lettuce) for bioindication and phytoremediation of aquatic environments contaminated with arsenic. Brazilian Journal of Biology. 2014 Aug;74(3):S108-12
  31. 31. De Campos FV, de Oliveira JA, da Silva AA, Ribeiro C, dos Santos Farnese F. Phytoremediation of arsenite-contaminated environments: is Pistia stratiotes L. a useful tool?. Ecological Indicators. 2019 Sep 1;104:794-801
  32. 32. Mkandawire M, Dudel EG. Accumulation of arsenic in Lemna gibba L. (duckweed) in tailing waters of two abandoned uranium mining sites in Saxony, Germany. Science of the Total Environment. 2005 Jan 5;336(1-3):81-9
  33. 33. Rahman MA, Hasegawa H, Ueda K, Maki T, Okumura C, Rahman MM. Arsenic accumulation in duckweed (Spirodela polyrhiza L.): a good option for phytoremediation. Chemosphere. 2007 Sep 1;69(3):493-9
  34. 34. Duman F, Ozturk F, Aydin Z. Biological responses of duckweed (Lemna minor L.) exposed to the inorganic arsenic species As (III) and As (V): effects of concentration and duration of exposure. Ecotoxicology. 2010 Jun;19(5):983-93
  35. 35. Zhang X, Hu Y, Liu Y, Chen B. Arsenic uptake, accumulation and phytofiltration by duckweed (Spirodela polyrhiza L.). Journal of environmental sciences. 2011 Apr 1;23(4):601-6
  36. 36. Favas PJ, Pratas J, Prasad MN. Accumulation of arsenic by aquatic plants in large-scale field conditions: opportunities for phytoremediation and bioindication. Science of the total Environment. 2012 Sep 1;433:390-7
  37. 37. Zhang X, Zhao FJ, Huang Q, Williams PN, Sun GX, Zhu YG. Arsenic uptake and speciation in the rootless duckweed Wolffia globosa. New Phytologist. 2009 Apr;182(2):421-8
  38. 38. Zhang X, Uroic MK, Xie WY, Zhu YG, Chen BD, McGrath SP, Feldmann J, Zhao FJ. Phytochelatins play a key role in arsenic accumulation and tolerance in the aquatic macrophyte Wolffia globosa. Environmental Pollution. 2012 Jun 1;165:18-24
  39. 39. Da Silva AA, Oliveira JA, Campos FV, Ribeiro C, Farnese FD. Role of glutathione in tolerance to arsenite in Salvinia molesta, an aquatic fern. Acta Botanica Brasilica. 2017 Dec;31(4):657-64
  40. 40. Hoffmann T, Kutter C, Santamaria J. Capacity of Salvinia minima Baker to tolerate and accumulate As and Pb. Engineering in Life Sciences. 2004 Feb 5;4(1):61-5
  41. 41. Rahman MA, Hasegawa H, Ueda K, Maki T, Rahman MM. Influence of phosphate and iron ions in selective uptake of arsenic species by water fern (Salvinia natans L.). Chemical Engineering Journal. 2008 Dec 15;145(2):179-84
  42. 42. Sood A, Uniyal PL, Prasanna R, Ahluwalia AS. Phytoremediation potential of aquatic macrophyte, Azolla. Ambio. 2012 Mar;41(2):122-37
  43. 43. Pandey VC. Phytoremediation of heavy metals from fly ash pond by Azolla caroliniana. Ecotoxicology and Environmental Safety. 2012 Aug 1;82:8-12
  44. 44. Rai PK. Phytoremediation of Hg and Cd from industrial effluents using an aquatic free floating macrophyte Azolla pinnata. International journal of phytoremediation. 2008 Jul 23;10(5):430-9
  45. 45. Mahmud R, Inoue N, Kasajima SY, Shaheen R. Assessment of potential indigenous plant species for the phytoremediation of arsenic-contaminated areas of Bangladesh. International Journal of Phytoremediation. 2008 Apr 3;10(2):119-32
  46. 46. Rofkar JR, Dwyer DF, Bobak DM. Uptake and toxicity of arsenic, copper, and silicon in Azolla caroliniana and Lemna minor. International journal of phytoremediation. 2014 Feb 1;16(2):155-66
  47. 47. Zhang X, Lin AJ, Zhao FJ, Xu GZ, Duan GL, Zhu YG. Arsenic accumulation by the aquatic fern Azolla: comparison of arsenate uptake, speciation and efflux by A. caroliniana and A. filiculoides. Environmental Pollution. 2008 Dec 1;156(3):1149-55
  48. 48. Srivastava S, Sounderajan S, Udas A, Suprasanna P. Effect of combinations of aquatic plants (Hydrilla, Ceratophyllum, Eichhornia, Lemna and Wolffia) on arsenic removal in field conditions. Ecological engineering. 2014 Dec 1;73:297-301
  49. 49. Srivastava S, Mishra S, Dwivedi S, Tripathi RD. Role of thiol metabolism in arsenic detoxification in Hydrilla verticillata (Lf) Royle. Water, Air, & Soil Pollution. 2010 Oct;212(1):155-65
  50. 50. Khang HV, Hatayama M, Inoue C. Arsenic accumulation by aquatic macrophyte coontail (Ceratophyllum demersum L.) exposed to arsenite, and the effect of iron on the uptake of arsenite and arsenate. Environmental and experimental botany. 2012 Nov 1;83:47-52
  51. 51. Chen G, Liu X, Brookes PC, Xu J. Opportunities for phytoremediation and bioindication of arsenic contaminated water using a submerged aquatic plant: Vallisneria natans (Lour.) Hara. International journal of phytoremediation. 2015 Mar 4;17(3):249-55
  52. 52. Norouznia H, Hamidian AH. Phytoremediation efficiency of pondweed (Potamogeton crispus) in removing heavy metals (Cu, Cr, Pb, As and Cd) from water of Anzali wetland. International Journal of Aquatic Biology. 2014 Sep 10;2(4):206-14
  53. 53. Krayem M, Baydoun M, Deluchat V, Lenain JF, Kazpard V, Labrousse P. Absorption and translocation of copper and arsenic in an aquatic macrophyte Myriophyllum alterniflorum DC. in oligotrophic and eutrophic conditions. Environmental Science and Pollution Research. 2016 Jun;23(11):11129-36
  54. 54. Li B, Gu B, Yang Z, Zhang T. The role of submerged macrophytes in phytoremediation of arsenic from contaminated water: A case study on Vallisneria natans (Lour.) Hara. Ecotoxicology and environmental safety. 2018 Dec 15;165:224-31
  55. 55. Datta R, Quispe MA, Sarkar D. Greenhouse study on the phytoremediation potential of vetiver grass, Chrysopogon zizanioides L., in arsenic-contaminated soils. Bulletin of environmental contamination and toxicology. 2011 Jan 1;86(1):124-8
  56. 56. Jomjun N, Siripen T, Maliwan S, Jintapat N, Prasak T, Somporn C, Petch P. Phytoremediation of arsenic in submerged soil by wetland plants. International journal of phytoremediation. 2010 Nov 18;13(1):35-46
  57. 57. Raj A, Jamil S, Srivastava PK, Tripathi RD, Sharma YK, Singh N. Feasibility Study of Phragmites karka and Christella dentata Grown in West Bengal as Arsenic Accumulator. International journal of phytoremediation. 2015 Sep 2;17(9):869-78
  58. 58. Guarino F, Miranda A, Castiglione S, Cicatelli A. Arsenic phytovolatilization and epigenetic modifications in Arundo donax L. assisted by a PGPR consortium. Chemosphere. 2020 Jul 1;251:126310
  59. 59. Simmons ZD, Suleiman AA, Theegala CS. Phytoremediation of arsenic and lead using alligator weed (Alternathera philoxeroides). Transactions of the ASABE. 2007;50(5):1895-900
  60. 60. Sharma P, Tripathi S, Chandra R. Highly efficient phytoremediation potential of metal and metalloids from the pulp paper industry waste employing Eclipta alba (L) and Alternanthera philoxeroide (L): Biosorption and pollution reduction. Bioresource Technology. 2021 Jan 1;319:124147
  61. 61. Ghassemzadeh F, Yousefzadeh H, Arbab-Zavar MH. Arsenic phytoremediation by Phragmites australis: green technology. International journal of environmental studies. 2008 Aug 1;65(4):587-94
  62. 62. Caporale AG, Sarkar D, Datta R, Punamiya P, Violante A. Effect of arbuscular mycorrhizal fungi (Glomus spp.) on growth and arsenic uptake of vetiver grass (Chrysopogon zizanioides L.) from contaminated soil and water systems. Journal of soil science and plant nutrition. 2014 Dec;14(4):955-72
  63. 63. Tripathi RD, Srivastava S, Mishra S, Singh N, Tuli R, Gupta DK, Maathuis FJ. Arsenic hazards: strategies for tolerance and remediation by plants. Trends in biotechnology. 2007 Apr 1;25(4):158-65
  64. 64. Zhao FJ, Ma JF, Meharg AA, McGrath SP. Arsenic uptake and metabolism in plants. New Phytologist. 2009 Mar;181(4):777-94
  65. 65. Mkandawire M, Lyubun YV, Kosterin PV, Dudel EG. Toxicity of arsenic species to Lemna gibba L. and the influence of phosphate on arsenic bioavailability. Environmental Toxicology: An International Journal. 2004 Feb;19(1):26-34
  66. 66. Abedin MJ, Feldmann J, Meharg AA. Uptake kinetics of arsenic species in rice plants. Plant physiology. 2002 Mar 1;128(3):1120-8
  67. 67. Meharg AA, Jardine L. Arsenite transport into paddy rice (Oryza sativa) roots. New phytologist. 2003 Jan;157(1):39-44
  68. 68. Ma JF, Yamaji N, Mitani N, Xu XY, Su YH, McGrath SP, Zhao FJ. Transporters of arsenite in rice and their role in arsenic accumulation in rice grain. Proceedings of the National Academy of Sciences. 2008 Jul 22;105(29):9931-5
  69. 69. Benga G. Water channel proteins (later called aquaporins) and relatives: past, present, and future. IUBMB life. 2009 Feb;61(2):112-33
  70. 70. Robinson B, Kim N, Marchetti M, Moni C, Schroeter L, van den Dijssel C, Milne G, Clothier B. Arsenic hyperaccumulation by aquatic macrophytes in the Taupo Volcanic Zone, New Zealand. Environmental and Experimental Botany. 2006 Dec 1;58(1-3):206-15
  71. 71. Srivastava S, Mishra S, Tripathi RD, Dwivedi S, Trivedi PK, Tandon PK. Phytochelatins and antioxidant systems respond differentially during arsenite and arsenate stress in Hydrilla verticillata (Lf) Royle. Environmental science & technology. 2007 Apr 15;41(8):2930-6
  72. 72. Raab A, Ferreira K, Meharg AA, Feldmann J. Can arsenic–phytochelatin complex formation be used as an indicator for toxicity in Helianthus annuus?. Journal of Experimental Botany. 2007 Apr 1;58(6):1333-8
  73. 73. Delnomdedieu M, Basti MM, Otvos JD, Thomas DJ. Reduction and binding of arsenate and dimethylarsinate by glutathione: a magnetic resonance study. Chemico-biological interactions. 1994 Feb 1;90(2):139-55
  74. 74. Bleeker PM, Hakvoort HW, Bliek M, Souer E, Schat H. Enhanced arsenate reduction by a CDC25-like tyrosine phosphatase explains increased phytochelatin accumulation in arsenate-tolerant Holcus lanatus. The Plant Journal. 2006 Mar;45(6):917-29
  75. 75. Meharg AA, Hartley-Whitaker J. Arsenic uptake and metabolism in arsenic resistant and nonresistant plant species. New Phytologist. 2002 Apr;154(1):29-43
  76. 76. Mittler R. Oxidative stress, antioxidants and stress tolerance. Trends in plant science. 2002 Sep 1;7(9):405-10
  77. 77. Dhankher OP, Pilon-Smits EA, Meagher RB, Doty S. Biotechnological approaches for phytoremediation. InPlant biotechnology and agriculture 2012 Jan 1 (pp. 309-328). Academic Press
  78. 78. Kotrba P, Najmanova J, Macek T, Ruml T, Mackova M. Genetically modified plants in phytoremediation of heavy metal and metalloid soil and sediment pollution. Biotechnology advances. 2009 Nov 1;27(6):799-810
  79. 79. Sunkar R, Kaplan B, Bouché N, Arazi T, Dolev D, Talke IN, Maathuis FJ, Sanders D, Bouchez D, Fromm H. Expression of a truncated tobacco NtCBP4 channel in transgenic plants and disruption of the homologous Arabidopsis CNGC1 gene confer Pb2+ tolerance. The Plant Journal. 2000 Nov;24(4):533-42
  80. 80. Hirschi KD, Korenkov VD, Wilganowski NL, Wagner GJ. Expression of Arabidopsis CAX2 in tobacco. Altered metal accumulation and increased manganese tolerance. Plant physiology. 2000 Sep 1;124(1):125-34
  81. 81. Zeng H, Xu L, Singh A, Wang H, Du L, Poovaiah BW. Involvement of calmodulin and calmodulin-like proteins in plant responses to abiotic stresses. Frontiers in plant science. 2015 Aug 11;6:600
  82. 82. Song WY, Sohn EJ, Martinoia E, Lee YJ, Yang YY, Jasinski M, Forestier C, Hwang I, Lee Y. Engineering tolerance and accumulation of lead and cadmium in transgenic plants. Nature biotechnology. 2003 Aug;21(8):914-9
  83. 83. Bienert GP, Thorsen M, Schüssler MD, Nilsson HR, Wagner A, Tamás MJ, Jahn TP. A subgroup of plant aquaporins facilitate the bi-directional diffusion of As (OH) 3 and Sb (OH) 3 across membranes. BMC biology. 2008 Dec;6(1):1-5
  84. 84. Mosa KA, Kumar K, Chhikara S, Mcdermott J, Liu Z, Musante C, White JC, Dhankher OP. Members of rice plasma membrane intrinsic proteins subfamily are involved in arsenite permeability and tolerance in plants. Transgenic research. 2012 Dec 1;21(6):1265-77
  85. 85. Xu XY, McGrath SP, Zhao FJ. Rapid reduction of arsenate in the medium mediated by plant roots. New Phytologist. 2007 Nov;176(3):590-9
  86. 86. Duan GL, Zhu YG, Tong YP, Cai C, Kneer R. Characterization of arsenate reductase in the extract of roots and fronds of Chinese brake fern, an arsenic hyperaccumulator. Plant Physiology. 2005 May 1;138(1):461-9
  87. 87. Ma JF, Tamai K, Ichii M, Wu GF. A rice mutant defective in Si uptake. Plant Physiology. 2002 Dec 1;130(4):2111-7
  88. 88. Ma JF, Tamai K, Yamaji N, Mitani N, Konishi S, Katsuhara M, Ishiguro M, Murata Y, Yano M. A silicon transporter in rice. Nature. 2006 Mar;440(7084):688-91
  89. 89. Meng YL, Liu Z, Rosen BP. As (III) and Sb (III) uptake by GlpF and efflux by ArsB in Escherichia coli. Journal of Biological Chemistry. 2004 Apr 30;279(18):18334-41
  90. 90. Dubey S, Shri M, Misra P, Lakhwani D, Bag SK, Asif MH, Trivedi PK, Tripathi RD, Chakrabarty D. Heavy metals induce oxidative stress and genome-wide modulation in transcriptome of rice root. Functional & integrative genomics. 2014 Jun;14(2):401-17
  91. 91. Wang Y, Dong C, Xue Z, Jin Q, Xu Y. De novo transcriptome sequencing and discovery of genes related to copper tolerance in Paeonia ostii. Gene. 2016 Jan 15;576(1):126-35
  92. 92. Lu YP, Li ZS, Rea PA. AtMRP1 gene of Arabidopsis encodes a glutathione S-conjugate pump: isolation and functional definition of a plant ATP-binding cassette transporter gene. Proceedings of the National Academy of Sciences. 1997 Jul 22;94(15):8243-8
  93. 93. Tommasini R, Vogt E, Fromenteau M, Hörtensteiner S, Matile P, Amrhein N, Martinoia E. An ABC-transporter of Arabidopsis thaliana has both glutathione-conjugate and chlorophyll catabolite transport activity. The Plant Journal. 1998 Mar;13(6):773-80
  94. 94. Gasic K, Korban SS. Transgenic Indian mustard (Brassica juncea) plants expressing an Arabidopsis phytochelatin synthase (AtPCS1) exhibit enhanced As and Cd tolerance. Plant molecular biology. 2007 Jul;64(4):361-9
  95. 95. Guo J, Dai X, Xu W, Ma M. Overexpressing GSH1 and AsPCS1 simultaneously increases the tolerance and accumulation of cadmium and arsenic in Arabidopsis thaliana. Chemosphere. 2008 Jul 1;72(7):1020-6
  96. 96. Dhankher OP, Li Y, Rosen BP, Shi J, Salt D, Senecoff JF, Sashti NA, Meagher RB. Engineering tolerance and hyperaccumulation of arsenic in plants by combining arsenate reductase and γ-glutamylcysteine synthetase expression. Nature biotechnology. 2002 Nov;20(11):1140-5
  97. 97. Li Y, Dhankher OP, Carreira L, Lee D, Chen A, Schroeder JI, Balish RS, Meagher RB. Overexpression of phytochelatin synthase in Arabidopsis leads to enhanced arsenic tolerance and cadmium hypersensitivity. Plant and Cell Physiology. 2004 Dec 15;45(12):1787-97
  98. 98. Xu L, Wang Y, Liu W, Wang J, Zhu X, Zhang K, Yu R, Wang R, Xie Y, Zhang W, Gong Y. De novo sequencing of root transcriptome reveals complex cadmium-responsive regulatory networks in radish (Raphanus sativus L.). Plant Science. 2015 Jul 1;236:313-23
  99. 99. Xie Y, Ye S, Wang Y, Xu L, Zhu X, Yang J, Feng H, Yu R, Karanja B, Gong Y, Liu L. Transcriptome-based gene profiling provides novel insights into the characteristics of radish root response to Cr stress with next-generation sequencing. Frontiers in plant science. 2015 Mar 31;6:202
  100. 100. Williams PN, Price AH, Raab A, Hossain SA, Feldmann J, Meharg AA. Variation in arsenic speciation and concentration in paddy rice related to dietary exposure. Environmental science & technology. 2005 Aug 1;39(15):5531-40
  101. 101. Zhu YG, Sun GX, Lei M, Teng M, Liu YX, Chen NC, Wang LH, Carey AM, Deacon C, Raab A, Meharg AA. High percentage inorganic arsenic content of mining impacted and nonimpacted Chinese rice. Environmental science & technology. 2008 Jul 1;42(13):5008-13
  102. 102. Qin J, Rosen BP, Zhang Y, Wang G, Franke S, Rensing C. Arsenic detoxification and evolution of trimethylarsine gas by a microbial arsenite S-adenosylmethionine methyltransferase. Proceedings of the National Academy of Sciences. 2006 Feb 14;103(7):2075-80
  103. 103. Qin J, Lehr CR, Yuan C, Le XC, McDermott TR, Rosen BP. Biotransformation of arsenic by a Yellowstone thermoacidophilic eukaryotic alga. Proceedings of the National Academy of Sciences. 2009 Mar 31;106 (13):5213-7
  104. 104. Norton GJ, Lou-Hing DE, Meharg AA, Price AH. Rice–arsenate interactions in hydroponics: whole genome transcriptional analysis. Journal of experimental botany. 2008 May 1;59(8):2267-76

Written By

Dibakar Roy, Dasari Sreekanth, Deepak Pawar, Himanshu Mahawar and Kamal K. Barman

Submitted: 07 June 2021 Reviewed: 17 June 2021 Published: 07 August 2021